Recent Trends in Nucleotide Synthesis - Chemical Reviews (ACS

Review pubs.acs.org/CR

Recent Trends in Nucleotide Synthesis Béatrice Roy, Anaïs Depaix, Christian Périgaud, and Suzanne Peyrottes*

Chem. Rev. 2016.116:7854-7897. Downloaded from pubs.acs.org by UNIV OF SUNDERLAND on 09/28/18. For personal use only.

Institut des Biomolécules Max Mousseron (IBMM), UMR 5247 CNRS, Université de Montpellier, ENSCM, Campus Triolet, cc 1705, Place Eugène Bataillon, 34095 Montpellier cedex 5, France ABSTRACT: Focusing on the recent literature (since 2000), this review outlines the main synthetic approaches for the preparation of 5′-mono-, 5′-di-, and 5′-triphosphorylated nucleosides, also known as nucleotides, as well as several derivatives, namely, cyclic nucleotides and dinucleotides, dinucleoside 5′,5′-polyphosphates, sugar nucleotides, and nucleolipids. Endogenous nucleotides and their analogues can be obtained enzymatically, which is often restricted to natural substrates, or chemically. In chemical synthesis, protected or unprotected nucleosides can be used as the starting material, depending on the nature of the reagents selected from P(III) or P(V) species. Both solution-phase and solid-support syntheses have been developed and are reported here. Although a considerable amount of research has been conducted in this field, further work is required because chemists are still faced with the challenge of developing a universal methodology that is compatible with a large variety of nucleoside analogues.

CONTENTS 1. Introduction 2. Structural Features and Properties of Nucleotides 2.1. Structural and Chemical Properties 2.1.1. Structure and Conformation 2.1.2. Acid and Base Properties 2.1.3. Chemical Stability 2.2. Analysis 2.3. Biological Applications 3. General Considerations 3.1. Phosphorus 3.2. Purification of Nucleotides 3.3. Solid-Phase and Polymer-Assisted Nucleotide Synthesis 4. Nucleoside 5′-Monophosphates 4.1. Solution-Phase Synthesis 4.1.1. Synthesis via a Phosphorodichloridate Intermediate 4.1.2. Synthesis via a Phosphoramidate Intermediate 4.1.3. Synthesis via a Phosphodiester Intermediate 4.1.4. Synthesis via a Phosphotriester Intermediate 4.1.5. Synthesis via a 5′-H-Phosphonate Intermediate 4.2. Polymer-Supported Synthesis 4.2.1. Synthesis Involving a Polymer-Bound Reagent 4.2.2. Synthesis Involving Attachment of the Sugar Moiety to the Support 4.2.3. Synthesis Involving Attachment of the Base Moiety to the Support 4.3. Enzymatic Synthesis 5. Nucleoside 5′-Diphosphates © 2016 American Chemical Society

7868

5.1. Solution-Phase Synthesis 5.1.1. Synthesis via a Phosphorodichloridate Intermediate 5.1.2. Synthesis via a Phosphoramidate Intermediate 5.1.3. Synthesis via a Tosylate Intermediate 5.1.4. Synthesis via a Mixed P(III)−P(V) Intermediate 5.1.5. Synthesis via a Phosphotriester Intermediate 5.2. Polymer-Supported Synthesis 5.2.1. Synthesis Involving a Polymer-Bound Reagent 5.2.2. Synthesis Involving Attachment of the Sugar Moiety to the Support 5.2.3. Synthesis Involving Attachment of the Base Moiety to the Support 6. Nucleoside 5′-Triphosphates 6.1. Solution-Phase Synthesis 6.1.1. Synthesis via a Phosphorodichloridate Intermediate 6.1.2. Synthesis via a Phosphoramidate Intermediate 6.1.3. Synthesis via a Mixed P(III)−P(V) Intermediate 6.1.4. Synthesis via a Phosphotriester Intermediate 6.1.5. Synthesis via a Phosphosulfonyl Intermediate 6.2. Solid-Supported Synthesis 6.2.1. Synthesis Involving a Polymer-Bound Reagent

7868 7869 7870

Received: March 14, 2016 Published: June 20, 2016

7855 7857 7857 7857 7857 7858 7858 7861 7861 7861 7861 7863 7863 7863 7863 7864 7864 7864 7867 7868 7868

7854

7870 7870 7870 7871 7871 7871 7872 7872 7872 7874 7874 7876 7876 7877 7878 7880 7880 7881 7881

DOI: 10.1021/acs.chemrev.6b00174 Chem. Rev. 2016, 116, 7854−7897

Chemical Reviews

Review

Figure 1. General structures of natural nucleobases, nucleotides, and some derivatives.

6.2.2. Synthesis Involving Attachment of the Sugar Moiety to the Support 6.2.3. Synthesis Involving Attachment of the Base Moiety to the Support 6.3. Enzymatic Synthesis 7. Miscellaneous 7.1. Cyclic Nucleotides 7.2. Cyclic Dinucleotides 7.3. Dinucleoside 5′,5′-Polyphosphates 7.4. Sugar Nucleotides 7.5. Nucleolipids 8. Conclusions Author Information Corresponding Author Notes Biographies Acknowledgments Abbreviations References

1. INTRODUCTION Nucleotides, such as 5′-mono- and 5′-polyphosphorylated nucleosides, and their conjugates are essential biomolecules that play key functional and structural roles in biological systems (Figure 1, Table 1). As an example, they provide the fundamental building blocks in the polymerase-mediated synthesis of nucleic acids. The structural feature common to all of these compounds is the presence of one or two nucleosides that are attached to one or more phosphate groups, with phosphorus in the oxidation state +5. The most versatile nucleotide is adenosine 5′triphosphate (ATP). It is the primary energy source for cellular functions. Indeed, many reactions that occur in the cell, which range from metabolic transformations to signaling events, are coupled to the hydrolysis of ATP. It is remarkable that the human body turns over its own body weight equivalent in ATP each day.1 In addition to serving as the major energy currency of cells, ATP also acts as an important allosteric effector in the regulation of cell metabolism. Cyclic mononucleotides (cNMPs) are single-phosphatecontaining compounds characterized by an intramolecular phosphodiester bond between the phosphorus atom and the

7881 7883 7883 7884 7884 7884 7884 7886 7888 7889 7889 7889 7889 7889 7890 7890 7890

7855


Chemical Reviews

Review

Table 1. Biological Functions of Natural Nucleotides and Their Conjugates in Humans compounds nucleotidesa (d)NMPs, (d)NDPs (d)NTPs

cyclic nucleotides and cyclic dinucleotides dinucleoside 5′,5′-polyphosphatesb nicotinamide mononucleotides flavin mononucleotides sugar nucleotides

role

purpose

substrates for nucleotide kinases35 signaling molecules (ADP, UDP)36−38 substrates for DNA or RNA polymerases protein regulators35 signaling molecules (ATP, UTP)36−38 cofactors (ATP, UTP)35,39 energy-rich carriers (ATP, GTP) secondary messengers2,5,40 mediators of the purinergic system3,4 signaling molecules (Ap4A)37 enzyme cofactors (NAD, NADH, NADP, NADPH) enzyme cofactors (FAD, FADH2) glycosyl donors for glycosyl transferases9,10 substrates for UDP-galactose 4-epimerase41 intermediates of carbohydrate metabolism

nucleolipidc

signaling molecules (UDP glucose)36−38 intermediates of lipid metabolism (CDP-DAG)12

(d)NTP synthesis activation of G protein-coupled membrane receptors storage and transmission of genetic information (replication/transcription) (d)NTP pool homeostasis, control of cell proliferation activation of G protein-coupled membrane receptors transfer of a phosphoryl group to an acceptor molecule energy supply in biochemical reactions signal transduction activation of cAMP-dependent protein kinase (PKA) impact on the physiology and pathology of cardiovascular systems activation of G protein-coupled membrane receptors act in redox processes act in redox processes biosynthesis of oligo- and polysaccharides glycosylation of proteins and lipids interconversion of glucosyl and galactosyl groups biosynthesis of deoxysugars, aminodeoxysugars, chain-branched sugar and uronic acids activation of G protein-coupled membrane receptors biosynthesis of phospholipids

a

(d)NMPs, (2′-deoxy)ribonucleoside 5′-monophosphates; (d)NDPs, (2′-deoxy)ribonucleoside 5′-diphosphates; (d)NTPs, (2′-deoxy)ribonucleoside 5′-triphosphates; ADP, adenosine 5′-diphosphate; UDP, uridine 5′-diphosphate; ATP, adenosine 5′-triphosphate; UTP, uridine 5′-triphosphate; GTP, guanosine 5′-triphosphate. bAp4A, P1-5′-O-adenosine-P4-5′-O-adenosine tetraphosphate. cCDP-DAG, cytosine 5′diphosphate diacylglycerol.

various hydroxyl groups of the sugar moieties.2 Among them, cyclic adenosine 5′-monophosphate (cAMP) and cyclic guanosine 5′-monophosphate (cGMP) act as second messengers (i.e., intracellular signaling molecules) in signal transduction systems. Second messengers are formed within cells following stimulation with intercellular signaling molecules (first messengers) such as hormones, neurotransmitters, and mediators of inflammation. Cyclic nucleotides other than cAMP and cGMP are known as noncanonical cyclic nucleoside monophosphates because their second-messenger function, which has not yet been firmly established. Dinucleoside 5′,5′-polyphosphates (DNPs), also called dinucleotides, include a group of naturally occurring compounds that incorporate two nucleosides linked by two to seven phosphate groups. These biomolecules are present in humans and other mammalian species and act as strong endogenous agonists of the purinergic system.3,4 Therefore, they have an impact on the cardiovascular system, with physiological consequences such as vasodilator effects, proliferative effects on vascular smooth muscle cells, and platelet antiaggregatory activity. Nicotinamide adenine dinucleotide (NADH/NAD+), nicotinamide adenine dinucleotide phosphate (NADPH/ NADP+), and flavin adenine dinucleotide (FADH2/FAD) are enzyme cofactors in biochemical redox reactions. Strictly speaking, these compounds are not dinucleotides, given that nicotinamide and flavin are not nucleobases. They should be classified as nicotinamide mononucleotide and flavin mononucleotide, respectively. Cyclic dinucleotides (cDNs) are important signaling molecules in bacteria and mammalian cells.5−8 Sugar nucleotides are the activated forms of monosaccharides and act as glycosyl donors for glycosyltransferases in the biosynthesis of oligosaccharides and polysaccharides, as well as in the glycosylation of proteins, lipids, and other cellular

metabolites.9,10 In addition, sugar nucleotides also serve as precursors of deoxysugars, aminodeoxysugars, chain-branched sugars, and uronic acids. In plants and most animals, vitamin C is biosynthesized using sugar nucleotides as starting materials. It is important to note that, in the course of evolution, humans have lost their ability to perform the crucial last step of vitamin C biosynthesis, namely, the conversion of L-gulono-γ-lactone into ascorbic acid, which is catalyzed by the enzyme gulonolactone oxidase.11 Thus, humans need to find their essential supply of vitamin C in their diet. Nucleolipids are a class of amphiphilic compounds that carry lipophilic moieties that are covalently attached to a nucleoside/ nucleotide scaffold.12 The most common nucleolipid is cytidine diphosphate diacylglycerol, a key intermediate for the biosynthesis of glycerophospholipids.13 Recently, nucleolipids have generated widespread interest as supramolecular devices for delivering nucleic acids and drugs.14−19 To investigate biological systems, many natural nucleotides and derivatives have been synthesized either chemically or enzymatically. Structural analogues are also of great interest as potential therapeutic and diagnostic agents, as well as for the study of biochemical and pharmacological processes. In particular, nucleoside 5′-triphosphates are key compounds in genome analysis and medical diagnostics.20−24 Consequently, efficient synthetic methods are of crucial importance for related research fields. However, developing synthetic methods remains a challenge because of the presence of multiple reactive functional groups in nucleosides, sugars, and lipids, which require the introduction of orthogonal protecting groups, in addition to extra time-consuming steps of synthesis. The current review seeks to provide an overview of the methods for the synthesis of nucleotides and some of their conjugates, involving either P(III) or P(V) intermediates, starting from the corresponding nucleosides or their synthetic analogues and 7856


Chemical Reviews

Review

Figure 2. (A,D) Two types of sugar pucker most commonly found in mononucleotides and (B,C) torsion angles χ and γ used to describe the conformations of nucleosides and nucleotides.

(Figure 2).42,43,47,50 First, the glycosyl torsion angle χ (O4′− C1′−N1−C2 for pyrimidine nucleosides and O4′−C1′−N9− C4 for purine nucleosides, Figure 2B and 2C) is related to the rotation about the β-N-glycosidic bond. When the C2 carbonyl of pyrimidines or the N3 of purines lies over the sugar ring, the conformation is called syn; otherwise, it is called anti. In the solid state and in solution, the conformation of natural nucleosides and nucleotides is generally anti.58 The second parameter is the torsion angle γ (O5′−C5′−C4′−C3′), which reflects the position of the 5′-hydroxyl group relative to the C3′ carbon atom (Figure 2B and 2C). Finally, the phase angle of pseudorotation P and the maximum out-of-plane pucker υmax are related to the sugar ring conformation.43,59 In mononucleotides, derivatives containing purine tend to adopt the southern (S, C2′-endo, Figure 2D) conformation, whereas the northern (N, C2′-exo, Figure 2A) conformer is predominant in pyrimidine derivatives.60 Shishkin et al. investigated the conformational equilibrium of natural dNMP using calculations. They concluded that S/anti is the predominant conformation, with the exception of 5′-dGMP, which behaved as an S/syn conformer.61 In biological systems, nucleotides serve as substrates for enzymes in the form of their metal ion complexes. These metals are mostly divalent cations, such as Mg2+, Mn2+, and Zn2+. The dominating conformations in nucleotides have consequences for the metal-ion-binding properties of these compounds, such as the formation of macrochelates.58 Stern et al. performed conformational studies on a series of dinucleoside polyphosphates (NpnN′) at physiological pH using various NMR techniques (i.e., 1H, 13C, and 31P NMR spectroscopies, as well as COSY, HMQC, HMBC, and NOESY 2D experiments).62 Ab initio calculations, supported by NMR data, showed that, in solution, physiologically active dinucleoside polyphosphates are more frequently found in a stacked rather than an extended conformation, and no predominant conformation for the ribose moiety was observed.62 Recently, the Gao research group investigated the conformational behavior and structural flexibility of purine cyclic dinucleotides in aqueous solution, demonstrating that the phosphodiester backbone (either 2′,5′- or 3′,5′-) and sugar puckering affect the overall flexibility of CDNs and, consequently, their binding affinities.63 2.1.2. Acid and Base Properties. The pKa values of the five main nucleobases in nucleotides are listed in Table 2. At physiological pH, they exist almost completely (>99.99%) in the keto and amino tautomeric forms, as shown in Figure 3.42 Using 1H and 13C NMR spectroscopies, Velikyan et al. accurately determined the pKa values of the 2′-hydroxyl group in several nucleosides and nucleotides.66 They showed that the pKa values depend on the ability of the various sugar substituents to

including the acyclic and carbocyclic ones. The strategies for the preparation of nucleoside 5′-mono-, 5′-di-, and 5′-triphosphates; 3′,5′-cyclic nucleotides; dinucleotides; sugar nucleotides; and nucleolipids are described. Since Burgess and Cook’s comprehensive review on NTPs synthesis, which was published in this journal in 2000,25 some aspects of these topics have been covered in several reports and chapters.5,26−34 Our objective is to review the synthesis of these nucleotides from a holistic perspective and highlight recent advances. Therefore, we focus on the methodologies reported since 2000, particularly those involving solidphase and polymer-assisted synthesis. We do not describe the methods for preparing oligonucleotides because they go beyond the scope of this review.

2. STRUCTURAL FEATURES AND PROPERTIES OF NUCLEOTIDES 2.1. Structural and Chemical Properties

2.1.1. Structure and Conformation. Endogenous nucleosides comprise a nitrogen-containing heterocycle, called a nucleobase, connected to a sugar, namely, β-D-ribofuranose or 2′-deoxy-β-D-ribofuranose.42,43 In nucleic acids, the common nucleobases are the purines (adenine and guanine) and the pyrimidines (cytosine; uracil; and thymine, also called 5methyluracil), which are covalently bonded from N1 of pyrimidine or N9 of purine to the anomeric carbon (C1′) of the D-ribose in a β-D configuration. Natural nucleotides incorporate one to three phosphate groups (Pα, Pβ, and Pγ) attached to the hydroxyl group on the C5′ position of the nucleosides (Figure 1). Extensive studies conducted during the 1960s and 1970s showed that nucleosides and nucleotides can adopt many different conformations in solution that are in a rapid dynamic equilibrium. Background information on natural nucleoside conformational studies is available in the literature.44−48 In addition, numerous research groups have been studying the impacts of various modifications/constraints on the puckering preferences of the furanose ring.49−54 Furthering our knowledge of nucleotides’ preferred conformations is important because it could help researchers understand and possibly even predict their interactions with various biological targets. Generally speaking, nucleotides are less flexible than their nucleoside counterparts.55 The conformational behavior of nucleotides can be significantly modified through electrostatic interactions between the nucleobase and the 5′-phosphate group and through the alteration of the intramolecular hydrogen bonds involving the nucleobase and the hydroxyl group in the 5′position.56,57 Three main types of structural data are commonly used to describe the conformational properties of these derivatives 7857


Chemical Reviews

Review

Table 2. pKa Values64 and Spectroscopic Data at pH 765 for Endogenous Nucleoside 5′-Monophosphates compound

pKa

λmax (nm)

ε (mM−1 cm−1)

AMP GMP CMP UMP dTMP

N1, 3.74 N7, 2.40; N1, 9.40 N3, 4.56 N3, 9.50 N3, 10.00

259 252 271 262 267

15.04 14.09 8.74 9.78 9.49

phenomenon. In the absence of a catalyst, the half-life of phosphate monoester dianion hydrolysis is estimated to be 1.1 × 1012 years at 25 °C,75 whereas in the presence of phosphatases, the rate of water attack on the substrate increases by a factor of 1021. Similarly, a kinetic study of the uncatalyzed hydrolysis of dineopentylphosphate (a model compound used to mimic phosphate diesters) at high temperature resulted in an extrapolated half-life of 30 billion years at 25 °C. The rate of hydrolysis increased by a factor of ∼1017 in the presence of staphylococcal nuclease, a phosphodiesterase.76 Therefore, the strong resistance to spontaneous/chemical hydrolysis of phosphodiester bonds contributes to the stability of genes. The mechanisms underlying the spontaneous or enzymatic hydrolysis of phosphate esters have been reviewed in the literature.39,64,77−79 The rate profile of the nonenzymatic hydrolysis of pyrophosphoric acid is a complex function closely related to the pH of the medium. The pyrophosphate bond increases in stability as the number of overall negative charges of the derivative increases. The tetra-anion is the form that is most resistant to hydrolysis.73,74 Nucleoside 5′-phosphates, including triphosphates, are stable only in slightly alkaline solution (around pH 8), whereas they are very sensitive under acidic conditions (pH below 5). This results from the stabilization of the negatively charged phosphate anion and contrasts with esters of carboxylic acids. Compared to nucleoside 5′-polyphosphates, dinucleoside 5′,5′-polyphosphates are more stable and have relatively long half-lives.4,80 For example, DNPs are stable during prolonged dry storage at room temperature, whereas mononucleotides must be stored at 0 °C or below. Mononucleotides slowly degrade in solution at neutral pH or lower, but this is not the case for DNPs.80 In 2010, Huhta et al. performed a kinetic study on the chemical cleavage of nucleoside diphosphate sugars.81 Using ADP-glucose and UDP-glucose as model compounds, they showed that these compounds are fairly stable under neutral conditions, even at high temperatures, and that their decomposition is enhanced by acids and bases.

stabilize the 2′-oxyanion; for example, the pKa value of 2′-OH in AMP (13.38) is greater than that of adenosine (12.17). The pKa values of several phosphate moieties found in biomolecules are indicated in Figure 4. Pyrophosphoric acid corresponds to the anhydride of two orthophosphoric (phosphoric) acid molecules. On the basis of their reported pKa values,67 these inorganic compounds behave as phosphate and pyrophosphate anions at physiological pH. Thus, phosphoric acid can be mono-, di-, or triesterified to give phosphate monoester, diester, or triester derivatives, respectively. Only phosphate monoesters and diesters are naturally occurring, whereas phosphate triesters are exclusively synthetic compounds. In phosphate monoesters such as nucleoside 5′monophosphates, the two ionizable hydroxyl groups near the phosphorus atom have pKa values of 1.6 and 6.6.64 In phosphate diesters, the remaining hydroxyl group is strongly acidic, with pKa ≈ 1.5. It is assumed that nature has chosen the canonical bases because they are not ionized under physiological pH, thus allowing Watson−Crick base pairing.68 Conversely, the phosphate moiety in phosphate diesters is ionized under physiological conditions. This enables the dissolution of nucleic acids in aqueous media, stabilizes the backbone against hydrolysis, and also retains the molecules in the cells because they are trapped by the lipidic membrane.69 Using phosphorus nuclear magnetic resonance (31P NMR) spectroscopy, Jancan and Macnaughtan determined the acid dissociation constants of UDP and UDP-sugars.70 The pKa values for the diphosphate of UDP and UDP-N-acetyl glucosamine (UDP-GlcNac) were found to be approximately 6.5 for both Pα and Pβ. Nucleoside 5′-triphosphates are in the form of NTP4− at physiological pH.71 Indeed, the fully protonated nucleoside 5′triphosphates release the first two protons from their triphosphate chain at very low pH. The third deprotonation is characterized by pKa ≈ 2, whereas the pKa of the terminal Pγ phosphate group is approximately 6.5.71 2.1.3. Chemical Stability. It is fascinating how nature has created biomolecules that can be either stable or reactive depending on the prevailing chemical conditions. The behavior of phosphate mono- and diesters is a perfect illustration of this

2.2. Analysis

The study of nucleotides and their analogues using NMR techniques can determine the conformation (syn/anti, sugar puckering) and nucleobase properties (tautomerism, H-bonds, and π-stacking interactions), as well as the anomeric α/β configuration.62 1H and 13C NMR chemical shifts for natural β-Dribonucleoside 5′-triphosphates are reported in Table 3. Nucleotides exhibit relatively simple 1H NMR spectra.43,62 The aromatic protons of the purines, as well as the H6 atoms of the pyrimidines, resonate at low field (δ = 7.62−8.52 ppm) because of the proximity of nitrogen atoms, whereas H5 of the

Figure 3. Tautomeric equilibria of purines and pyrimidines. 7858


Chemical Reviews

Review

Figure 4. Some pKa values of phosphate moieties found in biological systems.58,64,67,70−74

Table 3. 1H NMR and 13C NMR Chemical Shifts in ppm (D2O) of the Main Natural NTPs purine nucleotides62 ATP H1′ H2′ H3′ H4′ H5′ H5″ H2 H8 C1′ C2′ C3′ C4′ C5′ C2 C4 C5 C6 C8

6.12 4.78 4.58 4.37 4.26 4.18 8.24 8.51 87.3 74.9 71.1 84.8 65.9 153.6 149.9 119.4 156.4 140.7

pyrimidine nucleotides62,82

GTP 5.90 4.80 4.57 4.33 4.24 4.18 − 8.10 87.4 74.2 71.1 84.7 65.9 154.7 152.6 117.0 159.8 138.6

reaction intermediates. The range of chemical shifts (δ) for most organophosphorus compounds covers 700 ppm (from 500 to −200 ppm), using 85% H3PO4 as the external reference at δ 0.0 ppm. For endogenous nucleotides and derivatives, however, the chemical shift values are limited to a narrow range, from 10 to −30 ppm, and exhibit high pH and counterion dependences.90 A set of representative nucleotide spectra are shown in Figure 5. In 1 H-decoupled 31P NMR spectroscopy, nucleoside 5′-monophosphates are characterized by a singlet at approximately 4 ppm (Figure 5A), whereas cNMPs (Figure 5B) and NMP-sugars exhibit singlets at approximately −2 and −5 ppm, respectively.90,91 Nucleoside 5′-diphosphates feature a doublet of doublets with a coupling constant of 2Jαβ ≈ 20 Hz (Figure 5C). Nucleoside 5′-triphosphates show three resonance signals at approximately −10 (Pγ, doublet, 2Jγβ ≈ 20 Hz), −11 (Pα, doublet, 2 Jαβ ≈ 20 Hz), and −22 ppm (Pβ, pseudo triplet) (Figure 5D). It is important to note that the Pγ groups of (d)NTPs can shift between −5 and −10 ppm, depending on the pH.30 Within pyrophosphate diesters, the 31P nuclei are affected by the protonation states of the phosphate groups and by the types and conformational positions of the substituents. In this regard, pyrophosphate diesters fall into two categories: those characterized by a singlet in the range from −10 to −15 ppm and those exhibiting two doublets with a 31P−31P scalar coupling value (2Jαβ) of ∼20 Hz. The first category includes dinucleoside pyrophosphates,62 as well as the reduced cofactors NADPH and NADH (Figure 5E).92−95 For unsymmetrical pyrophosphate diesters, the singlet indicates that the 31P nuclei are in similar chemical environments because of the conformational symmetry around the pyrophosphate diesters and the absence of nearby substituents that have a strong influence on the chemical shift, such as aromatic rings or alkyne groups.92 The second category encompasses compounds with nonidentical phosphorus centers. Thus, if the difference in the 31P chemical shifts in hertz (Δν) is sufficiently high compared to the 2 Jαβ coupling constant (Δν/J > 5), the spectrum will show a characteristic first-order splitting of a doublet of doublets (two spin AX systems). The oxidized cofactors NADP+ and NAD+ (Figures 1 and 5F) and NDP-sugars (UDP-Glc, UDP-Gal, ADPGlc, GDP-Man) fall into this category.92−96 The difference between the reduced and oxidized cofactors is the conjugation

H1′ H2′ H3′ H4′ H5′ H5″ H5 H6 CH3 C1′ C2′ C3′ C4′ C5′ C2 C4 C5 C6 CH3

UTP

dTTP

CTP

5.97 4.38 4.42 4.26 4.24 4.21 5.95 7.96 − 88.8 74.4 70.3 84.1 65.6 152.6 167.0 103.4 142.5 −

6.22 2.24 4.54 4.07 4.09 4.06 − 7.62 1.80 85.7 38.9 71.1 85.3 65.8 153.4 166.9 112.1 137.8 12.0

5.96 4.38 4.38 4.35 4.25 4.23 6.34 8.22 − 89.5 74.5 69.2 83.5 64.6 149.5 159.9 95.6 144.0 −

pyrimidines occurs at a higher field (δ = 5.95−6.34 ppm). The sugar moieties exhibit a multispin system that ranges from δ ∼6 ppm (H1′) to δ ∼4 ppm (H5′, H5″). In addition, the spectra of 2′-deoxynucleotides exhibit the signal of the two hydrogen atoms in the 2′-position and appear as an ABMX system close to δ 2.5 ppm. Similarly to 1H and 13C, 31P has a spin quantum number of 1/2, but in contrast, 31P is the only natural isotope of the phosphorus element. Although the nucleus has a rather low sensitivity (ca. 7% that of 1H), NMR measurements are easy to conduct.83 31P NMR spectroscopy is highly valuable for studying the binding of phosphorus biomolecules to proteins and the structure and dynamics of phosphorylated proteins,84 as well as for the characterization of phosphorus compounds in metabolomic studies85−87 and food science.88,89 This technique is also very useful for monitoring the course of reactions and characterizing 7859


Chemical Reviews

Review

Figure 5. 31P NMR (162 MHz) spectra in D2O of common nucleotides and derivatives as sodium salts.

in Table 2. Because the sugar and phosphate moieties have no significant UV absorption above 230 nm, nucleotides exhibit UV absorption profiles similar to those of their parent nucleosides with λmax values close to 260 nm and molar extinction coefficients of about 10 mM−1 cm−1. In addition to NMR and UV spectroscopies, mass spectrometry (MS) is a key tool for the analysis of nucleotides, either as part of nucleic acids or as individual compounds. Recently, exhaustive reviews were published on this subject.97,98 Initially, high-performance liquid chromatography (HPLC) coupled with UV detection and based on ion-exchange (IE) chromatography was used to quantify nucleotides.99 In the past

state of the nicotinamide ring. In the oxidized form, the aromatic conjugation is intact, and the ring current has a major impact on the chemical shifts of nearby nuclei. The orientation of the ring relative to the phosphorus nuclei also affects the direction and amplitude of the chemical shift. Within the reduced cofactor, the nicotinamide ring is not conjugated, and the 31P nuclei are, therefore, magnetically equivalent. The electronic properties of nucleosides and nucleotides have been determined for more than 30 years. However, a recent study showed that nearly all of the previously published UV extinction coefficients for nucleotides are inaccurate, with errors of up to 7%.65 The revised electronic data for natural NMPs are reported 7860


Chemical Reviews

Review

DNA or RNA polymerases. 109 For example, AZT 5′triphosphate (AZTTP) and 3TC 5′-triphosphate (3TCTP), shown in Figure 6, interact with HIV reverse transcriptase,

15 years, liquid chromatography coupled with mass spectrometry (LC-MS) or tandem mass spectrometry (LC-MS/MS) has emerged, offering improved selectivity and sensitivity.100,101 However, classical IE analytical conditions are often incompatible with mass spectrometric detection, as high concentrations of nonvolatile salts are used in mobile phases. To overcome this drawback, reverse-phase liquid chromatography (RPLC) was developed. In this case, a typical mobile phase consists of a mixture of water and methanol, or acetonitrile, combined with a volatile ion-pairing agent, such as trifluoroacetic acid or N,Ndimethylhexylamine. Alternatively, hydrophilic interaction chromatography (HILIC) has recently generated interest in the analysis of polar compounds, such as nucleotides.102−104 This variant of normal-phase chromatography uses a hydrophilic stationary phase combined with a mixture of water (as the stronger eluting solvent) and methanol or acetonitrile as the eluent. Unlike RPLC, the HILIC gradient elution begins with a low-polarity organic solvent, and analytes are eluted by increasing the water content in the eluent. 2.3. Biological Applications

Figure 6. Several representatives of biologically active synthetic nucleotide analogues.

Given the importance of nucleotides and their conjugates in biological processes, considerable research effort has been directed toward developing synthetic routes to gain access to these compounds and structural analogues. Indeed, the structural modification of nucleotides significantly alters their chemical properties and, therefore, their biological activities. The scope of these compounds ranges from mechanistic probes and versatile chemical tools for assay development to therapies and diagnostics. Nucleoside 5′-triphosphates are key compounds in genome analysis and medicinal diagnostics. Thus, the “dideoxy method” of DNA sequencing, developed by Sanger et al.,23 is based on the DNA polymerase-dependent synthesis of a nucleic acid strand that is complementary to a nucleic acid template. This occurs in the presence of natural dNTPs and 2′,3′-didoxynucleotides (ddNTPs), which act as chain terminators.23 The DNA elongation is randomly terminated whenever a ddNTP (ddATP, ddCTP, ddTTP, or ddGTP) is added to the growing oligonucleotide chain. The resulting products have varying lengths and can be separated by size using polyacrylamide gel electrophoresis. Originally, four different reactions were required per template, and each reaction involved a different ddNTP. However, advances in fluorescence detection have made it possible to combine the four terminators into a single reaction using a set of four chain-terminating dideoxynucleotides, each of which is labeled with a different fluorescent dye.105,106 Over the past 10 years, the Sanger method has been partially superseded by several “next-generation” sequencing technologies that offer major increases in cost-effective sequence throughput.21,22,24 Modified (d)NTPs can also be involved in the systemic evolution of ligands by exponential enrichment (SELEX) and other related combinatorial methods of in vitro selection to generate modified catalytic nucleic acids and aptamers for various practical applications.107,108 In addition, (d)NTPs can be applied to pharmacological studies of biologically active nucleoside analogues. Nucleoside analogues (NAs), for example, 3′-azido-2′,3′-deoxythymidine (AZT, zidovudine), β-L-2′,3′-dideoxy-3′-thiacytidine (3TC, lamivudine), and β-D-arabinofuranosylcytosine (araC, cytarabine), are a class of antiviral and anticancer drugs whose mechanism of action involves the interaction of their 5′phosphorylated derivatives with essential enzymes, such as

leading to the inhibition of viral replication.110 In contrast, araC is a cytotoxic drug that incorporates into DNA as its 5′triphosphate derivative (araCTP), with subsequent DNA strand breaks. Thus, the availability of nucleotide analogues is crucial for biochemical and pharmacological studies. Another example of the nucleotides’ biological activity is illustrated by di(uridine) tetraphosphate (Up4U, diquafosol), an agonist of the P2Y2 purinergic receptor, which is used to treat dry eye disease (Figure 6).111 Dinucleotides also appear to be a promising new class of antiplatelet agents.112 Sugar nucleotides have been synthesized and studied as potential therapeutic candidates, and they may act as inhibitors/promoters of therapeutically significant enzymes.34 Finally, there is growing interest in nucleolipids as molecular carriers for drug delivery.14−17,19,113 In this architecture, the nucleic acid component has a functional role, providing selective interaction capacity. The bulkier amphiphile acts as a scaffold moiety with the potential to create assemblies of characteristic geometries and orientations.

3. GENERAL CONSIDERATIONS 3.1. Phosphorus

Phosphorus ( 15 P), with the electronic configuration 1s22s22p63s23p3, is in the same group as nitrogen in the periodic table. The oxidation state of phosphorus can range from −3 to +5, but the latter is the only state present in cells. The nomenclature of organophosphorus compounds depends on both the oxidation state of phosphorus and the type of atoms (C, N, O, S) to which it is attached.114 The main phosphorus functional groups covered in this review are summarized in Table 4. It is important to note that, in solution, tetracoordinated Hphosphonates are in equilibrium with tricoordinated phosphites (Figure 7). These tautomeric forms have different reactivities; therefore, the corresponding P(III) entities are versatile synthetic precursors in organophosphorus chemistry.115 3.2. Purification of Nucleotides

Isolating nucleotides and their analogues still presents a major challenge, because purification by chromatography of the polar 7861


Chemical Reviews

Review

order for this elution is as follows: monophosphates, diphosphates, and triphosphates, followed by oligo- and polyphosphates. As the nucleotides often coelute with inorganic phosphates (e.g., phosphate [PO43−], pyrophosphates [P2O72−], linear triphosphate [P3O105−], and cyclic trimetaphosphate [P3O93−]), a second purification step is performed involving reverse-phase chromatography, possibly using a semipreparative HPLC system.107 In addition to inorganic phosphates, an excess of triethylammonium cations can be observed, which can be attributed to the incomplete removal of triethylamine. During the reverse-phase chromatographic step and/or after the concentration of the combined fractions, these counterions can also be lost.117 Both types of purification steps were reported by Murphy.30 The technical details for buffer preparation and a description of the ion-exchange supports are available. In a few cases, an additional step has been reported, prior to the separation of the various nucleotides by ion-exchange chromatography, to avoid the presence of multiple counterions in the crude mixture [i.e., (Bu)4N+, (Bu)3NH+, and Et3NH+ cations], which can disrupt the order of elution. These quaternary ammonium cations were replaced by NH4+ ions using simple percolation through a cationexchange resin with pure water as the eluting solvent. Recently, Korhonen and co-workers reported the use of a new phosphorylating agent, called PPN pyrophosphate {tris[bis(triphenylphosphoranylidene)ammonium]pyrophosphate} for the synthesis of NTPs and NDPs.118,119 In this case, selective precipitation made it possible to eliminate the excess of pyrophosphate and PPN cations and allowed the nucleotides to be isolated directly as sodium salts. In the particular case of the enzymatic synthesis of nucleoside 5′-triphosphates, Wu et al.120 developed a purification procedure based on boronate affinity gel. The ribonucleotides were isolated through the formation of a complex between the borate group and the cis-diol of the ribonucleotides. In contrast, for deoxyribonucleotide derivatives, the hydrolysis of excess ATP

Table 4. Nomenclature of Phosphorus Functional Groups Covered in This Review

Figure 7. Tautomeric equilibrium between the H-phosphonate and phosphite forms.

compounds contaminated with various negatively charged species remains a limiting step. The multiple purification procedures associated with the derivatives’ relatively low chemical stability are time-consuming, require extreme care, and often produce low yields. Indeed, the crude material obtained after solution synthesis is made up of a complex mixture of nucleotides with different numbers of phosphate groups, as well as byproducts (mostly inorganic phosphates) with similar characteristics.116 Generally, purification procedures require at least two types of chromatography. The first involves an ion-exchange support that is positively charged, such as diethylaminoethyl (DEAE) Sephadex, where the species are eluted [using a gradient of triethylammonium hydrogen carbonate (TEAB) at a pH of approximately 7.4−7.6] according to the number of charges they have. The

Figure 8. Main supports used for polyphosphorylated nucleoside synthesis and their loadings. 7862


Chemical Reviews

Review

Figure 9. Intermediates formed during the synthesis of NMPs from nucleosides (NuOH).

Scheme 1

Despite the advantages offered by the solid-phase approach, the heterogeneous reaction conditions can cause other problems, such as nonlinear reaction kinetics, unequal distribution and/or access to the reaction sites, solvation problems, inefficient coupling rates, and difficulties with intermediate analysis. Soluble polymer-supported synthesis, also termed liquidphase synthesis, is an alternative method that has the advantages of solid-phase synthesis while working under homogeneous reaction conditions. The crude reaction mixture is usually worked-up by dilution with a solvent that causes the precipitation of the polymer-bound products, which are then isolated by filtration. The most widely used soluble polymers in liquid-phase synthesis are the two homopolymers poly(vinyl alcohol) (PVA) and poly(ethylene glycol) (PEG).122,123,125,139 Room-temperature ionic liquids (RTILs) are salts that are liquid at room temperature and have relatively low viscosities. These compounds have generated increased interest not only as solvents for organic synthesis but also as homogeneous supports thanks to their properties, such as nonflammability, nonvolatility, and greater thermal stability.140−143 They have recently been used for nucleotide supported synthesis.

(required during the enzymatic phosphorylation) was required. Finally, a last step of purification, using anion-exchange chromatography on Q sepharose FF, was required for all nucleotides. 3.3. Solid-Phase and Polymer-Assisted Nucleotide Synthesis

The different approaches for accessing nucleotides and related compounds involve classical solution synthesis, as well as supported solution synthesis. Supported organic chemistry emerged in the 1960s with the Merrifield method for peptide solid-phase synthesis.121 Anchoring reactants to a support enables reactions to be pushed to completion using an excess of a reagent. In addition, purification of the crude reaction mixture is simplified because the products are immobilized on the support, which means that they can easily be separated from the soluble byproducts and excess reagents by filtration. Alternatively, the anchored entities can also be reagents or catalysts. Supports are characterized by their loading capacity, which refers to the number of anchoring sites per gram of support (mmol/g). To improve the accessibility of the reagents and also to facilitate cleavage for product recovery, a linker is often anchored to the support before immobilization of the reactant. Solid-phase and polymer-assisted syntheses have been the subjects of numerous reviews in the literature.122−125 In this section, we provide a brief overview of the main supports currently used in nucleotide synthesis that involve either solid or soluble supports (Figure 8). Insoluble resins (typically beads 50−200 μm in diameter) are commonly used as supports for the synthesis of oligonucleotides. Controlled pore glass (CPG) and polystyrene (PS) have proved to be the most suitable. CPG is a rigid nonswelling material that has deep pores where oligonucleotide synthesis takes place. Highly cross-linked PS beads have good moisture-exclusion properties and allow for very efficient oligonucleotide synthesis.

4. NUCLEOSIDE 5′-MONOPHOSPHATES Synthetic approaches for the synthesis of nucleoside 5′monophosphates using both P(III) and P(V) chemistries have been extensively described, and the corresponding intermediates are shown in Figure 9. 4.1. Solution-Phase Synthesis

4.1.1. Synthesis via a Phosphorodichloridate Intermediate. This is the most widely used method for the synthesis of NMPs. In 1967, Yoshikawa and co-workers reported a onestep 5′-monophosphorylation of natural ribonucleosides using phosphoryl chloride in trimethylphosphate at 0−4 °C, followed 7863


Chemical Reviews

Review

Figure 10. Acyclic and carbocyclic NMPs synthesized according to Yoshikawa’s method.

Scheme 2

by hydrolysis (Scheme 1).144 Yields ranged from 88% to 98%. As shown in Scheme 1, the reaction’s regioselectivity can be explained by the formation of a nucleoside−trialkyl phosphate complex (1).145 Hydrolysis of the phosphorodichloridate intermediate 2 was initially performed with water, leading to the hydrolysis of excess phosphoryl chloride into phosphoric acid with the concomitant release of hydrogen chloride. To prevent the acid-catalyzed cleavage of the glycosidic bond, water was replaced by a TEAB buffer at pH ∼7.5. Furthermore, the addition of molecular sieves or 1,8-bis(dimethylamino)naphthalene, alias Proton Sponge, proved to be effective for the synthesis of highly acid-sensitive nucleotides.116,134 In addition to numerous nucleoside analogues, this approach was also applied to the preparation of acyclic NMPs 3−5 and carbocyclic NMPs 6−8, as shown in Figure 10.146−149 The uracil derivatives were synthesized in 50−60% (3a,b) and 10−15% (5a−c) yields.148 Interestingly, the carbocyclic nucleosides (in which a fused cyclopropane moiety constrains the pseudo sugar ring) react differently toward POCl3 depending on the sugar ring conformation.146 Indeed, the adenosine analogue in the southern (S, 2′-endo) conformation was easily monophosphorylated to produce 6 in 60% yield, whereas, for the derivative in the northern (N, 2′-exo) conformation, the cyclic 3′,5′-nucleotide was isolated as a major product. This was attributed to the close proximity between the 3′-OH and 5′-OH groups. 4.1.2. Synthesis via a Phosphoramidate Intermediate. Vanboom et al. reported that 2,2,2-tribromoethyl phosphoromorpholinochloridate (9) was a convenient reagent for synthesizing ribonucleotides.150 The reaction of the basemodified analogues of adenosine 10a−c provided the corresponding phosphoromorpholidates 11a−c, followed by the in situ removal of the 2,2,2-tribromoethyl protecting group with the Cu−Zn couple. The subsequent acid hydrolysis gave AMP in 65−70% yields (Scheme 2). 4.1.3. Synthesis via a Phosphodiester Intermediate. Scheit described the synthesis of TMP and its N-methyl derivative 12 by coupling the 2′,3′-protected nucleosides 13 and 14 with 2-cyanoethyl phosphate in the presence of N,N′dicyclohexylcarbodiimide (DCC), followed by in situ removal of the cyanoethyl group (Scheme 3).151

Scheme 3

More recently, another phosphorylating reagent, 2-O-(4,4′dimethoxytrityl)ethylsulfonylethan-2′-yl-phosphate (15), was developed by Taktakishvili and Nair for the phosphorylation of primary and secondary alcohols of deoxyribonucleosides 16−20 in the presence of triisopropylbenzenesulfonyl tetrazolide (TPSTAZ) (Scheme 4).152 The phosphodiester intermediates 21−25 were deprotected in situ under basic conditions to afford dNMPs in 80−95% yields. These approaches, involving a phosphodiester as an intermediate, have one drawback: protection is required for the nucleobase, as well as on the 2′- and 3′-hydroxyl groups of the sugar, prior to phosphorylation. 4.1.4. Synthesis via a Phosphotriester Intermediate. This type of synthesis, developed by Kimura et al., involves a Mitsunobu-type coupling between an unprotected nucleoside (thymidine or uridine) and dibenzyl phosphate in the presence of triphenylphosphine and diethylazodicarboxylate.153 The best results were obtained using hexamethylphosphoramide (HMPA) as a solvent (Scheme 5). Subsequent debenzylation of the resulting phosphotriester intermediates 26 and 27 by catalytic hydrogenation provided the corresponding NMPs in 73−78% yields. Another approach for accessing a phosphotriester intermediate relies on P(III) chemistry and involves the coupling of a protected nucleoside with a phosphoramidite reagent, followed by the in situ oxidation of the resulting phosphite triester. As illustrated in Scheme 6, the uridine and adenosine analogues 28 and 29 reacted first with di-tert-butyloxy N,N-diethylphosphoramidite in the presence of 1H-tetrazole and were then oxidized 7864


Chemical Reviews

Review

Scheme 4

Scheme 5

Scheme 6

Figure 11. Carbocyclic NMPs synthesized via phosphotriester intermediates.

Figure 12. Formation of NMP from cycloSal pronucleotides.

with m-CPBA to produce the corresponding phosphotriesters 30 and 31.146 Finally, both tert-butyl and acetonide groups were removed simultaneously under acidic conditions (using a Dowex resin), and the desired monophosphates 32 and 33 were isolated in 68% and 54% yields, respectively. The carbocyclic NMPs 34−38 shown in Figure 11 were obtained in three steps according to this synthetic methodology. In several cases, the deprotection step was achieved by treatment with a solution of trifluoroacetic acid (TFA; 5−10%) in dichloromethane.154−156 The 3′-OH function was protected

prior to the synthesis of compounds 36 and 37 with a tetrahydropyranyl group, which was then removed together with the tert-butyl groups in the last step.155,156 The yields for this type of phosphotriester approach ranged from 45−69% for compounds 36 and 37 to 97% for compound 38.154 In the late 1990s, Chris Meier introduced a new concept for the intracellular delivery of antiviral nucleotides157−161 based on the use of salicylic alcohols to mask the phosphate group of NMPs. This led to neutral and lipophilic phosphotriesters called cycloSal pronucleotides. This type of phosphate protecting group 7865


Chemical Reviews

Review

Figure 13. Syntheses of cycloSal phosphotriesters via P(III) and P(V) chemistries.

Scheme 7

Scheme 8

is cleaved according to a pH-driven chemical hydrolysis mechanism. Thus, the nucleophilic attack of water or hydroxide anion on the phosphotriester gives rise to a benzyl phosphodiester intermediate that is spontaneously converted into the NMP (Figure 12). By varying the nature of the substituents on the aromatic ring (X, Figure 12), the phosphorus atom’s electrophilicity and the reaction’s kinetics can be finely tuned. Accordingly, acceptor substituents, such as chloro and nitro groups, increase the reactivity of the cycloSal phosphate triesters compared to donor substituents, such as methyl groups. In addition to their interest as original prodrugs, such phosphotriester derivatives have also been used for the synthesis of polyphosphorylated nucleosides and their conjugates. The coupling of the cycloSal phosphate moiety to the 5′-hydroxyl group of a nucleoside is achieved using either P(III) or P(V) chemistry, as shown in Figure 13. The first approach is based on

the coupling of a nucleoside with saligenylchlorophosphite, followed by in situ oxidation (Figure 13, path A). Oxone was found to be a better oxidizing agent than t-BuOOH or the mixture I2/pyridine/water for two reasons: (i) it allows the quantitative oxidation of the phosphite triesters into the phosphotriesters and (ii) inorganic salts of Oxone are easily washed out by liquid−liquid extraction.161 The second P(III) pathway involves the reaction of a nucleoside with a phosphoramidite and then the oxidation of the phosphite triester (Figure 13, path B). The third strategy requires the reaction of a nucleoside with a cyclosaligenylphosphorochloridate (Figure 13, path C), whereas the fourth approach involves the prior synthesis of nucleoside phosphorodichloridate, which is then treated with salicylic alcohol (Figure 13, path D). The synthetic approaches using P(III) intermediates are the most 7866


Chemical Reviews

Review

Scheme 9

Figure 14. Resin-bound phosphitylating reagents.

Scheme 10

approach provides an alternative for the monophosphorylation of acid-sensitive nucleosides, as shown by the synthesis of 3TC 5′-monophosphate (Scheme 8).164 Nucleoside 5′-H-phosphonate monoesters are easily prepared through the transesterification of diphenyl H-phosphonate with suitably protected nucleosides in pyridine and produce nucleoside phenyl Hphosphonate diesters intermediates.165 The addition of aqueous triethylamine to the reaction mixture results in the rapid hydrolysis of both the excess reagent and the nucleoside phenyl H-phosphonate diester. Accordingly, H-phosphonate monoester 46 was obtained in 95% yield (Scheme 8). Because H-phosphonate monoesters are more resistant to oxidation than the corresponding H-phosphonate diesters, they need to be converted into trivalent silyl phosphites prior to oxidation. As shown in Scheme 8, the reaction of nucleoside H-

common because P(III) species have greater reactivity than P(V) species. For the synthesis of carbocyclic NMPs,162,163 only P(III) chemistry has been used. Accordingly, carbocyclic nucleosides 39 and 40 were first reacted with saligenylchlorophosphite 41 in the presence of N,N-diisopropylethylamine (DIPEA) to produce the corresponding cycloSal phosphite triesters, which were oxidized in situ. Derivatives 42 and 43 were obtained in 26−46% yields (Scheme 7). After hydrolysis under aqueous basic conditions, compounds 44 and 45 were isolated in 39% and 84% yields, respectively.163 4.1.5. Synthesis via a 5′-H-Phosphonate Intermediate. H-phosphonate monoesters are relevant P(III) precursors that can be used as substrates for oxidative transformations to provide a variety of phosphate monoesters, such as NMPs.115 This 7867


Chemical Reviews

Review

phosphonate monoester 46 with excess N,O-bis(trimethylsilyl) acetamide (BSA) leads to the quantitative formation of the corresponding bis(trimethylsilyl) phosphite 47. The subsequent addition of (−)-(8,8-dichlorocamphorylsulfonyl)oxaziridine (DCSO) to the reaction mixture produced the bis(trimethylsilyl) phosphotriester 48, which was finally hydrolyzed to eliminate the TMS groups (overall yield of 85% from 46).

Scheme 11

4.2. Polymer-Supported Synthesis

4.2.1. Synthesis Involving a Polymer-Bound Reagent. Over the past decade, the Parang research group has developed various synthetic approaches for the regioselective phosphorylation of unprotected nucleosides and carbohydrates, involving P(III) chemistry and a polystyrene support. In their first report,129 the immobilized phosphitylating reagent 49, prepared by coupling polystyrene-bound p-hydroxybenzyl alcohol with the commercially available 2-cyanoethyl N,N-diisopropylchlorophosphoramidite, was reacted with uridine in the presence of 1H-tetrazole to produce the corresponding polymer-bound phosphite triester 50 (Scheme 9). In situ oxidation with tBuOOH gave the polymer-bound phosphotriester, which was treated with 1,8-diazabicyclo[5.4.0]undec-7-ene (DBU) to remove the 2-cyanoethyl (CNE) protecting group. Finally, basic cleavage of the p-hydroxybenzyl linker of 51 afforded UMP in 67% overall yield. Because of the cleavage mechanism, the linker was released along with the phosphorylated products, leading to contamination. Extra purification steps were required as a result. To overcome this limitation, two new linkers, involving an amide (52) or an N-Boc aminomethyl (53) bond, were proposed and coupled with 2-cyanoethyl N,N-diisopropylchlorophosphoramidite to produce the corresponding polymer-bound phosphitylating reagents 54 and 55 (Figure 14).131 This modification involves an additional step (acidic treatment leading to the cleavage of the p-acetoxybenzyl alcohol linker, Scheme 10) that was not included in the previous reaction sequence (coupling, oxidation, and removal of the CNE group, Scheme 9). It is important to note that, after the final cleavage, the solid-phase resins can be reused for generating the solidphase phosphitylating reagents. Using this methodology, UMP, dTMP, and AMP were synthesized in overall yields of 53−67%. The Parang research group also reported an alternative method using two types of polymer-bound oxathiophospholanes, 56 and 57 (Scheme 11), which were prepared from NovaSyn Tentagel bromo resin and bromoacetamidomethyl NovaGel resin.127 Coupling of A, U, and dT with 56 and 57 gave P(III) derivatives 58 and 59, which were further oxidized to produce 60 and 61, respectively. Cleavage of these cyclic P(V) intermediates with 3-hydroxypropionitrile, followed by treatment with DBU, resulted in the corresponding nucleoside 5′monophosphates through the elimination of the polymer-bound ethylene episulfide. Accordingly, UMP, dTMP, and AMP were obtained in 67−78% yields from the polymer-bound linkers. This approach was expanded to the synthesis of nucleoside 5′monophosphorothioates by using 3H-1,2-benzodithiol-3-one1,1-dioxide (Beaucage reagent) during the oxidation step. 4.2.2. Synthesis Involving Attachment of the Sugar Moiety to the Support. In 2010, Oliviero et al. developed this approach to prepare 5-amino-1-β-D-ribofuranosylimidazole-4carboxamide (AICAR) 5′-monophosphate, a biosynthetic precursor of purine nucleotides, and its 4-N-alkyl derivatives.128 The solution-phase synthesis of these compounds is difficult to achieve; therefore, the authors set up a high-yielding supported

synthesis. This involved the connection of inosine to the solid support through the formation of an acetal bond with the hydroxyl groups in the 2′,3′-positions (Scheme 12). Because of the nature of anchoring, this approach is restricted to the phosphorylation of ribonucleosides. The supported nucleoside 62 was obtained in three steps: treatment of the 5′-protected inosine 63 with 4(hydroxymethyl)benzaldehyde dimethyl acetal in the presence of catalytic amounts of p-TsOH, followed by coupling of the resulting intermediate with the polystyrene MMTrCl resin and, finally, removal of the tert-butyldiphenylsilyl (TBDPS) protecting group with ammonium fluoride. Therefore, inosine was bound to the trityl resin through a linker bearing two acid-labile groups, namely, a benzyl tritylether and a 2′,3′-acetal that could be selectively cleaved in anhydrous and aqueous acidic conditions, respectively. Synthesis of the phosphotriester precursors 64a and 64b was achieved upon treatment of 62 with bis(cyanoethyl)- or bis(trimethylsilylethoxy)-N,N′-diisopropylphosphoramidites in the presence of 1H-tetrazole, followed by an oxidation step with t-BuOOH. Finally, IMP was released from 64a using acidic treatment followed by washing with water. Recovery from 64b required an extra step to eliminate the cyanoethyl protection under basic conditions. In addition to the synthesis of IMP, triesters 64a and 64b also served as starting materials for the selective modifications of the nucleobase in order to form 4-Nalkyl derivatives of AICAR 5′-monophosphate. 4.2.3. Synthesis Involving Attachment of the Base Moiety to the Support. In 2009, our group first reported a soluble-supported synthesis of cytosine-containing nucleotides.133 This synthetic strategy was based on the use of a PEG anchored to the nucleobase moiety through a base labile linker (Scheme 13). Thus, the succinyl linker was introduced onto the soluble support by reacting commercially available PEG4000-(OH)2 with succinic anhydride in the presence of a catalytic amount of 4dimethylaminopyridine (DMAP) in pyridine (86% yield). The 7868


Chemical Reviews

Review

Scheme 12

Scheme 13

nucleoside ddC.134 The supported H-phosphonate monoester 73 was converted to 74 by silylation with BSA and final oxidation with t-BuOOH. The remaining salts and excess reagents were removed by a simple and easy liquid−liquid extraction process. Finally, NMPs were isolated in 60−92% yields after precipitation of the supported nucleotides in cold diethyl ether and then cleavage with concentrated ammonia. Compared to classical solution procedures, this PEG-supported methodology proved to be more efficient and scalable, as well as easier to handle.

resulting PEG-(O-succinate)2 65 was subsequently coupled with the exocyclic amino group of the free nucleosides C, dC, araC, and ddC in the presence of the coupling agents 1hydroxybenzotriazole (HOBt) and DCC to produce 66−69. Interestingly, the reactions were easy to monitor with 1H and 13C NMR spectroscopies. Conversions were quantitative, and yields were ∼85%. With one nucleoside at each end of the polymeric chain, the capacity of the synthesized PEG nucleoside was evaluated at 0.5 mmol·g−1. Finally, regioselective 5′-O-phosphorylation of the nucleosides was achieved using P(V) chemistry according to Yoshikawa’s method, albeit at 35−40 °C,133,135 to produce the compounds 70−72. P(III) chemistry was used for the acid-sensitive

4.3. Enzymatic Synthesis

In cells, NMPs are synthesized from their nucleoside counterparts by nucleoside kinases, which usually requires ATP as a phosphate donor.110 A few enzymatic procedures have been 7869


Chemical Reviews

Review

5.1. Solution-Phase Synthesis

reported for the preparation of natural and modified NMPs starting from the corresponding nucleoside precursors.166 Although the main advantage of using enzymes (especially kinases) is the regioselectivity of the reaction toward the 5′-OH group, they are somehow selective for their natural substrates. Consequently, this approach might not be applicable to all structural substrate analogues. Therefore, microbial and plant nucleoside phosphotransferases (EC 2.7.1.77; NPase) are preferentially used as biocatalysts for the 5′-monophosphorylation of nucleoside analogues, because of their broader specificity with respect to both the phosphate donors and acceptors. Barai et al. described the synthesis of (β-D-arabinofuranosyl) nucleoside 5′-monophosphates using whole cells of Erwinia herbicola.167 This method uses the shift in the equilibrium state of the reaction that occurs during the formation of the desired product when it is precipitated by Zn2+. Under optimal conditions, the conversion of nucleosides into NMP reached 41−91%. More recently, Cotticelli and Salvetti patented a procedure for the preparation of natural and modified NMPs using either free or immobilized purified enzymes or enzymes contained in cell pastes or cells.168

5.1.1. Synthesis via a Phosphorodichloridate Intermediate. This one-pot, three-step approach starts with the synthesis of an unprotected nucleoside phosphorodichloridate 2 according to Yoshikawa’s procedure for NMPs (Scheme 1, section 4.1.1), followed by the addition of tetra-n-butyl ammonium phosphate for a short period of time and then hydrolysis with TEAB (Scheme 14). A large panel of diphosphate derivatives of natural and nucleoside analogues have been obtained using this synthetic pathway. Whereas the formation of a small amount of nucleoside triphosphates, as byproducts, has been reported in some cases,116 Mishra and Broom were able to obtain NTPs as major products when using excess POCl3 and tri-n-butyl ammonium phosphate.169 5.1.2. Synthesis via a Phosphoramidate Intermediate. This approach is based on the nucleophilic substitution of an NMP, activated as the phosphoramidate monoester by inorganic phosphate salts. It is important to note that nucleoside phosphoroimidazolidates are more reactive than the corresponding phosphoromorpholidates and more permissive when it comes to the choice of solvent.34 Since the pioneering work of several groups more than 40 years ago,150,170,171 this approach has become the main strategy for the synthesis of NDPs from NMPs. Investigation of the first step, which involves activation of NMPs with CDI, by 31P NMR spectroscopy revealed carbonation of ribonucleotides during CDI treatment (Scheme 15).172 Removal of the 2′,3′-carbonate protecting group of 75 was easily performed under basic conditions. Finally, the last step involves the in situ treatment of phosphorimidazolate intermediates with tetra(-n-butyl)ammonium phosphate or tri(-n-butyl)ammonium phosphate in dimethylformamide (DMF) to produce the diphosphate derivatives. This method has been applied to the synthesis of a large number of NDP analogues, such as base-modified NDPs,173,174 as well as the carbocyclic 76−78 and acyclic 79a−e146,155,175 derivatives shown in Figure 16. A similar strategy was reported by Kore and Parmar, involving the coupling of the triethylammonium salts of ribonucleoside 5′monophosphates and imidazole in the presence of triphenylphosphine and 2,2′-dithiodipyridine as activating agents (Scheme 16).176 The resulting 5′-phosphorimidazolides 80−83 were isolated by precipitation with sodium perchlorate in acetone and filtration. Their treatment with tri(-n-butyl)ammonium phosphate in DMF in the presence of zinc chloride produced the diphosphates in high yields (95−98%). In 2013, Sun and co-workers described another multistep approach for the synthesis of NDPs and NTPs that involved protected nucleoside 5′-phosphoropiperidates and was promoted by 4,5-dicyanoimidazole (DCI).177 First, phosphitylation of the carboxybenzyl-protected nucleosides 84 and 85 with benzyl N,N-diisopropylchlorophosphoramidite 86 was per-

5. NUCLEOSIDE 5′-DIPHOSPHATES Synthetic approaches for the synthesis of nucleoside 5′diphosphates involve either P(III) and/or P(V) chemistry. The related intermediates are highlighted in Figure 15. The

Figure 15. Intermediates formed during the synthesis of NDPs from nucleosides or NMPs.

availability of dry and organic-solvent soluble reagents (i.e., phosphate or pyrophosphate salts) is often a critical factor for successful reactions. To increase both their nucleophilicity and solubility in organic solvents, the corresponding tri- or tetraalkylammonium salts are often preferred over the commercially available sodium salts. Scheme 14

7870


Chemical Reviews

Review

Scheme 15

hygroscopic, which is a major advantage in this water-sensitive reaction. Moreover, it can be easily prepared from commercially available PPN chloride. Interestingly, a workup procedure based on selective precipitation was proposed to eliminate the excess reagent from the crude reaction mixture. Precipitation of both pyrophosphate and PPN ions with sodium iodide in acetone at 0 °C and then centrifugation enabled the removal of both pyrophosphate and PPN ions. Subsequently, NDPs were isolated at high levels of purity and at reasonable levels of mass recovery with no chromatographic purifications through the addition of further volumes of sodium iodide in acetone at 0 °C. 5.1.4. Synthesis via a Mixed P(III)−P(V) Intermediate. Recently, the Jessen research group reported an iterative strategy to access NMPs, NDPs, and NTPs starting from the unprotected nucleosides.27,180 Its application to the synthesis of natural NDPs is presented in Scheme 19. First, NMPs in the form of their tetraN-butyl or tris-N-hexyl ammonium salts were regioselectively phosphitylated with the bulky phosphoramidite reagent (iPr)2NP(OFm)2181 (95) in the presence of various activating agents to selectively produce the mixed P(III)−P(V) anhydrides 96−100. Oxidation to 101−105 and then cleavage of the fluorenylmethyl protecting groups led to NDPs as piperidium salts in 75−93% yields starting from the NMPs. Ambient temperature and nondry conditions (reagents and solvents) are essential if coupling is to occur selectively because traces of water hydrolyze the excess phosphoramidite reagent and, therefore, prevent side phosphitylation reactions with the sugar’s free hydroxyl groups. In addition to high yields, short reaction times, and simple procedures, product purification is achieved through precipitation upon addition of Et2O. 5.1.5. Synthesis via a Phosphotriester Intermediate. As with the synthesis of NMPs, NDPs can be obtained from cycloSal phosphotriester precursors.82,161 Because of the high reactivity of P(III) reagents, such as chlorophosphites, prior protection of the functional groups of the starting nucleoside (except 5′-OH) is required to avoid side reactions. For example, the synthesis of dTDP is presented in Scheme 20. The 5-nitrosaligenyl chlorophosphite 106 was first prepared in 70−80% yields by reacting 5-nitrosalicyl alcohol with PCl3 in pyridine/Et2O at −20 °C. Coupling to 3′-O-acetyl-2′-deoxythymidine 17 was then performed, and in situ oxidation of the resulting phosphite triester 107 with Oxone produced the phosphotriester 108 in

Figure 16. Acyclic and carbocyclic NDPs.

formed in the presence of 1H-tetrazole, and then oxidative coupling with CCl4/Et3N/piperidine produced the phosphoropiperidates 87 and 88 in 75−85% yields over three steps (Scheme 17). Then, both carboxybenzyl (Cbz) and benzyl (Bn) esters of the nucleosidic and phosphoramidate moieties were simultaneously and quantitatively cleaved by mild catalytic hydrogenation. After filtration of the reaction mixture, treatment with excess DCI and bis(tetra-n-butylammonium) hydrogen phosphate made it possible to isolate the corresponding NDPs in 68−79% yields. This strategy was applied to the acyclic antiviral drug acyclovir [9-(2-hydroxyethoxymethyl)guanine, 79a in Figure 16] and enabled the formation of the corresponding diphosphate derivative in 56% overall yield.178 5.1.3. Synthesis via a Tosylate Intermediate. The Poulter research group reported a diphosphorylation procedure based on the nucleophilic substitution (SN2) of 5′-O-tosyl nucleosides 89−93 by tris(tetra-n-butylammonium) pyrophosphate in acetonitrile (Scheme 18).179 This strategy requires the prior multistep synthesis of 5′-O-tosyl nucleosides (introduction of N,O-protecting groups, tosylation, and removal of the protecting groups in 52−83% overall yields). Yields for the phosphorylation step ranged from 43% to 83%. This approach has been expanded to the synthesis of isosteric methylene-bridged diphosphonate derivatives using the suitable phosphorylating reagents. However, depending on the nature of the nucleobase, side reactions can occur (such as intramolecular cyclization of the nucleobase to the 5′-activated position). In 2015, Hodgson and co-workers described tris[bis(triphenylphosphoranylidene)ammonium] pyrophosphate (94), also called PPN pyrophosphate, as a new and effective phosphorylating reagent (Figure 17).118,119 Compared to the tris(tetra-n-butylammonium) salt, PPN pyrophosphate is less Scheme 16

7871


Chemical Reviews

Review

Scheme 17

yields and purity by using polymer-bound phosphitylating reagents.130,182 For (d)NDP synthesis (Scheme 21, n = 1), the polystyrene support 52 or 53 (Figure 14, section 4.2.1.) was treated with the diphosphitylating reagent 109a in the presence of 1H-tetrazole to give the polymer-bound diphosphorylating reagents 110a. It is important to note that 109a was obtained in four steps from phosphorus trichloride (97% overall yield) and should be stored at −20 °C (stable for at least 2 weeks under these conditions). Then, unprotected nucleosides were reacted with the polymer-bound reagent 110a in the presence of 1Htetrazole to yield 111a, 112a, and 113a. Oxidation with tBuOOH, followed by removal of the cyanoethyl group with DBU, produced the corresponding polymer-bound NDPs, which were released from the support under acidic conditions and then isolated in 64−80% overall yields.182 5.2.2. Synthesis Involving Attachment of the Sugar Moiety to the Support. In 2011, Meier adapted the cycloSal strategy to solid-support syntheses.132 The general procedure for the synthesis of natural 2′-deoxyribonucleotides consists of three steps, as shown in Scheme 22. The 5′-phosphotriester derivatives, including the succinyl linker attached to the 3′hydroxyl of the nucleosides, have to be prepared using classical solution synthesis before anchoring. Thus, synthesis of 3′-Osuccinyl-nucleotides was performed by reacting succinic

Scheme 18

Figure 17. Structure of PPN pyrophosphate (94).

91% yield over the two steps. Treatment of the latter with bis(tetra-n-butylammonium)phosphate in DMF, followed by removal of the acetyl protection, produced dTDP in 83% yield starting from the protected nucleoside 17. 5.2. Polymer-Supported Synthesis

5.2.1. Synthesis Involving a Polymer-Bound Reagent. In 2005, Ahmadibeni and Parang generated nucleotides in good Scheme 19

7872


Chemical Reviews

Review

Scheme 20

Scheme 21

This strategy was also applied to the synthesis of a single ribonucleotide, UDP, starting from 2′- or 3′-acetylated uridines. After several steps of synthesis in solution (DMTr protection, coupling of succinyl linker, deprotection of 5′-OH, and coupling with the chlorophosphanes), the 2′/3′-O-succinyl-5′-cycloSalnucleotide was grafted to the support and treated with bis(tetran-butylammonium)phosphate and then cleaved under basic conditions to produce UDP. In 2014, the Jessen research group applied the iterative strategy shown previously in Scheme 19 (section 5.1.4) to the supported synthesis of NDPs using CPG as the solid support.180 For this purpose, commercially available dG 3′-succinylanchored to CPG was first phosphitylated with bis(fluorenylmethyl)diisopropylphosphoramidite 95, and after two steps (oxidation with m-CPBA and treatment with 5% piperidine), the CPG-bound dGMP was obtained. One iteration followed by cleavage of the products from CPG under basic conditions produced reasonably pure dGDP.

anhydride with the 5′-dimethoxytrityl- (5′-O-DMTr-) protected nucleosides 114−116 and then removing the 5′-O-DMTr group with TFA. The 3′-O-succinyl-nucleosides 117−119 were then converted to cycloSal phosphotriesters 120−122 by phosphitylation with saligenylchlorophosphites 123 or 124, followed by oxidation as previously stated (Figure 13). Phosphotriester derivatives were finally anchored to the support using classical coupling conditions [with 1-hydroxybenzotriazole (HOBt) or O-(benzotriazol-1-yl)-N,N,N',N′tetramethyluronium tetrafluoroborate (TBTU) serving as the coupling agent]. Treatment of 125−127 with excess bis(tetra-nbutylammonium)phosphate followed by cleavage under basic conditions produced the desired (d)NDPs in purities ranging from 44% to 90%. The purity of dCDP was unexpectedly low compared to those of the other (d)NDP because of the formation of a dCDP conjugate. Finally, the desired compounds required further purification using reverse-phase column chromatography (with C18 silica gel). 7873


Chemical Reviews

Review

Scheme 22

Scheme 23

5.2.3. Synthesis Involving Attachment of the Base Moiety to the Support. This synthesis pathway is an extension of the soluble-supported synthesis of cytosine-NMPs as shown in Scheme 13 (section 4.2.3). Accordingly, the supported nucleoside 5′-monophosphates 71, 72, and 74 were first activated by CDI, and subsequent condensation of the 5′-phosphorimidazolate intermediates 128−130 with inorganic phosphate was carried out (Scheme 23).133−135 PEG-NDPs 131−133 were isolated after purification on reverse-phase RP-C18 column to eliminate residual phosphorus salts. Treatment of the supported diphosphates with concentrated aqueous ammonia, purification

by reverse-phase column chromatography, and dialysis yielded the desired NDPs in moderate to good yields (51−96%).

6. NUCLEOSIDE 5′-TRIPHOSPHATES Because of their crucial role in biological systems, synthetic access to nucleoside 5′-triphosphates has received considerable attention. In 2000, Burgess and Cook published a comprehensive review on (d)NTP synthesis.25 Since then, several reviews26,29 and chapters in books30,183,184 have focused on the subject. However, these reports only partially cover solid support synthesis, and in recent years, a number of relevant synthetic 7874


Chemical Reviews

Review

Figure 18. Intermediates formed during the synthesis of NTPs starting from nucleosides or NMPs.

Figure 19. Examples of acyclic and carbocyclic analogues of NTPs.

Scheme 24

approaches have also emerged.180,185,186 Similarly to NDPs, synthesis of NTPs relies on P(III) and/or P(V) intermediates (Figure 18) and involves the nucleoside or nucleoside 5′monophosphates as the starting material. In all cases, anhydrous conditions are essential to avoid the generation of byproducts formed by side reactions with water.

A substantial number of acyclic and carbocyclic nucleoside 5′triphosphates have been synthesized (134−151 in Figure 19) using either phosphorodichloridate, phosphoramidate, or mixed P(III)−P(V) intermediates. Some examples are reported in the following sections. 7875


Chemical Reviews

Review

6.1. Solution-Phase Synthesis

are shown in Figure 21. The spectra of NMP and nucleotides 154−156 show a single signal between 3 and −5 ppm, whereas the spectra of cyclic trimetaphosphate 157 feature a singlet at −20 ppm. The polyphosphorylated compound 158 shows three signals that are characteristic of the 5′-triphosphate moiety (−10 ppm for Pγ, −11 ppm for Pα, and −23 ppm for Pβ) and a fourth signal at +20 ppm corresponding to the 2′,3′-cyclic phosphate. The major byproduct (ca. 60% yield) was identified as AMP and resulted from the hydrolysis of the nucleoside 5′-phosphorodichloridate intermediate with residual water. In addition, the reaction of DMF with POCl3 is known to produce the Vilsmeier reagent [(CH3)2NCHClPO2Cl2], which can further react with pyrophosphate or with the 2′- and 3′-OH groups of 152a to produce byproducts 157 and 158, respectively. Despite its poor to moderate yields, the Ludwig procedure is one of the most widely used methods for NTP synthesis because of its simplicity (use of unprotected nucleosides, one-pot reaction, short reaction times) and its applicability to a wide range of nucleoside analogues modified either on the base moiety116,192−203 and/or on the sugar moiety.202,204 Carbocyclic 134205 and acyclic 135 and 136148 derivatives (Figure 19) have been synthesized in 25−35% yields according to this procedure. Significant improvements have been made to the Ludwig method since it was first reported in 1987. These include addition of Proton Sponge during the first step of the reaction sequence, even for non-acid-sensitive nucleosides, to increase the rate of phosphorylation,206 and working at a lower temperature while extending the reaction time.191 Accordingly, the ATP/ AMP ratio was subsequently improved when the reaction temperature was reduced from 0 to −15 °C and the reaction time was extended to 2 h for the second step. Under these last conditions, neither nucleotide 158 nor cyclic trimetaphosphate 157 were observed. Similar results were obtained for UTP and GTP syntheses, whereas CTP synthesis required prior protection of the exocyclic amine. Thus, natural NTPs were isolated in 54− 74% yields. Another improved procedure for solution-phase synthesis of (d)NTPs through a phosphodichloridate intermediate was reported by Kore et al.207,208 Initially developed for the synthesis of dNTPs,207 this protection-free and gram-scale procedure involves the use of (1) trimethylphosphate as the solvent for the phosphorodichloridate formation; (2) acetonitrile as the solvent in the second step of the reaction, instead of DMF, to prevent the formation of the Vilsmeier−Haack complex; and (3) substoichiometric amounts of bis(tri-n-butylammonium) pyrophosphate. Both steps were performed at −5 °C. Under these

6.1.1. Synthesis via a Phosphorodichloridate Intermediate. This one-pot, three-step synthesis was initially developed by Ludwig to synthesize ATP and dATP (Scheme 24).187 Unprotected nucleosides were first reacted with phosphoryl chloride in trimethylphosphate according to Yoshikawa’s procedure144 to produce phosphorodichloridate intermediates. Then, treatment with tributylamine and a 5-fold excess of bis(tri-n-butylammonium) pyrophosphate in dry DMF for 1 min led to the cyclic entity 152, which was hydrolyzed with TEAB (pH 7.5) to produce the nucleoside triphosphates in 78− 86% yields. To date, this approach has been applied to numerous protected and unprotected nucleosides and their analogues. The corresponding yields of NTPs ranged from poor to high because this reaction is highly dependent on the nature of the substrate. Interestingly, this approach can also be adapted for the synthesis of nucleotide analogues, including modifications on the phosphate moieties. For example, nucleoside 5′-O-(α-thio)triphosphate derivatives can be obtained by simply replacing POCl3 with thiophosphoryl chloride (PSCl3).188,189 Nucleoside (β,γ-imido)- or (β,γ-dichloromethylene)triphosphates were generated by using imidodiphosphate or dichloromethylenediphosphonate, respectively, instead of pyrophosphate.116,190 As previously stated in section 5.1.1, the use of a large excess of POCl3 and tri-n-butylammonium phosphate results in the formation of ATP as a major product, instead of ADP.169 In this case, the proposed mechanism involves the formation of a pseudo-ATP intermediate (153, Figure 20), which rearranges itself to form the cyclic triphosphate 152a.

Figure 20. Pseudo-ATP intermediate.169

In 2006, El-Tayeb and co-workers focused on the byproducts formed during the synthesis of base-modified UTP derivatives. They were able to isolate and identify NMP and NDP, as well as 2′,3′-cyclic phosphate and 2′-phosphate NTPs.116 More recently, a detailed analysis was performed by Gillerman and Fischer within the framework of ATP synthesis.191 The various byproducts, identified by 1H-decoupled 31P NMR spectroscopy,

Figure 21. Byproducts formed during ATP synthesis.172 7876


Chemical Reviews

Review

Scheme 25

Scheme 26

optimized conditions, the five natural dNTPs were prepared in 65−70% yields. This protocol was successfully exemplified on base-modified dNTPs.209−212 It is important to note that the monophosphorylation reaction of ribonucleosides does not require a base in the reaction medium, unlike the successful monophosphorylation reaction of a deoxyribonucleoside, which requires a carefully chosen base.213 6.1.2. Synthesis via a Phosphoramidate Intermediate. Similarly to NDPs (section 5.1.2), NTPs can be synthesized through the nucleophilic substitution of nucleoside 5′phosphoramidates using inorganic pyrophosphate. Two options should be considered for the phosphoromorpholidate approach: (1) the synthesis of a nucleoside phosphoromorpholidate intermediate by coupling NMP with morpholine in the presence of DCC, followed by nucleophilic substitution with tributylammonium pyrophosphate171,214 (for example, synthesis of the carbocyclic 143215), and (2) the use of reagent 9, mentioned previously (Scheme 2, section 4.1.2.), followed by the removal of the 2,2,2-tribromoethyl protecting group and then treatment with tributylammonium pyrophosphate in DMF (81−85% yields).150 Another method introduced by Hoard and Ott relies on a phosphorimidazolate intermediate that is formed by reacting NMP with CDI in DMF.216 Under these conditions and when using ribonucleoside analogues, the cyclic carbonate function introduced onto the 2′,3′-hydroxyl groups can be removed by a final treatment with triethylamine in aqueous methanol (Scheme 15, section 5.1.2). This approach has also been applied to the synthesis of various carbocyclic derivatives 137−141 and 144− 147.146,149,154,175 As illustrated in Scheme 25, the triphosphate 142 was isolated in 61% yield starting from 159.154 As for the protocol detailed in Scheme 16 (see section 5.1.2), nucleoside phosphoroimidazolates could be prepared by coupling NMPs with N-methylimidazole in the presence of triphenylphosphine and 2,2′-dithiodipyridine. Subsequent treat-

ment with bis(tetra-n-butylammonium) hydrogen pyrophosphate then produces the corresponding NTPs. Vasilyeva and coworkers obtained higher yields for the synthesis of base-modified pyrimidine NTPs using this type of phosphorimidazolate intermediate compared to the phosphorodichloridate approach.203 Bogachev developed a one-pot, three-step procedure using trifluoroacetic anhydride (TFAA) as the activating agent to convert dNMPs to dNTPs.217 TFAA is highly reactive toward the acylation of phosphate, hydroxyl, and amino groups but is easily eliminated from the reaction mixtures. Thus, the in situ activation and protection of dNMPs with a large excess of TFAA in the presence of a tertiary amine in acetonitrile were performed, and the remaining excess TFAA was removed in a vacuum. This step is highly sensitive to moisture. The resulting mixed anhydrides were treated using N-methylimidazole to produce the corresponding phosphoromethylimidazolide intermediates. Substitution with pyrophosphate and removal of the trifluoroacetyl protecting groups afforded dATP, dTTP, dGTP, and dCTP in 89−92% yields. It is important to note that the reaction time did not exceed 2−5 min for any given step. In 2004, the Borch research group reported an original strategy involving the in situ generation of pyrrolidinium phosphoramidate species as shown in Scheme 26.218 The starting materials phosphoramidate diesters 160−163 were obtained beforehand using a one-pot reaction. Natural and modified pyrimidinecontaining nucleotides were synthesized using this one-pot, twostep procedure. Initially, this involved the catalytic hydrogenolysis of the phosphoramidate diesters 160−163 and the spontaneous rearrangement [intramolecular cyclization of the N(3-chlorobutyl), N-methyl moiety] of the phosphoramidate monoesters 164−167, leading to the formation of the pyrrolidinium phosphoramidate intermediates 168−171. Then, treatment with tris(tetra-n-butylammonium)hydrogen pyrophosphate produced dTTP, dUTP, dCTP, and some analogues 7877


Chemical Reviews

Review

Scheme 27

Scheme 28

approach to synthesize dNDPs, based on the phosphitylation of protected nucleosides with salicylchlorophosphite.222 Anhydrous conditions are essential to prevent the formation of nucleoside H-phosphonates. A detailed description of this method, including crucial experimental details, was reported in a recent video article.107 Scheme 28 illustrates this methodology for dTTP synthesis. The reaction of 3′-O-acetylthymidine 17 with 2-chloro-1,3,2benzodioxaphosphorin-4-one 180 in pyridine/dioxane produced a first intermediate 181 as two diastereoisomers, characterized by 31 P NMR spectroscopy with two signals at 127.6 and 126.3 ppm. Treatment with bis(tri-n-butylammonium) pyrophosphate produced the corresponding cyclic intermediate 182, which shows two quartets at about −19 ppm for P(V), along with a triplet centered at 105.5 ppm for P(III). Oxidation of the trivalent phosphorus with an aqueous pyridine solution of iodine led to Pα oxidation and concomitant ring opening. Removal of the acetate protecting group using ammonia generated dTTP in 72% yield.222 This methodology can be applied to ribonucleosides, but both 2′- and 3′-hydroxyl functions require protection. In addition, for adenine, guanine, and cytosine nucleobases, the exocyclic amino groups must be protected to prevent any side reactions.222 This method has also been applied to the synthesis of base-modified NTPs108,223−225 and sugar-modified NTPs.224 In 2011−2013, the Huang research group reported a method based on the hypothesis that a bulky phosphitylation reagent would react selectively with the primary 5′-OH group versus the secondary 2′- and 3′-OH groups,185,186,226,227 thus avoiding extra

in yields ranging from 55% to 77%. The advantages of this method include short reaction times and easy purification steps. However, additional steps of synthesis were required to prepare the starting materials. In 2008, Sun and co-workers reported a one-pot procedure to prepare NTPs from nucleoside 5′-H-phosphonate monoesters through pyridinium phosphoramidate intermediates (Scheme 27).219 Nucleoside H-phosphonates 172−175 were obtained in three steps and in 71−85% yields by treating the 2′,3′isopropylidene nucleosides 176−179 with either salicylchlorophosphite 180 or phosphorus trichloride, followed by hydrolysis with aqueous triethylamine and removal of the protecting group.219,220 Silylation of the H-phosphonate monoesters with TMSCl in pyridine, followed by oxidation with iodine and substitution of the resulting pyridinium phosphoramidates with pyrophosphate, produced NTPs in 26−53% yields starting from 172−175. An alternative approach, mentioned previously, involves nucleoside 5′-phosphoropiperidate intermediates (Scheme 17, section 5.1.2). It was adapted for the synthesis of NTP by replacing bis(tetra-n-butylammonium) hydrogen phosphate with tris(tetra-n-butylammonium) hydrogen pyrophosphate in the last step of the reaction sequence.177,221 Accordingly, natural (d)NTPs and acyclovir 5′-triphosphate 148178 (Figure 19) were obtained in 70−81% yields starting from the corresponding fully protected nucleoside 5′-phosphoropiperidates. 6.1.3. Synthesis via a Mixed P(III)−P(V) Intermediate. In 1989, Ludwig and Eckstein described a one-pot synthetic 7878


Chemical Reviews

Review

Scheme 29

Scheme 30

Scheme 31

organic salts in the presence of 1H-tetrazole to form the cyclic intermediate 190. The reaction was monitored by 31P NMR spectroscopy. During the course of the reaction, the singlet at 127.72 ppm [corresponding to the phosphorobis(amidite) entity] was replaced by a triplet at 105.73 ppm for P(III), along with a doublet at −20.73 for P(V). This step was completed in 15 min after the addition of 4 equiv of the coupling agent. Then, oxidation of 190 with an aqueous solution of iodine led to the isolation of the acyclothymidine 5′-triphosphate 149 in 48% yield. Finally, using the iterative strategy (coupling, oxidation, deprotection) developed by the Jessen research group and previously discussed in section 5.1.4, it is possible to access not only (d)NDPs (Scheme 19), but also (d)NTPs, as shown in Scheme 31.27,180 Interestingly, all previously cited methods involving a mixed P(III)−P(V) intermediate for nucleoside 5′-triphosphate synthesis can also be used to access analogues containing

steps of synthesis (introduction and removal of protecting groups). New reagent 183 was generated in situ through the reaction of salicylic chlorophosphite 180 with excess tetra(tri-nbutylammonium) pyrophosphate (Scheme 29). Regioselective phosphitylation of the 5′-position of unprotected nucleosides generated the cyclic intermediates 184−187, which were oxidized by iodine in pyridine and water and subsequently hydrolyzed to give NTPs. Conversion was estimated to be about 10−50% of the crude material, and HPLC purification was subsequently carried out. This method was recently applied to the synthesis of ATP analogues.228 As an alternative phosphitylating reagent to salicylchlorophosphite, which is difficult to handle because of its high reactivity and hygroscopicity, Li and co-workers used bis(diisopropylamino)chlorophosphine to prepare the phosphorobis(amidite) derivative 188 (Scheme 30).229 Phosphitylation of 189 was carried out in the presence of DMAP and DIPEA. The corresponding phosphorobis(amidite) 188 was treated with pyrophosphate 7879


Chemical Reviews

Review

Scheme 32

Scheme 33

Scheme 34

modifications at the α-phosphate, such as 5′-(α-P-thiotriphosphates), 5′-(α-P-boranotriphosphates), and 5′-(α-P-selenotriphosphates).185,186,222,229 6.1.4. Synthesis via a Phosphotriester Intermediate. In 2009, Meier and co-workers expanded the use of the cycloSal phosphate triester 108 as an intermediate for the synthesis of (d)NTPs.82,161 Scheme 32 illustrates the synthetic pathway for dTTP. Details of the preparation of the starting material 108 were previously described in section 5.1.5 (Scheme 20). The reaction of 108 with pyrophosphate in DMF, followed by the removal of the acetyl group, generated dTTP in 80% yield. As stated before for the synthesis of (d)NDPs, this approach requires the introduction of N,O-protecting groups on the nucleoside moiety because of the high reactivity of the reagents involved in the phosphitylation reaction. Under these restrictions, ATP, GTP, CTP, and UTP were obtained in 40−

65% yields, and carbocyclic nucleotides 150 and 151 (Figure 19) were synthesized in 18−19% yields.163 6.1.5. Synthesis via a Phosphosulfonyl Intermediate. In 2012, the Taylor research group described a procedure for the synthesis of nucleoside polyphosphates and their conjugates using sulfonylimidazolium salts as key reagents.230 Interestingly, this procedure appears to be useful for activating nucleoside mono-, di-, and triphosphates, and the nucleoside functionalities do not require prior protection. Sulfonylimidazolium salt 191 was prepared in high yield by reacting phenylsulfonylimidazolide with methyl triflate in ether (Scheme 33). Treatment of the tetran-butylammonium salts of NMPs with 191 in the presence of Nmethylimidazole (NMI) or N,N′-diisopropylethylamine (DIPEA) as a base, followed by displacement with bis(tetra-nbutylammonium) pyrophosphate, produced high yields (84− 90%) of NTPs. 7880


Chemical Reviews

Review

Scheme 35

Scheme 36

Scheme 37

6.2. Solid-Supported Synthesis

butylammonium) pyrophosphate led to the concomitant formation of the P(III)−P(V) cyclic intermediate and release from the support. Thus, dTTP was obtained after oxidation, hydrolysis, and deprotection steps carried out in solution. Yields ranged from 4% to 50% depending on the solid support. The best yield corresponded to the use of microporous polystyrene resin. However, it was lower than that reported for solution-phase synthesis (Scheme 28, section 6.1.3). 6.2.2. Synthesis Involving Attachment of the Sugar Moiety to the Support. In the 1990s, two groups adapted the Ludwig−Eckstein triphosphorylation procedure using a solid support. The Gaur group performed the synthesis of 2′-O-methyl ribonucleoside 5′-triphosphates using a succinimide linker, which was attached to an aminopropyl-functionalized CPG.126 Commercially available 5′-O-dimethoxytrityl-N-acyl-2′-O-methyl ribonucleoside derivatized supports were first treated with 3% trichloroacetic acid in dichloromethane to remove the dimethoxytrityl protecting group, followed by phosphitylation with salicylchlorophosphite 180 and the addition of pyrophosphate salts to generate compounds 194−197 (Scheme 35). The

6.2.1. Synthesis Involving a Polymer-Bound Reagent. By analogy with the synthesis of (d)NDPs (see section 5.2.1), nucleoside 5′-triphosphates can be obtained using the polystyrene-bound phosphitylating reagent 110b (Scheme 21, n = 2).130,182 Coupling of the unprotected nucleosides (A, T, U, AZT) with the supported reagent, oxidation with t-BuOOH, then subsequent removal of the cyanoethyl groups with DBU, and final cleavage of the polymer-bound compounds under acidic conditions generated the corresponding (d)NTPs in 60−79% yields.130 In 2007, in a patent, Bradley and Bruckler reported the preparation of an immobilized phosphitylating reagent and its application to the synthesis of (d)NTPs.137 Based on the Ludwig−Eckstein procedure, the patented approach involved the use of the supported chlorophosphite 192, prepared beforehand in four steps from the polystyrene chloromethyl resin 193 (Scheme 34). Proof of concept was given with the synthesis of dTTP. First, 3′-O-acetyl-thymidine was reacted with the supported chlorophosphite. Then, the addition of bis(tri-n7881


Chemical Reviews

Review

Scheme 38

Scheme 39

first coupled to the commercially available polystyrene−TPP resin 207 to form supported iminophosphoranes 208 and 209, which were treated following the Ludwig−Eckstein procedure to produce 210 and 211 and then cleaved under basic conditions to yield the 3′-amino dNTPs 203 and 204. Yields, determined by HPLC, ranged from 70% to 75%. In contrast to the situation for the solution-phase synthesis, the 31P NMR spectra of the final products did not show the presence of side products, such as pyrophosphate or inorganic cyclic triphosphate, which were eliminated during the washing step before the oxidation step. However, the main drawback of this approach is that it is limited to the use of azidonucleosides as substrates and to the preparation of 2′- or 3′-amino NTPs. As previously detailed for (d)NDP synthesis (see section 5.2.2), supported cycloSal phosphotriester intermediates can also be used to prepare (d)NTPs. This involves replacing phosphate salts with pyrophosphate salts as the nucleophile in the last

2′-O-methyl ribonucleoside triphosphates 198−201 were obtained in yields of 60−65% after phosphitylation, oxidation, and removal of the base protecting group, along with cleavage of the products from the support by heating with aqueous ammonia. The Schoetzau research group described the synthesis of 2′and 3′-amino nucleoside-5′-triphosphates using a polymerbound triphenylphosphine resin as the support.138 No linker was required because immobilization of the azidonucleosides to the support was performed according to the Staudinger reaction. This reaction occurs between an azide and triphenylphosphine (TPP), which, under the loss of nitrogen, results in the formation of an iminophosphorane intermediate 202 (Scheme 36). In the presence of water, this intermediate is hydrolyzed to produce a primary amine and triphenylphosphine oxide. The synthesis of 3′-amino dNTPs 203 and 204 is shown in Scheme 37. The 3′-azido-2′-deoxynucleosides 205 and 206 were 7882


Chemical Reviews

Review

Scheme 40

step.132 In dTTP synthesis, the replacement of tetra-nbutylammonium phosphate with tetra-n-butylammonium pyrophosphate during the last step of the synthetic pathway, shown in Scheme 22, led to the formation of dTTP of 90% purity. 6.2.3. Synthesis Involving Attachment of the Base Moiety to the Support. Both strategies reported in this section were conducted in a homogeneous solution. The PEGsupported synthesis of cytosine-(d)NDPs was adapted to the synthesis of the corresponding cytosine-(d)NTPs by using tri-nbutylammonium pyrophosphate instead of the phosphate salt (Scheme 23, section 5.2.3).133−135 After cleavage of the products from the support, purification on a reverse-phase column, and then dialysis, CTP, dCTP, ddCTP, araCTP, and 3TCTP were obtained in 35−92% yields and 76−87% purities. Remarkably, the use of this supported methodology led to a 5-fold increase in yield for araCTP compared to the Hoard−Ott solution-phase synthesis.133 In 2014, Kore and Parang reported an ionic-tag-assisted synthesis of dNTPs (Scheme 38).136 The ionic liquid 1carboxylmethyl-3-methylimidazolium tetrafluoroborate (CMMIMBF4), shown in Figure 8, was synthesized in a onepot, two-step procedure starting from bromoacetic acid and methylimidazole.231,232 Coupling conditions of cytosine with PEG-(O-succinate)2, as reported by Crauste et al.,133 were applied to selectively anchor the exocyclic amino groups of dC and dA with the ionic liquids (Scheme 38). Upon reaction completion, ionic-liquid-tagged 2′-deoxynucleosides 212 and 213 were oiled out by the addition of ethyl acetate, leaving excess organics and unreacted materials in the top organic layer. Triphosphorylation was performed according to the Ludwig method. Finally, removal of the ionic tag with aqueous ammonium hydroxide produced dCTP and dATP in 72% and 69% yields, respectively.

selectivity of enzymes toward their natural substrates. Whole cell systems, crude enzyme preparations, and purified enzymes have been used to synthesize natural (d)NTPs and some of their labeled analogues, such as 32P-labeled compounds.25,29,233 The following examples focus specifically on the recent literature. In 2003, the Davisson research group combined chemical and enzymatic methods to synthesize azole carboxamide (d)NTPs, by taking advantage of the poor selectivity of nucleoside diphosphate kinase toward these substrates.120,234 Indeed, P(III) or P(V) chemical strategies proved to be inefficient in accessing these types of NTP analogues.120 The chemical synthesis of the diphosphate derivatives 214−216 was first carried out in solution in 70−91% yields. It involved selective 5′-tosylation of the nucleoside analogues 217−219, followed by the displacement of the 5′-tosylate group with tris(tetra-n-butylammonium) pyrophosphate (Scheme 39A). Regarding the ribo derivatives, 2′,3′methoxymethylidene group was introduced before the tosylation step and was removed before the enzymatic reaction (Scheme 39B). Two enzymatic conditions were developed: (i) For dNTP analogues 220−222, ATP served as the phosphate donor and nucleoside diphosphate kinase as the catalyst; this system was coupled with the use of pyruvate kinase and phosphoenolpyruvate (PEP) as an ATP regeneration system (Scheme 39A). (ii) In contrast, for NTP analogues 223 and 224, phosphorylation was performed by pyruvate kinase, with PEP as the phosphate donor (Scheme 39B). In 2007, Hennig et al. described the enzymatic synthesis of 5fluorouridine and 5-fluorocytidine 5′-triphosphates 5F-UTP (225) and 5F-CTP (226), respectively, using either the corresponding heterocycle and ribose or the nucleoside analogue as starting materials.235 As shown in Scheme 40, the enzymatic process involved a cascade of reactions, such as the formation of monophosphates 227 and 228 from 5-fluorouracil by uracil phosphoribosyl transferase (uraP) or from 5-fluorocytidine phosphorylation by uridine kinase (udk), respectively. Two subsequent phosphorylation steps under the control of pyrimidine-specific monophosphate kinase (pyrH) and pyruvate kinase (pyrK) produced the triphosphates 225 and 226. This

6.3. Enzymatic Synthesis

As previously mentioned, biocatalytic approaches are useful for the synthesis of natural nucleotides. However, they are less efficient when applied to the synthesis of their analogues, which contain unnatural base and/or sugar residues, because of the 7883


Chemical Reviews

Review

process provided access to all nucleotidic entities, namely, mono-, di-, and triphosphorylated derivatives of 5-fluorouridine and 5-fluorocytidine.

It is important to note that solid-phase synthesis of cyclic nucleotides has not been described so far.

7. MISCELLANEOUS The following sections cover the synthesis of cyclic nucleotides, dinucleoside 5′,5′-polyphosphates, and nucleotide conjugates. We highlight the emerging strategies that have been reviewed in recent years (e.g., cyclic dinucleotides).5,32,34,236 We do not include the synthesis of nucleoside 5′-tetra- and 5′-pentaphosphates31 or nucleoside cyclopyrophosphates34 because readers can refer to summary reviews published in 2015.

In cyclic dinucleotides (cDNs), two nucleosides are interconnected through two 3′−5′ phosphodiester bounds. Naturally occurring cyclic dinucleotides are symmetrical, as shown by cyclic diguanosine monophosphate (c-di-GMP) and its adenosine counterpart c-di-AMP (Figure 1). Enzymatic synthesis is restricted to endogenous compounds (such as c-di-GMP and c-di-AMP), whereas chemical synthesis generates structural diversity. The synthetic strategies for accessing cyclic dinucleotides and their analogues, as well as their biological properties, have been reviewed in recent years.5,236 Briefly, synthetic cDNs are prepared either by nucleotide cyclization or by stereospecific base insertion on a cyclic bis(3′−5′)-sugar phosphate. The first and most widespread approach comprises several strategies shown in Figure 22: (A) intramolecular cyclization of a 5′monophosphate-3′,5′-dinucleotide; (B) dimerization of a nucleoside 3′- or 5′-monophosphate to produce symmetric derivatives only; (C) intramolecular cyclization of a 3′,5′dinucleotide bearing a phosphate, phosphodiester, or Hphosphonate group at the 3′-end; and (D) intramolecular cyclization of a 3′,5′-phosphotriester dinucleoside. Solid-phase synthesis has only been reported within the framework of strategy C, using Tentagel or CPG polymers as solid supports.5 Briefly, the required cyclic dinucleotide was obtained either from a nucleoside 3′-phosphate, whose nucleobase is anchored through its exocyclic amino group to the support, or from a nucleotide whose 3′-phosphate group is linked to the support. This last approach is more common, as it is independent of the nature of the nucleobase moiety.

7.2. Cyclic Dinucleotides

7.1. Cyclic Nucleotides

Cyclic nucleotides differ from regular nucleoside 5′-monophosphates in that they have an intramolecular phosphodiester bridge connecting two hydroxyl groups of the same sugar moiety (Figure 1).2 The Khorana research group reported the first synthesis of nucleoside 3′,5′-cyclic phosphates, based on the reaction of NMPs with DCC.237 Later, such compounds were obtained by the phosphorylation of unprotected nucleosides with phosphorus oxychloride in trialkyl phosphate, followed by the dilution of the reaction mixture in a large volume of a potassium hydroxide solution (Scheme 41),238 leading to Scheme 41

7.3. Dinucleoside 5′,5′-Polyphosphates

Physiological dinucleoside 5′,5′-polyphosphates (DNPs), commonly abbreviated as NpnN, contain two ribonucleosides that are linked at the 5′-position of their sugar moiety through n phosphate groups (Figure 1). The first compound belonging to this family to be identified in mammals was the P1-5′-Oadenosine-P4-5′-O-adenosine tetraphosphate (Ap4A).240 Since then, 16 additional DNPs have been isolated from human tissues and characterized.4 Both enzymatic and chemical approaches can be used for preparing DNPs. The former are restricted to naturally occurring compounds and small-scale syntheses.80 For example, synthesis of dinucleoside tri- and tetraphosphates has been described using an engineered diadenosine triphosphate hydrolase as a catalyst.241 Because of the limitations inherent to enzymatic catalysis, DNPs are most often obtained chemically by extending the methods for the synthesis of nucleotides described previously.31,34 It is important to note that yields drop

concomitant cyclization and hydrolysis of the chlorophosphodiester intermediate. This one-pot procedure led to the formation of the title compounds 229 and 230 in 35−49% yields. In 2013, Rozniewska et al. reported an alternative pathway involving nucleoside 3′,5′-cyclic H-phosphonates as key intermediates (Scheme 42).239 This approach requires prior protection of the exocyclic amines of Ade, Gua, and Cyt and then synthesis of the corresponding nucleoside 3′-H-phosphonate monoesters 231−234. Thus, treatment of the starting materials in the presence of pivaloyl chloride resulted in the rapid and quantitative formation of a diasteromeric mixture of cyclic Hphosphonate diesters 235−238. In situ oxidation with iodine in pyridine, followed by hydrolysis and removal of the protecting group (except for Thy) under basic conditions, produced the desired 3′,5′-cyclic NMPs 239−242 in 65−82% yields (calculated on the basis of the nucleoside 3′-H-phosphonate as the starting material). Scheme 42

7884


Chemical Reviews

Review

Figure 22. Retrosynthetic pathways for the synthesis of cyclic nucleotides via nucleotide cyclization.

Scheme 43

(Figure 23, path A) is based on Ludwig and Eckstein’s procedure for NTPs (Scheme 28, section 6.1.3), involving a salicylphosphite intermediate. Oxidation of the cyclic P(III)−P(V) intermediate under anhydrous conditions, followed by reaction with an NMP or NDP in dry DMF catalyzed by ZnCl2 and then removal of the acetyl groups under basic conditions, generated the corresponding DNPs derivatives. Accordingly, Np4N and Np5N were synthesized in 47−85% yields.248 The second pathway (Figure 23, path B), performed either in solution82 or on a support,132 relies on a cycloSal phosphotriester intermediate, as reported previously for NDPs (Scheme 20, section 5.1.5; Scheme 22, section 5.2.2) and NTPs (Scheme 32, section 6.1.4). Phosphate or pyrophosphate salts were replaced by nucleotides to form the corresponding DNPs, after deprotection of the 3′hydroxyl group. Yields for Up2T and Ap4T were 60% and 52%, respectively.82 The third approach (Figure 23, path C) is derived from the approach developed for NTPs (Scheme 27, section 6.1.2) and makes it possible to access symmetrical dinucleoside diphosphates in 68−91% yields starting from the nucleoside 5′H-phosphonates.177 The fourth pathway (Figure 23, path D) is based on the reaction of unprotected nucleosides with polymerbound phosphitylating reagents, which are structurally similar to those developed for the synthesis of NDPs and NTPs (Scheme 21, section 5.2.1). Symmetrical DNPs were obtained in 59−68% yields, starting from the supported reagent.249 The last pathway (Figure 23, path E) is based on the iterative phosphoramidite approach described by the Jessen research group (Scheme 31, section 6.1.3) and generated Ap4U and Up2U in 36% and 83% yields, respectively.

significantly as the length of the polyphosphate chain increases.242 One widely used method involves the activation of a 5′nucleotide (NMP, NDP, or NTP) as its trialkylammonium salt with CDI in DMF, followed by in situ condensation with the other 5′-nucleotide (tributylammonium salt of NMP, NDP, or NTP) or pyrophosphate to form the required DNPs containing two to five bridging phosphate groups in 10−60% yields.62,80,243−245 Alternatively, the activation of an NTP with DCC produces a cyclic nucleoside 5′-trimetaphosphate, which can react with an NMP or an NDP to produce the corresponding DNP.62,80,243,245 Whereas CDI is preferentially used for the synthesis of dinucleoside diphosphates (50−60% yields) and dinucleoside triphosphates (20−30% yields), DCC has the greatest conversion rates and highest isolated yields for dinucleoside tetraphosphates.80,245 A recent variant of the CDI method consists of preparing P 1 ,P 2 -di(1-imidazolyl)pyrophosphate 243 (Scheme 43), which then reacts with AMP or UMP to generate the symmetrical 5′,5′-dinucleoside tetraphosphates 244 and 245 in 74% and 61% yields, respectively.246 Alternatively, DNPs can be obtained in 50−70% yields through a phosphoromethyl imidazolium intermediate, following the modification of the Bogachev procedure for the synthesis of dNTPs.217,247 A few methods based on P(III) chemistry and initially developed for the synthesis of nucleotides were adapted to the synthesis of DNPs by introducing minor modifications in the last steps of the reaction sequence (Figure 23). The first pathway 7885


Chemical Reviews

Review

Figure 23. Syntheses of DNPs involving P(III) intermediates.

DNPs.242,252,253 As shown in Scheme 46, the reaction of nucleoside 5′-phosphoropiperidates with nucleotides in the presence of excess DCI led to the formation of more than 20 symmetrical and mixed DNPs with moderate to high yields.242,253 Symmetrical DNPs could also be obtained by reacting nucleoside 5′-phosphoropiperidates with substoichiometric amounts of inorganic phosphate, pyrophosphate, or triphosphate in the presence of excess DCI.252 Compared to other methods, this approach has a shorter reaction time and higher isolated yields.

Recently, the Taylor research group reported the synthesis of symmetrical dinucleoside di- and tetraphosphates using sulfonyl imidazolium salt 191 as a reagent (Scheme 44).230 Compared to the synthesis of NTPs illustrated in Scheme 33 (section 6.1.5) and using either NMP or NDP as the starting material, the reactions were performed in the presence of 191, NMI, and MgCl2 in DMF and generated the corresponding dimers 246− 248. The mixed DNPs 249−253 could also be obtained in high yields, starting from NMPs or NTPs and using various NMPs, NDPs, and NTPs as acceptors (Scheme 44). The Taylor research group also reported an original method for preparing dinucleoside pentaphosphates (Np5N) using cyclic trimetaphosphate 157 (Scheme 45) as the phosphorylating agent.250 The reaction of the tri(tetra-n-butylammonium) salt of 157 with 191 or mesitylenesulfonyl chloride (MstCl, 254) in the presence of NMI in DMF, followed by the addition of an NMP, produced Np5N in 77−85% yields. In 2016, this strategy was adapted for the synthesis of NTPs by reacting 157 with MstCl in the presence of DABCO for 1 min at room temperature and then adding 2′,3′-acetylated nucleosides followed by phtalimide.251 After removal of the protecting groups under basic conditions, satisfactory yields of NTPs were obtained. The precise mechanism involved in the triphosphorylation step has not yet been elucidated. Finally, the approach developed by the Sun research group for the solution-phase synthesis of NDPs, which involves the activation of a nucleoside 5′-phosphoropiperidate with DCI (Scheme 17, section 5.1.2), was adapted for the synthesis of

7.4. Sugar Nucleotides

Sugar nucleotides are important intermediates in carbohydrate metabolism and function, given that they act as activated glycosyl donors in most glycosyl transferase-catalyzed glycosylations.10 Nucleoside diphosphate sugars (NDP-sugars), such as UDP-αD-galactose, and nucleoside monophosphate sugars (NMPsugars), such as CMP-sialic acid, form two subgroups of natural conjugates.9,10 To provide an overview, eukaryotic glycoproteins and glycolipids are synthesized from nine sugar-nucleotide donors, most of which are NDP-sugars. The chemical and enzymatic syntheses of these compounds have been described comprehensively in recent reviews and articles.32,34,254−259 In this section, we focus specifically on the more relevant or recent progress achieved in the chemical synthesis of NDP-sugars. NDP-sugars are mainly synthesized through the glycosylation of an NDP with a sugar activated entity (Figure 24, path A) or by coupling a sugar-1-phosphate with an activated NMP (Figure 24, 7886


Chemical Reviews

Review

Scheme 44

Scheme 45

methylimidazolides,262−264 zwitterionic pyrrolidinium ions,265 5′-phosphoropiperidates,242 phosphosulfonyl derivatives,230 mixed P(III)−P(V) anhydrides,266 and cycloSal phosphotriesters.132,161,267,268 In 2012, Tanaka et al.96,269 made a breakthrough in the chemical synthesis of NDP-sugars, by performing the coupling of a sugar-1-phosphate with a nucleotide in water (Scheme 47). Interestingly, phosphorylated reagents do not need to be converted into their trialkyl- or tetraalkylammonium cations because their commercially available sodium (NMP) and potassium salts (sugar-1-phosphate) are water-soluble. The key

path B). In most cases, the reaction sequence does not require the presence of a protecting group on the nucleobase.34 When the NDP glycosylation approach is used, the yields are usually low, and in many cases, the stereochemistry at the anomeric center of the sugar in the final products cannot be controlled.32,34 Regarding path B, a number of methods described for NDP or NTP synthesis have been adapted for the preparation of a variety of NDP-sugars, by substituting the phosphate or the pyrophosphate reagent with a sugar phosphate. These methods rely on intermediates, as already mentioned, such as phosphoromorpholidates,260 phosphorimidazolates,261 phosphoro-N7887


Chemical Reviews

Review

Scheme 46

Figure 24. Retrosynthetic approaches for the chemical synthesis of NDP sugars.

Scheme 47

intermediate is 2-imidazolyl-1,3-dimethylimidazolinium chloride (ImIm), formed in situ by mixing 2-chloro-1,3-dimethylimidazolinium chloride (DMC) and imidazole. It can activate an NMP into its corresponding phosphoroimidazolidate (Scheme 47). Optimization procedures showed that the sugar-1-phosphate salt must be added to the reaction mixture 1 h after activation of the NMP (Scheme 48) to minimize both the activation of sugar-1phosphate by ImIm and the formation of symmetrical dinucleoside diphosphate as a byproduct. This strategy made it possible to synthesize NDP-sugars 255− 257 in 23−35% isolated yields (determined by UV and based on the sugar-1-phosphates). Interestingly, the compounds require no further purification for use as a source of glycosyl donors for preparative oligosaccharide synthesis via glycosyltransferase.32,96

Scheme 48

Compared to the nucleotide analogues described so far, only a few methods have been reported to access nucleotide−lipid conjugates. These methods have been covered in several reviews over the past decade.12,15,16,34,114 The phosphoramidite and phosphoramidate strategies have been predominantly used for their chemical synthesis. For example, nucleoside diacylglycerol monophosphates were synthesized through the condensation of 3′-O-protected nucleosides with diacylglyceryl phosphorami-

7.5. Nucleolipids

Nucleolipids (Figure 1) combine a nucleobase, nucleoside, nucleotide, or oligonucleotide with a lipophilic moiety.12,16 7888


Chemical Reviews

Review

dites, followed by oxidation with iodine and then deprotection.270 In the case of phosphoramidates (usually phosphormorpholidates), two options can be considered: the reaction of a lipid monophosphate with a nucleoside 5′-phosphoramidate or the reaction of an NMP with a lipid phosphoramidate.12,34 Alternatively, nucleolipids can be obtained by condensing an acyl phosphate/pyrophosphate with a free nucleoside/nucleotide in the presence of DCC114 or by coupling an activated carboxylic acid with a nucleotide.34

exists for the anchoring and phosphorylation of unprotected nucleosides. Finding a general method that is compatible with a huge range of nucleoside analogues remains a challenge. Indeed, some methods are well suited for certain nucleosides and produce high yields, but when applied to other nucleosides, yields decrease significantly. Until recently, the preparation of unsymmetrical disubstituted pyro- and polyphosphate derivatives in satisfactory yields presented significant difficulties. Nevertheless, the increasing interest in such compounds as substrates, cofactors, and regulators for a wide range of important biochemical processes calls for research on new synthetic strategies and activating reagents. One approach sets out to obtain nucleoside 5′,5′polyphosphate derivatives and terminal-phosphate-labeled nucleoside 5′-polyphosphates. The protocols, which are based on unprotected nucleotides as parent compounds, look promising, despite moderate yields in some cases. It is because of the absence of nucleotide protection that laborious and timeconsuming process are often required. The thorough selection of activating reagents, solvents, and conjugation strategies might help increase yields and shorten reaction times in approaches based on the activation of phosphate-containing derivatives. In addition, these approaches often have poor reproducibility because of the difficulty in maintaining anhydrous reaction conditions when using hygroscopic substrates and reagents. Research in the field of nucleic acids has been and will continue to be a major driving force in the development of phosphorylation chemistry. Although it could be argued that many of the problems associated with P-anhydride synthesis have been solved, some issues have yet to be addressed, and new challenges are emerging.

8. CONCLUSIONS After decades of research to develop efficient, easy, and universal synthetic protocols to obtain mononucleoside polyphosphates and their analogues, several reasonably effective strategies and methods have emerged for the preparation of target compounds from both nucleosides and nucleotides. Researchers continue their investigations in this field because of the considerable therapeutic potential of nucleoside analogues and their active forms, nucleoside 5′-triphosphates. Synthetic approaches can rely on P(V) and/or P(III) chemistry. The use of protected, partially protected, and even unprotected starting materials can provide the expected nucleotide derivatives in satisfactory to high yields. Whereas the condensation of activated P(V) species (such as Pmorpholidates, P-imidazolides, P-imidazolium ions, and others) with phosphates has been successfully developed and can be performed without the use of protecting groups, only a few examples exist for P(III)-based couplings. These phosphorylation reactions often require long reaction times and high amounts of excess reagents and provide low to moderate yields. It is important to point out that the available methods work well with many but not all substrates. Consequently, the search for an ideal synthesis goes on. In comparison, P(III) chemistry can usually be conducted using almost equimolar amounts of the reactants. The high speed and efficiency of coupling have been well established in the context of oligonucleotide chemistry. Thus, couplings based on P(III) chemistry could, theoretically, deliver the desired compounds with satisfactory yields, easy purifications, and efficient coupling rates. However, competitive yields are only obtained when working under strictly dry conditions. Indeed, for many synthetic approaches, involving either P(V) or P(III) intermediates, it is crucial that the reactions be carried out under rigorously dry conditions. Otherwise, huge amounts of nucleotide side products are generated, together with several byproducts, such as organic polyphosphorylated salts. An ideal synthesis would involve little or no excess reagents and activators, short reaction times, the absence of protecting groups on the starting material, simple conditions (i.e., nondry solvents and reagents, open flasks, room temperature, etc.), high yields, and simple purification procedures. This last point is especially important because the separation of polar nucleotide derivatives from polar contaminants is far more difficult and sluggish than the purification of nonpolar compounds using normal-phase column chromatography. Moreover, as water and buffers are used in the elution during reverse-phase or ionexchange chromatography, repeated freeze-drying is required. This prolongs the overall process and is problematic in the case of labile P-anhydrides. In the course of work on this problem, some prospective approaches have recently been proposed, most of which are based on the supported synthesis of oligonucleotides. Unfortunately, no universally applicable and high-yielding procedure

AUTHOR INFORMATION Corresponding Author

*E-mail: [email protected]. Notes

The authors declare no competing financial interest. Biographies Béatrice Roy graduated in 1989 from Ecole Européenne des Hautes Industries Chimiques de Strasbourg. In 1993, she was awarded a Ph.D. in Organic Chemistry from the University Joseph Fourier (UJF, Grenoble, France), where she worked under the supervision of Professor Marc Fontecave on the design of new inhibitors of ribonucleotide reductase. She pursued postdoctoral studies first at the UJF and then at the University Paris Sud (Orsay, France). In 1997, she held a position of Assistant Professor in Professor G. Lemaire’s group at the University Paris Sud. In 2002, she joined Professor C. Périgaud’s research group (Montpellier, France) and was appointed by the University of Montpellier in 2007. She was a visiting faculty member in 2011 and 2012 at the University of Canterbury in Christchurch, New Zealand. Her research interests focus on the synthesis and analysis of nucleoside analogues and their polyphosphorylated entities. Anais̈ Depaix was awarded her Master’s degree in 2014 in Organic Chemistry by the University Joseph Fourier (UJF, Grenoble, France). In October 2014, she began her Ph.D. studies at the University of Montpellier (France) as part of the Nucleosides & Phosphorylated Effectors group. She is working on the development of a new synthetic methodology for polyphosphorylated nucleosides. 7889


Chemical Reviews

Review

N,N′-diisopropylethylamine 4-(dimethylamino)pyridine dinucleoside polyphosphates ion exchange flavin adenine dinucleotide G-protein-coupled receptors heteronuclear multiple-bond correlation heteronuclear multiple-quantum coherence hexamethylphosphoramide 1-hydroxybenzotriazole 2-imidazolyl-1,3-dimethylimidazolinium chloride HPLC high-performance liquid chromatography LC-MS liquid chromatography coupled with mass spectrometry LC-MS/MS liquid chromatography tandem mass spectrometry LC-UV liquid chromatography with UV detection m-CPBA meta-chloroperoxybenzoic acid MMTCl resin polystyrene monomethoxytrityl chloride resin MstCl mesitylenesulfonyl chloride NA nucleoside analogue NADH/NAD+ nicotinamide adenine dinucleotide NADPH, NADP+ nicotinamide adenine dinucleotide phosphate NDP nucleoside diphosphate NMP nucleoside 5′-monophosphate NOESY nuclear Overhauser effect spectroscopy PEG polyethylene glycol PS polystyrene PS-AM polystyrene aminomethyl PVA poly(vinyl alcohol) PvCl pivaloyl chloride RTILs room-temperature ionic liquids SELEX systemic evolution of ligands by exponential enrichment TBDPS tert-butyldiphenylsilyl TEAB triethylammonium hydrogen carbonate TFA trifluoroacetic acid TFAA trifluoroacetic anhydride dTMP thymidine 5′-monophosphate TMS trimethylsilyl TPP triphenylphosphine TPPO triphenylphosphine oxide TPS-TAZ triisopropylbenzenesulfonyl tetrazolide TriMP cyclic trimetaphosphate UMP uridine 5′-monophosphate DIPEA DMAP DNPs IE FADH2/FAD GPCRs HMBC HMQC HMPA HOBt ImIm

Christian Périgaud received his Master’s and Ph.D. (1991) degrees in Chemistry from the University of Montpellier (France), where he worked with Professor J. L. Imbach and Dr. G. Gosselin on the synthesis of nucleoside analogues. Then, Dr. Périgaud held a postdoctoral position at the University of Alabama in Birmingham, working with Professor J.-P. Sommadossi. When he returned to France in 1994, he joined the University of Montpellier (France) as an Assistant Professor. Nominated Full Professor in 2001, he was the group leader of the Nucleosides & Phosphorylated Effectors research team until 2014. His main areas of expertise and interest concern the organic and medicinal chemistry of nucleosides, nucleotides, and related prodrugs, as well as their analysis. He is coauthor of over 100 publications and eight patents. Suzanne Peyrottes studied organic chemistry at the University of Montpellier (France). In 1992, she joined the Laboratory of Prof. J. L. Imbach (Montpellier, France) and obtained her Ph.D. in 1995 under the direction of Dr J. J. Vasseur, working on the synthesis and study of modified oligonucleotides. In 1996, she joined the group Dr. M. J. Gait at MRC (Cambridge, U.K.) as a Postdoctoral Fellow, where she worked on the solid-phase synthesis of oligonucleotide−peptide conjugates. In 1998, she joined the laboratory of Dr G. Gosselin (Montpellier, France) to focus on the synthesis of antitumoral mononucleotide prodrugs. A year later, she was appointed by CNRS as senior scientist. Today, she is research director at CNRS (France) and is working on the design of potential therapeutic agents to treat infections and cancers, in addition to a new synthetic methodology related to nucleic acid components. She is coauthor of about 50 publications and five patents.

ACKNOWLEDGMENTS We gratefully acknowledge Gilles Gosselin and Isis Olivier for proofreading and Marie-Christine Bergogne for the bibliography database update. We also thank Géraldine Petitclerc for creating the graphical abstract. We are thankful for the financial support provided by the Université de Montpellier (Ph.D. grant for A.D.). ABBREVIATIONS 3TC β-L-2′,3′-dideoxy-3′-thiacytidine ADP adenosine 5′-diphosphate AICAR 5-amino-1-β- D -ribofuranosylimidazole-4carboxamide AMP adenosine 5′-monophosphate AraC β-D-arabinofuranosylcytosine ATP adenosine 5′-triphosphate AZT 3′-azido-2′,3′-dideoxythymidine cAMP adenosine 3′,5′-cyclic monophosphate CBz carboxybenzyl CDI 1,1′-carbonyldiimidazole c-di-AMP cyclic diadenosine monophosphate cDN cyclic dinucleotide cGMP guanosine 3′,5-cyclic monophosphate cNMPs cyclic nucleoside monophosphates COSY correlation spectroscopy CPG controlled pore glass cycloSal cyclosaligenyl DABCO 1,4-diazabicyclo[2.2.2]octane DBU 1,8-diazabicyclo[5.4.0]undec-7-ene DCC N,N′-dicyclohexylcarbodiimide DCI 4,5-dicyanoimidazole DCSO (−)-8,8-dichlorocamphorylsulfonyl)oxaziridine ddC 2′,3′-dideoxycytidine DIC N,N′-diisopropylcarbodiimide

REFERENCES (1) Tornroth-Horsefield, S.; Neutze, R. Opening and Closing the Metabolite Gate. Proc. Natl. Acad. Sci. U. S. A. 2008, 105 (50), 19565− 19566. (2) Seifert, R.; Schneider, E. H.; Baehre, H. From Canonical to NonCanonical Cyclic Nucleotides as Second Messengers: Pharmacological Implications. Pharmacol. Ther. 2015, 148, 154−184. (3) Delicado, E. G.; Miras-Portugal, M. T.; Carrasquero, L. M. G.; Leon, D.; Perez-Sen, R.; Gualix, J. Dinucleoside Polyphosphates and their Interaction with other Nucleotide Signaling Pathways. Pfluegers Arch. 2006, 452 (5), 563−572. (4) Jankowski, V.; van der Giet, M.; Mischak, H.; Morgan, M.; Zidek, W.; Jankowski, J. Dinucleoside Polyphosphates: Strong Endogenous Agonists of the Purinergic System. Br. J. Pharmacol. 2009, 157 (7), 1142−1153. 7890


Chemical Reviews

Review

(26) Hollenstein, M. Nucleoside TriphosphatesBuilding Blocks for the Modification of Nucleic Acids. Molecules 2012, 17 (11), 13569− 13591. (27) Jessen, H. J.; Ahmed, N.; Hofer, A. Phosphate Esters and AnhydridesRecent Strategies Targeting Nature’s Favoured Modifications. Org. Biomol. Chem. 2014, 12 (22), 3526−3530. (28) Johnson, D. C., II; Widlanski, T. S. Overview of the Synthesis of Nucleoside Phosphates and Polyphosphates. In Current Protocols in Nucleic Acid Chemistry; John Wiley & Sons: New York, 2003; Vol. 15, Unit 13.1. (29) Kore, A. R.; Srinivasan, B. Recent Advances in the Syntheses of Nucleoside Triphosphates. Curr. Org. Synth. 2013, 10 (6), 903−934. (30) Murphy, P. J. D. Organophosphorus Reagents: A Practical Approach in Chemistry; Oxford University Press: Oxford, U.K., 2004; Vol. 9, pp 237−272. (31) Sherstyuk, Y. V.; Abramova, T. V. How to Form a Phosphate Anhydride Linkage in Nucleotide Derivatives. ChemBioChem 2015, 16 (18), 2562−2570. (32) Tanaka, H. Recent Approaches to the Chemical Synthesis of Sugar Nucleoside Diphosphates. Trends Glycosci. Glycotechnol. 2015, 27 (155), 99−110. (33) Vaghefi, M. M., Ed. Nucleoside Triphosphates and Their Analogs; CRC Press: Boca Raton, FL, 2005. (34) Xu, Z. A Review on the Chemical Synthesis of Pyrophosphate Bonds in Bioactive Nucleoside Diphosphate Analogs. Bioorg. Med. Chem. Lett. 2015, 25 (18), 3777−3783. (35) Van Rompay, A. R.; Johansson, M.; Karlsson, A. Substrate Specificity and Phosphorylation of Antiviral and Anticancer Nucleoside Analogues by Human Deoxyribonucleoside Kinases and Ribonucleoside Kinases. Pharmacol. Ther. 2003, 100 (2), 119−139. (36) Erb, L.; Weisman, G. A. Coupling of P2Y Receptors to G Proteins and other Signaling Pathways. Wiley Interdiscip. Rev.: Membr. Transp. Signaling 2012, 1 (6), 789−803. (37) Jacobson, K. A.; Paoletta, S.; Katritch, V.; Wu, B.; Gao, Z.-G.; Zhao, Q.; Stevens, R. C.; Kiselev, E. Nucleotides Acting at P2Y Receptors: Connecting Structure and Function. Mol. Pharmacol. 2015, 88 (2), 220−230. (38) Lazarowski, E. R.; Boucher, R. C.; Harden, T. K. Mechanisms of Release of Nucleotides and Integration of Their Action as P2X- and P2Y-Receptor Activating Molecules. Mol. Pharmacol. 2003, 64 (4), 785−795. (39) Lassila, J. K.; Zalatan, J. G.; Herschlag, D. Biological PhosphorylTransfer Reactions: Understanding Mechanism and Catalysis. Annu. Rev. Biochem. 2011, 80, 669−702. (40) Johnson, L. N. The Regulation of Protein Phosphorylation. Biochem. Soc. Trans. 2009, 37, 627−641. (41) Frey, P. A.; Hegeman, A. D. Chemical and Stereochemical Actions of UDP-Galactose 4-Epimerase. Acc. Chem. Res. 2013, 46 (7), 1417− 1426. (42) Blackburn, G. M.; Gait, M. J.; Loakes, D.; Williams, D. M. DNA and RNA Structure. In Nucleic Acids in Chemistry and Biology, 3rd ed.; The Royal Society of Chemistry: London, 2006; Chapter 2, pp 13−76. (43) Simons, C. Nucleoside Mimetics: Their Chemistry and Biological Properties; Gordon & Breach Science Publishers: Philadelphia, PA, 2000. (44) Altona, C.; Sundaralingam, M. Conformational Analysis of the Sugar Ring in Nucleosides and Nucleotides. A New Description Using the Concept of Pseudorotation. J. Am. Chem. Soc. 1972, 94 (23), 8205− 8212. (45) Luyten, I.; Thibaudeau, C.; Chattopadhyaya, J. The Strength of the Anomeric Effect in Adenosine, Guanosine, and in their 2′-Deoxy Counterparts is Medium-Dependent. J. Org. Chem. 1997, 62 (25), 8800−8808. (46) Plavec, J.; Tong, W. M.; Chattopadhyaya, J. How do the Gauche and Anomeric Effects Drive the Pseudorotational Equilibrium of the Pentofuranose Moiety of Nucleosides. J. Am. Chem. Soc. 1993, 115 (21), 9734−9746. (47) Saenger, W. Principles of Nucleic Acid Structure; Springer: New York, 1984.

(5) Clivio, P.; Coantic-Castex, S.; Guillaume, D. (3′-5′)-Cyclic Dinucleotides: Synthetic Strategies and Biological Potential. Chem. Rev. 2013, 113 (10), 7354−7401. (6) Danilchanka, O.; Mekalanos, J. J. Cyclic Dinucleotides and the Innate Immune Response. Cell 2013, 154 (5), 962−970. (7) Gomelsky, M. cAMP, c-di-GMP, c-di-AMP and now cGMP: Bacteria Use Them All! Mol. Microbiol. 2011, 79 (3), 562−565. (8) Sureka, K.; Choi, P. H.; Precit, M.; Delince, M.; Pensinger, D. A.; Huynh, T. N.; Jurado, A. R.; Goo, Y. A.; Sadilek, M.; Iavarone, A. T.; et al. The Cyclic Dinucleotide c-di-AMP is an Allosteric Regulator of Metabolic Enzyme Function. Cell 2014, 158 (6), 1389−1401. (9) Thibodeaux, C. J.; Melancon, C. E., III; Liu, H.-w. Natural-Product Sugar Biosynthesis and Enzymatic Glycodiversification. Angew. Chem., Int. Ed. 2008, 47 (51), 9814−9859. (10) Wagner, G. K.; Pesnot, T.; Field, R. A. A Survey of Chemical Methods for Sugar-Nucleotide Synthesis. Nat. Prod. Rep. 2009, 26 (9), 1172−1194. (11) De Tullio, M. C. The Mystery of Vitamin C. Nat. Educ. 2010, 3 (9), 48. (12) Rosemeyer, H. Nucleolipids: Natural Occurrence, Synthesis, Molecular Recognition, and Supramolecular Assemblies as Potential Precursors of Life and Bioorganic Materials. Chem. Biodiversity 2005, 2 (8), 977−1062. (13) Fahy, E.; Subramaniam, S.; Brown, H. A.; Glass, C. K.; Merrill, A. H.; Murphy, R. C.; Raetz, C. R. H.; Russell, D. W.; Seyama, Y.; Shaw, W.; et al. A Comprehensive Classification System for Lipids. J. Lipid Res. 2005, 46 (5), 839−862. (14) Allain, V.; Bourgaux, C.; Couvreur, P. Self-Assembled Nucleolipids: From Supramolecular Structure to Soft Nucleic Acid and Drug Delivery Devices. Nucleic Acids Res. 2012, 40 (5), 1891−1903. (15) Gangadhara, K.; Srivastava, P.; Rozenski, J.; Mattelaer, H.-P.; Leen, V.; Dehaen, W.; Hofkens, J.; Lescrinier, E.; Herdewijn, P. Design and Synthesis of Nucleolipids as Possible Activated Precursors for Oligomer Formation via Intramolecular Catalysis: Stability Study and Supramolecular Organization. J. Syst. Chem. 2014, 5 (1), 5. (16) Gissot, A.; Camplo, M.; Grinstaff, M. W.; Barthelemy, P. Nucleoside, Nucleotide and Oligonucleotide Based Amphiphiles: A Successful Marriage of Nucleic Acids with Lipids. Org. Biomol. Chem. 2008, 6 (8), 1324−1333. (17) Latxague, L.; Patwa, A.; Amigues, E.; Barthelemy, P. GlycosylNucleolipids as New Bioinspired Amphiphiles. Molecules 2013, 18 (10), 12241−12263. (18) Simeone, L.; Mangiapia, G.; Irace, C.; Di Pascale, A.; Colonna, A.; Ortona, O.; De Napoli, L.; Montesarchio, D.; Paduano, L. Nucleolipid Nanovectors as Molecular Carriers for Potential Applications in Drug Delivery. Mol. BioSyst. 2011, 7 (11), 3075−3086. (19) Taib, N.; Aime, A.; Houmadi, S.; Castano, S.; Barthelemy, P.; Laguerre, M.; Bestel, I. Chemical Details on Nucleolipid Supramolecular Architecture: Molecular Modeling and Physicochemical Studies. Langmuir 2012, 28 (19), 7452−7460. (20) Mizusawa, S.; Nishimura, S.; Seela, F. Improvement of the Dideoxy Chain Termination Method of DNA Sequencing by Use of Deoxy-7-Deazaguanosine Triphosphate in Place of dGTP. Nucleic Acids Res. 1986, 14 (3), 1319−1324. (21) Morozova, O.; Hirst, M.; Marra, M. A. Applications of New Sequencing Technologies for Transcriptome Analysis. Annu. Rev. Genomics Hum. Genet. 2009, 10, 135−151. (22) Morozova, O.; Marra, M. A. Applications of Next-Generation Sequencing Technologies in Functional Genomics. Genomics 2008, 92 (5), 255−264. (23) Sanger, F.; Nicklen, S.; Coulson, A. R. DNA Sequencing with Chain-Terminating Inhibitors. Proc. Natl. Acad. Sci. U. S. A. 1977, 74 (12), 5463−5467. (24) Su, Z.; Ning, B.; Fang, H.; Hong, H.; Perkins, R.; Tong, W.; Shi, L. Next-Generation Sequencing and Its Applications in Molecular Diagnostics. Expert Rev. Mol. Diagn. 2011, 11 (3), 333−343. (25) Burgess, K.; Cook, D. Syntheses of Nucleoside Triphosphates. Chem. Rev. 2000, 100 (6), 2047−2059. 7891


Chemical Reviews

Review

(67) Mitra, R. P.; Malhotra, H. C.; Jain, D. V. S. Dissociation Equilibria in Pyrophosphates and Kinetics of Degradation.I. Dissociation Constants of Pyrophosphoric Acid. Trans. Faraday Soc. 1966, 62 (517P), 167−172. (68) Krishnamurthy, R. Role of pKa of Nucleobases in the Origins of Chemical Evolution. Acc. Chem. Res. 2012, 45 (12), 2035−2044. (69) Westheimer, F. H. Why Nature Chose Phosphates. Science 1987, 235 (4793), 1173−1178. (70) Jancan, I.; Macnaughtan, M. A. Acid Dissociation Constants of Uridine-5′-diphosphate Compounds Determined by 31Phosphorus Nuclear Magnetic Resonance Spectroscopy and Internal pH Referencing. Anal. Chim. Acta 2012, 749, 63−69. (71) Corfu, N. A.; Sigel, H. Acid-Base Properties of Nucleosides and Nucleotides as a Function of Concentration: Comparison of the Proton Affinity of the Nucleic Base Residues in the Monomeric and SelfAssociated, Oligomeric 5′-Triphosphates of Inosine (ITP), Guanosine (GTP), and Adenosine (ATP). Eur. J. Biochem. 1991, 199 (3), 659−669. (72) Massoud, S. S.; Sigel, H. Metal Ion Coordinating Properties of Pyrimidine-Nucleoside 5′-Monophosphates (CMP, UMP, TMP) and of Simple Phosphate Monoesters, Including D-Ribose 5′-Monophosphate. Establishment of Relations Between Complex Stability and Phosphate Basicity. Inorg. Chem. 1988, 27 (8), 1447−1453. (73) Mistry, D.; Powles, N. The Relative Hydrolytic Reactivities of Pyrophosphites and Pyrophosphates. Org. Biomol. Chem. 2013, 11 (34), 5727−5733. (74) Stockbridge, R. B.; Wolfenden, R. The Intrinsic Reactivity of ATP and the Catalytic Proficiencies of Kinases Acting on Glucose, NAcetylgalactosamine, and Homoserine A Thermodynamic Analysis. J. Biol. Chem. 2009, 284 (34), 22747−22757. (75) Lad, C.; Williams, N. H.; Wolfenden, R. The Rate of Hydrolysis of Phosphomonoester Dianions and the Exceptional Catalytic Proficiencies of Protein and Inositol Phosphatases. Proc. Natl. Acad. Sci. U. S. A. 2003, 100 (10), 5607−5610. (76) Schroeder, G. K.; Lad, C.; Wyman, P.; Williams, N. H.; Wolfenden, R. The Time Required for Water Attack at the Phosphorus Atom of Simple Phosphodiesters and of DNA. Proc. Natl. Acad. Sci. U. S. A. 2006, 103 (11), 4052−4055. (77) Cleland, W. W.; Hengge, A. C. Enzymatic Mechanisms of Phosphate and Sulfate Transfer. Chem. Rev. 2006, 106 (8), 3252−3278. (78) Hengge, A. C.; Onyido, I. Physical Organic Perspectives on Phospho Group Transfer from Phosphates and Phosphinates. Curr. Org. Chem. 2005, 9 (1), 61−74. (79) Wolfenden, R. Degrees of Difficulty of Water-Consuming Reactions in the Absence of Enzymes. Chem. Rev. 2006, 106 (8), 3379−3396. (80) Shaver, S. R.; Rideout, J. L.; Pendergast, W.; Douglass, J. G.; Brown, E. G.; Boyer, J. L.; Patel, R. I.; Redick, C. C.; Jones, A. C.; Picher, M.; et al. Structure-Activity Relationships of Dinucleotides: Potent and Selective Agonists of P2Y Receptors. Purinergic signalling 2005, 1 (2), 183−191. (81) Huhta, E.; Parjanen, A.; Mikkola, S. A Kinetic Study on the Chemical Cleavage of Nucleoside Diphosphate Sugars. Carbohydr. Res. 2010, 345 (5), 696−703. (82) Warnecke, S.; Meier, C. Synthesis of Nucleoside Di- and Triphosphates and Dinucleoside Polyphosphates with cycloSal-Nucleotides. J. Org. Chem. 2009, 74 (8), 3024−3030. (83) Quin, V. L. D.; Williams, A. J. Practical Interpretation of P-31 NMR Spectra and Computer-Assisted Structure Verification; Advanced Chemistry Development: Toronto, Ontario, 2004. (84) Thapar, R. Contribution of Protein Phosphorylation to BindingInduced Folding of the SLBP-Histone mRNA Complex Probed by Phosphorus-31 NMR. FEBS Open Bio 2014, 4, 853−857. (85) Bothwell, J. H. F.; Griffin, J. L. An Introduction to Biological Nuclear Magnetic Resonance Spectroscopy. Biol. Rev. 2011, 86 (2), 493−510. (86) DeSilva, M. A.; Shanaiah, N.; Nagana Gowda, G. A.; Rosa-Perez, K.; Hanson, B. A.; Raftery, D. Application of 31P NMR Spectroscopy and Chemical Derivatization for Metabolite Profiling of Lipophilic Compounds in Human Serum. Magn. Reson. Chem. 2009, 47, S74−S80.

(48) Thibaudeau, C.; Plavec, J.; Chattopadhyaya, J. Quantitation of the Anomeric Effect in Adenosine and Guanosine by Comparison of the Thermodynamics of the Pseudorotational Equilibrium of the Pentofuranose Moiety, in N-Nucleosides and C-Nucleosides. J. Am. Chem. Soc. 1994, 116 (18), 8033−8037. (49) Barchi, J. J., Jr.; Karki, R. G.; Nicklaus, M. C.; Siddiqui, M. A.; George, C.; Mikhailopulo, I. A.; Marquez, V. E. Comprehensive Structural Studies of 2′,3′-Difluorinated Nucleosides: Comparison of Theory, Solution, and Solid State. J. Am. Chem. Soc. 2008, 130 (28), 9048−9057. (50) Lebreton, J.; Escudier, J.-M.; Arzel, L.; Len, C. Synthesis of Bicyclonucleosides Having a C-C Bridge. Chem. Rev. 2010, 110 (6), 3371−3418. (51) Ludek, O. R.; Marquez, V. E. Synthesis of Conformationally North-Locked Pyrimidine Nucleosides Built on an Oxabicyclo 3.1.0 Hexane Scaffold. J. Org. Chem. 2012, 77 (2), 815−824. (52) Marquez, V. E. The Properties of Locked Methanocarba Nucleosides in Biochemistry, Biotechnology, and Medicinal Chemistry. In Modified Nucleosides; Herdewijn, P., Ed.; Wiley-VCH: Weinheim, Germany, 2008; Chapter 12, pp 305−341. (53) Mathe, C.; Perigaud, C. Recent Approaches in the Synthesis of Conformationally Restricted Nucleoside Analogues. Eur. J. Org. Chem. 2008, 2008 (9), 1489−1505. (54) Zhou, C.; Plashkevych, O.; Chattopadhyaya, J. Double Sugar and Phosphate Backbone-Constrained Nucleotides: Synthesis, Structure, Stability, and their Incorporation into Oligodeoxynucleotides. J. Org. Chem. 2009, 74 (9), 3248−3265. (55) Evans, F. E.; Sarma, R. H. Nucleotide Rigidity. Nature 1976, 263 (5578), 567−572. (56) Vijayaiakshmi, K. S.; Yathindra, N. Conformational Analysis of Nucleoside and Nucleotide Antibiotics Possessing Five-Membered Base RingsA Comparison of the Glycosyl Barrier for Purine, Pyrimidine and Imidazole Rings. Biochim. Biophys. Acta, Nucleic Acids Protein Synth. 1980, 607 (1), 171−186. (57) Yathindra, N.; Sundaralingam, M. Conformational-Analysis of Arabinonucleosides and NucleotidesComparison with the Ribonucleosides and Nucleotides. Biochim. Biophys. Acta, Nucleic Acids Protein Synth. 1979, 564 (2), 301−310. (58) Sigel, H.; Griesser, R. Nucleoside 5′-Triphosphates: SelfAssociation, Acid-Base, and Metal Ion-Binding Properties in Solution. Chem. Soc. Rev. 2005, 34 (10), 875−900. (59) Altona, C.; Sundaralingam, M. Conformational Analysis of the Sugar Ring in Nucleosides and Nucleotides. Improved Method for the Interpretation of Proton Magnetic Resonance Coupling Constants. J. Am. Chem. Soc. 1973, 95 (7), 2333−2344. (60) Davies, D. B. Conformation of Nucleosides and Nucleotides. Prog. Nucl. Magn. Reson. Spectrosc. 1978, 12 (3), 135−225. (61) Shishkin, O. V.; Palamarchuk, G. V.; Gorb, L.; Leszczynski, J. Intramolecular Hydrogen Bonds in Canonical 2′-Deoxyribonucleotides: An Atoms in Molecules Study. J. Phys. Chem. B 2006, 110 (9), 4413− 4422. (62) Stern, N.; Major, D. T.; Gottlieb, H. E.; Weizman, D.; Fischer, B. What is the Conformation of Physiologically-Active Dinucleoside Polyphosphates in Solution? Conformational Analysis of Free Dinucleoside Polyphosphates by NMR and Molecular Dynamics Simulations. Org. Biomol. Chem. 2010, 8 (20), 4637−4652. (63) Che, X.; Zhang, J.; Zhu, Y.; Yang, L.; Quan, H.; Gao, Y. Q. Structural Flexibility and Conformation Features of Cyclic Dinucleotides in Aqueous Solutions. J. Phys. Chem. B 2016, 120 (10), 2670−2680. (64) Blackburn, G. M.; Gait, M. J.; Loakes, D.; Williams, D. M. Nucleosides and Nucleotides. In Nucleic Acids in Chemistry and Biology, 3rd ed.; The Royal Society of Chemistry: London, 2006; Chapter 3, pp 77−142. (65) Cavaluzzi, M. J.; Borer, P. N. Revised UV Extinction Coefficients for Nucleoside-5′-Monophosphates and Unpaired DNA and RNA. Nucleic Acids Res. 2004, 32 (1), e13. (66) Velikyan, I.; Acharya, S.; Trifonova, A.; Foldesi, A.; Chattopadhyaya, J. The pKa’s of 2′-Hydroxyl Group in Nucleosides and Nucleotides. J. Am. Chem. Soc. 2001, 123 (12), 2893−2894. 7892


Chemical Reviews

Review

Chain-Terminating Dideoxynucleotides. Science 1987, 238 (4825), 336−341. (106) Smith, L. M.; Sanders, J. Z.; Kaiser, R. J.; Hughes, P.; Dodd, C.; Connell, C. R.; Heiner, C.; Kent, S. B. H.; Hood, L. E. Fluorescence Detection in Automated DNA-Sequence Analysis. Nature 1986, 321 (6071), 674−679. (107) Hollenstein, M.; Smith, C. C.; Raez, M. Nucleoside TriphosphatesFrom Synthesis to Biochemical Characterization. J. Visualized Exp. 2014, 86, e51385. (108) Vaught, J. D.; Bock, C.; Carter, J.; Fitzwater, T.; Otis, M.; Schneider, D.; Rolando, J.; Waugh, S.; Wilcox, S. K.; Eaton, B. E. Expanding the Chemistry of DNA for In Vitro Selection. J. Am. Chem. Soc. 2010, 132 (12), 4141−4151. (109) Jordheim, L. P.; Durantel, D.; Zoulim, F.; Dumontet, C. Advances in the Development of Nucleoside and Nucleotide Analogues for Cancer and Viral Diseases. Nat. Rev. Drug Discovery 2013, 12 (6), 447−464. (110) Varga, A.; Lionne, C.; Roy, B. Intracellular Metabolism of Nucleoside/Nucleotide Analogues: A Bottleneck to Reach Active Drugs on HIV Reverse Transcriptase. Curr. Drug Metab. 2016, 17 (3), 237− 252. (111) Lau, O. C. F.; Samarawickrama, C.; Skalicky, S. E. P2Y2 Receptor Agonists for the Treatment of Dry Eye Disease: A Review. Clin. Ophthalmol. 2014, 8, 327−334. (112) Yanachkov, I. B.; Chang, H.; Yanachkova, M. I.; Dix, E. J.; BernyLang, M. A.; Gremmel, T.; Michelson, A. D.; Wright, G. E.; Frelinger, A. L., III. New Highly Active Antiplatelet Agents with Dual Specificity for Platelet P2Y(1) and P2Y(12) Adenosine Diphosphate Receptors. Eur. J. Med. Chem. 2016, 107, 204−218. (113) Khiati, S.; Pierre, N.; Andriamanarivo, S.; Grinstaff, M. W.; Arazam, N.; Nallet, F.; Navailles, L.; Barthelemy, P. Anionic NucleotideLipids for In Vitro DNA Transfection. Bioconjugate Chem. 2009, 20 (9), 1765−1772. (114) Pradere, U.; Garnier-Amblard, E. C.; Coats, S. J.; Amblard, F.; Schinazi, R. F. Synthesis of Nucleoside Phosphate and Phosphonate Prodrugs. Chem. Rev. 2014, 114 (18), 9154−9218. (115) Kraszewski, A.; Stawinski, J. H-Phosphonates: Versatile Synthetic Precursors to Biologically Active Phosphorus Compounds. Pure Appl. Chem. 2007, 79 (12), 2217−2227. (116) El-Tayeb, A.; Qi, A. D.; Muller, C. E. Synthesis and Structure− Activity Relationships of Uracil Nucleotide Derivatives and Analogues as Agonists at Human P2Y2, P2Y4, and P2Y6 Receptors. J. Med. Chem. 2006, 49 (24), 7076−7087. (117) Kolodziej, K.; Romanowska, J.; Stawinski, J.; Kraszewski, A.; Sobkowski, M. The Case of Triethylammonium Cation Loss during Purification of certain Nucleotide Analogues: A Cautionary Note. Anal. Bioanal. Chem. 2015, 407 (6), 1775−1780. (118) Korhonen, H. J.; Bolt, H. L.; Hodgson, D. R. W. A Procedure for the Preparation and Isolation of Nucleoside-5′-diphosphates. Beilstein J. Org. Chem. 2015, 11, 469−472. (119) Korhonen, H. J.; Bolt, H. L.; Vicente-Gines, L.; Perks, D. C.; Hodgson, D. R. W. PPN Pyrophosphate: A New Reagent for the Preparation of Nucleoside Triphosphates. Phosphorus, Sulfur Silicon Relat. Elem. 2015, 190 (5−6), 758−762. (120) Wu, W. D.; Bergstrom, D. E.; Davisson, V. J. A Combination Chemical and Enzymatic Approach for the Preparation of Azole Carboxamide Nucleoside Triphosphate. J. Org. Chem. 2003, 68 (10), 3860−3865. (121) Merrifield, R. B. Solid Phase Peptide Synthesis 0.1. Synthesis of a Tetrapeptide. J. Am. Chem. Soc. 1963, 85 (14), 2149−2154. (122) Geckeler, K. E. Soluble Polymer Supports for Liquid-Phase Synthesis. Adv. Polym. Sci. 1995, 121, 31−79. (123) Gravert, D. J.; Janda, K. D. Organic Synthesis on Soluble Polymer Supports: Liquid-Phase Methodologies. Chem. Rev. 1997, 97 (2), 489−509. (124) Skoda-Foeldes, R. The Use of Supported Acidic Ionic Liquids in Organic Synthesis. Molecules 2014, 19 (7), 8840−8884. (125) Toy, P. H.; Janda, K. D. Soluble Polymer-Supported Organic Synthesis. Acc. Chem. Res. 2000, 33 (8), 546−554.

(87) Muruganandham, M.; Alfieri, A. A.; Matei, C.; Chen, Y.; Sukenick, G.; Schemainda, I.; Hasmann, M.; Saltz, L. B.; Koutcher, J. A. Metabolic Signatures Associated with a NAD Synthesis Inhibitor-Induced Tumor Apoptosis Identified by 1H-Decoupled-31P Magnetic Resonance Spectroscopy. Clin. Cancer Res. 2005, 11 (9), 3503−3513. (88) Renou, J.-P.; Webb, G. A.; Belton, P. S. Magnetic Resonance in Food Science: An Exciting Future; The Royal Society of Chemistry. London, 2011. (89) Spyros, A.; Dais, P. 31P NMR Spectroscopy in Food Analysis. Prog. Nucl. Magn. Reson. Spectrosc. 2009, 54 (3−4), 195−207. (90) Lebedev, A. V.; Rezvukhin, A. I. Tendencies of 31P ChemicalShifts Changes in NMR Spectra of Nucleotide Derivatives. Nucleic Acids Res. 1984, 12 (14), 5547−5566. (91) Wolf, S.; Warnecke, S.; Ehrit, J.; Freiberger, F.; Gerardy-Schahn, R.; Meier, C. Chemical Synthesis and Enzymatic Testing of CMP-Sialic Acid Derivatives. ChemBioChem 2012, 13 (17), 2605−2615. (92) Ghezal, S.; Thomasson, M. S.; Lefebvre-Tournier, I.; Périgaud, C.; Macnaughtan, M. A.; Roy, B. CDP-Ethanolamine and CDP-Choline: One-Pot Synthesis and 31P NMR Study. Tetrahedron Lett. 2014, 55, 5306−5310. (93) Kuesel, A. C.; Graschew, G.; Hull, W. E.; Lorenz, W.; Thielmann, H. W. 31P NMR Studies of Cultured Human Tumor Cells. Influence of pH on Phospholipid Metabolite Levels and the Detection of Cytidine 5′-Diphosphate Choline. NMR Biomed. 1990, 3 (2), 78−89. (94) Ragg, E.; Scaglioni, L.; Mondelli, R.; Carelli, I.; Casini, A.; Tortorella, S. 1H, 13C, 31P-NMR Studies and Conformational Analysis of NADP+, NADPH Coenzymes and of Dimers from Electrochemical Reduction of NADP+. Biochim. Biophys. Acta, Protein Struct. Mol. Enzymol. 1991, 1076 (1), 49−60. (95) Robitaille, P.-M. L.; Robitaille, P. A.; Brown, G. G., Jr.; Brown, G. G. An Analysis of the pH-Dependent Chemical-Shift Behavior of Phosphorus-Containing Metabolites. J. Magn. Reson. 1991, 92 (1), 73− 84. (96) Tanaka, H.; Yoshimura, Y.; Jorgensen, M. R.; Cuesta-Seijo, J. A.; Hindsgaul, O. A Simple Synthesis of Sugar Nucleoside Diphosphates by Chemical Coupling in Water. Angew. Chem., Int. Ed. 2012, 51 (46), 11531−11534. (97) Banoub, J. H.; Newton, R. P.; Esmans, E.; Ewing, D. F.; Mackenzie, G. Recent Developments in Mass Spectrometry for the Characterization of Nucleosides, Nucleotides, Oligonucleotides, and Nucleic Acids. Chem. Rev. 2005, 105 (5), 1869−1915. (98) Dudley, E.; Bond, L. Mass Spectrometry Analysis of Nucleosides and Nucleotides. Mass Spectrom. Rev. 2014, 33 (4), 302−331. (99) Huang, D.; Zhang, Y. H.; Chen, X. G. Analysis of Intracellular Nucleoside Triphosphate Levels in Normal and Tumor Cell Lines by High-Performance Liquid Chromatography. J. Chromatogr. B: Anal. Technol. Biomed. Life Sci. 2003, 784 (1), 101−109. (100) Cohen, S.; Jordheim, L. P.; Megherbi, M.; Dumontet, C.; Guitton, J. Liquid Chromatographic Methods for the Determination of Endogenous Nucleotides and Nucleotide Analogs Used in Cancer Therapy: A Review. J. Chromatogr. B: Anal. Technol. Biomed. Life Sci. 2010, 878 (22), 1912−1928. (101) Thomas, D.; Herold, N.; Keppler, O. T.; Geisslinger, G.; Ferreiros, N. Quantitation of Endogenous Nucleoside Triphosphates and Nucleosides in Human Cells by Liquid Chromatography Tandem Mass Spectrometry. Anal. Bioanal. Chem. 2015, 407 (13), 3693−3704. (102) Bajad, S. U.; Lu, W.; Kimball, E. H.; Yuan, J.; Peterson, C.; Rabinowitz, J. D. Separation and Quantitation of Water Soluble Cellular Metabolites by Hydrophilic Interaction Chromatography-Tandem Mass Spectrometry. J. Chromatogr. A 2006, 1125 (1), 76−88. (103) Buszewski, B.; Noga, S. Hydrophilic Interaction Liquid Chromatography (HILIC)-A Powerful Separation Technique. Anal. Bioanal. Chem. 2012, 402 (1), 231−247. (104) Hemstrom, P.; Irgum, K. Hydrophilic Interaction Chromatography. J. Sep. Sci. 2006, 29 (12), 1784−1821. (105) Prober, J. M.; Trainor, G. L.; Dam, R. J.; Hobbs, F. W.; Robertson, C. W.; Zagursky, R. J.; Cocuzza, A. J.; Jensen, M. A.; Baumeister, K. A System for Rapid DNA Sequencing with Fluorescent 7893


Chemical Reviews

Review

(147) Krenitsky, T. A.; Tuttle, J. V.; Miller, W. H.; Moorman, A. R.; Orr, G. F.; Beauchamp, L. Nucleotide Analogue Inhibitors of Purine Nucleoside Phosphorylase. J. Biol. Chem. 1990, 265 (6), 3066−3069. (148) Sauer, R.; El-Tayeb, A.; Kaulich, M.; Mueller, C. E. Synthesis of Uracil Nucleotide Analogs with a Modified, Acyclic Ribose Moiety as P2Y(2) Receptor Antagonists. Bioorg. Med. Chem. 2009, 17 (14), 5071− 5079. (149) Yamaguchi, T.; Saneyoshi, M.; Takahashi, H.; Hirokawa, S.; Amano, R.; Liu, X.; Inomata, M.; Maruyama, T. Synthetic Nucleosides and Nucleotides. 43. Inhibition of Vertebrate Telomerases by Carbocyclic Oxetanocin G (C.OXT-G) Triphosphate Analogues and Influence of C.OXT-G Treatment on Telomere Length in Human HL60 Cells. Nucleosides, Nucleotides Nucleic Acids 2006, 25 (4−6), 539− 551. (150) Vanboom, J. H.; Crea, R.; Luyten, W. C.; Vink, A. B. 2,2,2Tribromoethyl PhosphoromorpholinochloridateConvenient Reagent for Synthesis of Ribonucleoside Mono-Phosphates, DiPhosphates and Tri-Phosphates. Tetrahedron Lett. 1975, 16 (32), 2779−2782. (151) Scheit, K. H. Die Synthese der 5′-Diphosphate von 5Methyluridin 5-Hydroxymethyl-Uridin und 3,5-Dimethyluridin. Chem. Ber. 1966, 99 (12), 3884−3891. (152) Taktakishvili, M.; Nair, V. A New Method for the Phosphorylation of Nucleosides. Tetrahedron Lett. 2000, 41 (37), 7173−7176. (153) Kimura, J.; Fujisawa, Y.; Yoshizawa, T.; Fukuda, K.; Mitsunobu, O. Studies on Nucleosides and Nucleotides 0.7. Preparation of Pyrimidine Nucleoside 5′-Phosphates and N3,5′-Purine Cyclonucleosides by Selective Activation of the 5′-Hydroxyl Group. Bull. Chem. Soc. Jpn. 1979, 52 (4), 1191−1196. (154) Choi, Y. S.; George, C.; Comin, M. J.; Barchi, J. J., Jr.; Kim, H. S.; Jacobson, K. A.; Balzarini, J.; Mitsuya, H.; Boyer, P. L.; Hughes, S. H.; Marquez, V. E. qA Conformationally Locked Analogue of the Anti-HIV Agent Stavudine. An Important Correlation between Pseudorotation and Maximum Amplitude. J. Med. Chem. 2003, 46 (15), 3292−3299. (155) Costanzi, S.; Joshi, B. V.; Maddileti, S.; Mamedova, L.; GonzalezMoa, M. J.; Marquez, V. E.; Harden, T. K.; Jacobson, K. A. Human P2Y(6) Receptor: Molecular Modeling Leads to the Rational Design of a Novel Agonist Based on a Unique Conformational Preference. J. Med. Chem. 2005, 48 (26), 8108−8111. (156) Xu, B.; Stephens, A.; Kirschenheuter, G.; Greslin, A. F.; Cheng, X. Q.; Sennelo, J.; Cattaneo, M.; Zighetti, M. L.; Chen, A. S.; Kim, S. A.; et al. Acyclic Analogues of Adenosine Bisphosphates as P2Y Receptor Antagonists: Phosphate Substitution Leads to Multiple Pathways of Inhibition of Platelet Aggregation. J. Med. Chem. 2002, 45 (26), 5694− 5709. (157) Meier, C. cycloSal-PronucleotidesDesign of Chemical Trojan Horses. Mini-Rev. Med. Chem. 2002, 2 (3), 219−234. (158) Meier, C. cycloSal Phosphates as Chemical Trojan Horses for Intracellular Nucleotide and Glycosylmonophosphate Delivery Chemistry Meets Biology. Eur. J. Org. Chem. 2006, 2006 (5), 1081− 1102. (159) Meier, C.; Balzarini, J. Application of the cycloSal-Prodrug Approach for Improving the Biological Potential of Phosphorylated Biomolecules. Antiviral Res. 2006, 71 (2−3), 282−292. (160) Meier, C.; Ruppel, M. F. H.; Vukadinovic, D.; Balzarini, J. “Lockin”-cycloSal-PronucleotidesA New Generation of Chemical Trojan Horses? Mini-Rev. Med. Chem. 2004, 4 (4), 383−394. (161) Wolf, S.; Zismann, T.; Lunau, N.; Warnecke, S.; Wendicke, S.; Meier, C. A Convenient Synthesis of Nucleoside Diphosphate Glycopyranoses and other Polyphosphorylated Bioconjugates. Eur. J. Cell Biol. 2010, 89 (1), 63−75. (162) Ludek, O. R.; Meier, C. Synthesis of Carbocyclic Nucleotides as Potential Substrates for Thymidylate Kinase. Nucleosides, Nucleotides Nucleic Acids 2005, 24 (5−7), 683−686. (163) Mahler, M.; Reichardt, B.; Hartjen, P.; van Lunzen, J.; Meier, C. Stereoselective Synthesis of D- and L-Carbocyclic Nucleosides by Enzymatically Catalyzed Kinetic Resolution. Chem. - Eur. J. 2012, 18 (35), 11046−11062.

(126) Gaur, R. K.; Sproat, B. S.; Krupp, G. Novel Solid Phase Synthesis of 2′-O-Methylribonucleoside 5′-Triphosphates and their α-Thio Analogues. Tetrahedron Lett. 1992, 33 (23), 3301−3304. (127) Ahmadibeni, Y.; Parang, K. Polymer-Bound Oxathiaphospholane: A Solid-Phase Reagent for Regioselective Monothiophosphorylation and Monophosphorylation of Unprotected Nucleosides and Carbohydrates. Org. Lett. 2005, 7 (10), 1955−1958. (128) Oliviero, G.; D’Errico, S.; Borbone, N.; Amato, J.; Piccialli, V.; Piccialli, G.; Mayol, L. Facile Solid-Phase Synthesis of AICAR 5′Monophosphate (ZMP) and its 4-N-Alkyl Derivatives. Eur. J. Org. Chem. 2010, 2010 (8), 1517−1524. (129) Parang, K.; Fournier, E. J. L.; Hindsgaul, O. A Solid Phase Reagent for the Capture Phosphorylation of Carbohydrates and Nucleosides. Org. Lett. 2001, 3 (2), 307−309. (130) Ahmadibeni, Y.; Parang, K. Selective Diphosphorylation, Dithiodiphosphorylation, Triphosphorylation, and Trithiotriphosphorylation of Unprotected Carbohydrates and Nucleosides. Org. Lett. 2005, 7 (25), 5589−5592. (131) Ahmadibeni, Y.; Parang, K. Solid-Phase Reagents for Selective Monophosphorylation of Carbohydrates and Nucleosides. J. Org. Chem. 2005, 70 (3), 1100−1103. (132) Tonn, V. C.; Meier, C. Solid-Phase Synthesis of (Poly)phosphorylated Nucleosides and Conjugates. Chem. - Eur. J. 2011, 17 (35), 9832−9842. (133) Crauste, C.; Perigaud, C.; Peyrottes, S. Insights into the Soluble PEG-Supported Synthesis of Cytosine-Containing Nucleoside 5′Mono-, Di-, and Triphosphates. J. Org. Chem. 2009, 74 (23), 9165− 9172. (134) Crauste, C.; Perigaud, C.; Peyrottes, S. Synthesis of 2′,3′Dideoxynucleoside Phosphoesters Using H-Phosphonate Chemistry on Soluble Polymer Support. J. Org. Chem. 2011, 76 (3), 997−1000. (135) Peyrottes, S.; Périgaud, C.; Crauste, C. Method for Preparing Nucleotides and Related Analogues by Synthesis on Soluble Substrate, and Biological Tools thus Prepared. WO2009115694(A1), 2009. (136) Kore, A. R.; Yang, B.; Srinivasan, B. Ionic-Tag-Assisted Synthesis of Nucleoside Triphosphates. Tetrahedron Lett. 2014, 55 (36), 5088− 5091. (137) Bradley, M.; Bruckler, C. Immobilised Reagent. International Patent WO2007110624A2, 2007. (138) Schoetzau, T.; Holletz, T.; Cech, D. A Facile Solid Phase Synthesis of 2′- and 3′-Aminonucleoside Triphosphates. Chem. Commun. 1996, No. 3, 387−388. (139) Cheng, T.-L.; Chuang, K.-H.; Chen, B.-M.; Roffler, S. R. Analytical Measurement of PEGylated Molecules. Bioconjugate Chem. 2012, 23 (5), 881−899. (140) Dupont, J.; de Souza, R. F.; Suarez, P. A. Z. Ionic Liquid (Molten Salt) Phase Organometallic Catalysis. Chem. Rev. 2002, 102 (10), 3667− 3691. (141) Patel, D. D.; Lee, J.-M. Applications of Ionic Liquids. Chem. Rec. 2012, 12 (3), 329−355. (142) Wasserscheid, P.; Keim, W. Ionic LiquidsNew “Solutions” for Transition Metal Catalysis. Angew. Chem., Int. Ed. 2000, 39 (21), 3772− 3789. (143) Wasserscheid, P.; Welton, T. Ionic Liquids in Synthesis; WileyVCH Verlag GmbH & Co: Weinheim, Germany, 2002. (144) Yoshikawa, M.; Kato, T.; Takenishi, T. A Novel Method for Phosphorylation of Nucleosides to 5′-Nucleotides. Tetrahedron Lett. 1967, 8 (50), 5065−5068. (145) Ikemoto, T.; Haze, A.; Hatano, H.; Kitamoto, Y.; Ishida, M.; Nara, K. Phosphorylation of Nucleosides with Phosphorus Oxychloride in Trialkyl Phosphate. Chem. Pharm. Bull. 1995, 43 (2), 210−215. (146) Kim, H. S.; Ravi, R. G.; Marquez, V. E.; Maddileti, S.; Wihlborg, A. K.; Erlinge, D.; Malmsjo, M.; Boyer, J. L.; Harden, T. K.; Jacobson, K. A. Methanocarba Modification of Uracil and Adenine Nucleotides: High Potency of Northern Ring Conformation at P2Y(1), P2Y(2), P2Y(4), and P2Y(11) but not P2Y(6) Receptors. J. Med. Chem. 2002, 45 (1), 208−218. 7894


Chemical Reviews

Review

(164) Roy, B.; Lefebvre, I.; Puy, J.-Y.; Périgaud, C. A Facile and Effective Synthesis of Lamivudine 5′-Diphosphate. Tetrahedron Lett. 2011, 52 (12), 1250−1252. (165) Jankowska, J.; Sobkowski, M.; Stawinski, J.; Kraszewski, A. Studies on Aryl H-Phosphonates 0.1. An Efficient Method for the Preparation of Deoxyribo- and Ribonucleoside 3′-H-Phosphonate Monoesters by Transesterification of Diphenyl H-Phosphonate. Tetrahedron Lett. 1994, 35 (20), 3355−3358. (166) Wever, R.; Babich, L.; Hartog, A. F. Transphosphorylation. In Biocatalysis in Organic Synthesis 1, 2015 ed.; Faber, K., Fessner, W. D., Turner, N. J., Eds.; Georg Thieme Verlag: Stuttgart, Germany, 2015; Vol. 1, pp 223−254. (167) Barai, V. N.; Kvach, S. V.; Zinchenko, A. I.; Mikhailopulo, I. A. An Improved Method for the Enzymatic Transformation of Nucleosides into 5′-Monophosphates. Biotechnol. Lett. 2004, 26 (24), 1847−1850. (168) Cotticelli, G.; Salvetti, R. Enzymatic Process for Preparation of 5′-Monophosphate-Nucleotides. International Patent WO2007144168A1, 2007. (169) Mishra, N. C.; Broom, A. D. A Novel Synthesis of Nucleoside 5′Triphosphates. J. Chem. Soc., Chem. Commun. 1991, 18, 1276−1277. (170) Cramer, F.; Neunhoeffer, H. Zür Chemie der Energiereichen Phosphate. 15. Reaktionen von Adenosin-5′-Phosphorsaure-Imidazolid-Eine Neue Synthese von Adenosindiphosphat und Flavin-AdeninDinucleotid. Chem. Ber. 1962, 95 (7), 1664−1669. (171) Moffatt, J. G.; Khorana, H. G. Nucleoside Polyphosphates. X. The Synthesis and Some Reactions of Nucleoside-5′ Phosphoromorpholidates and Related Compounds. Improved Methods for the Preparation of Nucleoside-5′ Polyphosphates. J. Am. Chem. Soc. 1961, 83 (3), 649−658. (172) Zatorski, A.; Goldstein, B. M.; Colby, T. D.; Jones, J. P.; Pankiewicz, K. W. Potent Inhibitors of Human Inosine Monophosphate Dehydrogenase Type II. Fluorine-Substituted Analogues of Thiazole-4carboxamide Adenine Dinucleotide. J. Med. Chem. 1995, 38 (7), 1098− 1105. (173) Calleri, E.; Ceruti, S.; Cristalli, G.; Martini, C.; Temporini, C.; Parravicini, C.; Volpini, R.; Daniele, S.; Caccialanza, G.; Lecca, D.; et al. Frontal Affinity Chromatography-Mass Spectrometry Useful for Characterization of New Ligands for GPR17 Receptor. J. Med. Chem. 2010, 53 (9), 3489−3501. (174) Hyde, R. M.; Broom, A. D.; Buckheit, R. W. Antiviral Amphipathic Oligo- and Polyribonucleotides: Analogue Development and Biological Studies. J. Med. Chem. 2003, 46 (10), 1878−1885. (175) Ravi, R. G.; Kim, H. S.; Servos, J.; Zimmermann, H.; Lee, K.; Maddileti, S.; Boyer, J. L.; Harden, T. K.; Jacobson, K. A. Adenine Nucleotide Analogues Locked in a Northern Methanocarba Conformation: Enhanced Stability and Potency as P2Y(1) Receptor Agonists. J. Med. Chem. 2002, 45 (10), 2090−2100. (176) Kore, A. R.; Parmar, G. Convenient Synthesis of Nucleoside-5′diphosphates from the Corresponding Ribonucleoside-5′-phosphoroimidazole. Synth. Commun. 2006, 36 (22), 3393−3399. (177) Sun, Q.; Gong, S. S.; Sun, J.; Liu, S.; Xiao, Q.; Pu, S. Z. A P(V)-N Activation Strategy for the Synthesis of Nucleoside Polyphosphates. J. Org. Chem. 2013, 78 (17), 8417−8426. (178) Li, X. J.; Gong, S. S.; Sun, Q. A Novel Synthesis of Acyclovir Polyphosphates via Acyclovir Phosphoropiperidate Intermediate. Adv. Mater. Res. 2014, 908, 203−206. (179) Davisson, V. J.; Davis, D. R.; Dixit, V. M.; Poulter, C. D. Synthesis of Nucleotide 5′-Diphosphates from 5′-O-Tosyl Nucleosides. J. Org. Chem. 1987, 52 (9), 1794−1801. (180) Cremosnik, G. S.; Hofer, A.; Jessen, H. J. Iterative Synthesis of Nucleoside Oligophosphates with Phosphoramidites. Angew. Chem., Int. Ed. 2014, 53 (1), 286−289. (181) Bialy, L.; Waldmann, H. Total Synthesis and Biological Evaluation of the Protein Phosphatase 2A Inhibitor Cytostatin and Analogues. Chem. - Eur. J. 2004, 10 (11), 2759−2780. (182) Ahmadibeni, Y.; Parang, K. Solid-Supported Diphosphitylating and Triphosphitylating Reagents for Nucleoside Modification. In Current Protocols in Nucleic Acid Chemistry; John Wiley & Sons: New York, 2008; Vol. 33, Unit 13.8.

(183) Vaghefi, M. M. Phosphorus Nuclear Magnetic Resonance Chemical Shifts of Nucleotide Derivatives and Some Related OrganoPhosphorus Compounds. In Nucleoside Triphosphates Their Analogs; Vaghefi, M. M., Ed.; CRC Press: Boca Raton, FL, 2005; pp 373−375. (184) Weinschenk, L.; Meier, C. Chemical Syntheses of Nucleoside Triphosphates. In Chemical Synthesis of Nucleoside Analogues; John Wiley & Sons, Inc.: New York, 2013; Chapter 5, pp 209−227. (185) Caton-Williams, J.; Hoxhaj, R.; Fiaz, B.; Huang, Z. Use of a Novel 5′-Regioselective Phosphitylating Reagent for One-Pot Synthesis of Nucleoside 5′-Triphosphates from Unprotected Nucleosides. In Current Protocols in Nucleic Acid Chemistry; John Wiley & Sons: New York, 2013; Vol. 52, Unit 1.30. (186) Huang, Z. Novel Synthesis of Nucleoside 5′-Triphosphates and Their Derivatives. International Patent WO2012024625A2, 2012. (187) Ludwig, J. A New Route to Nucleoside 5′-Triphosphates. Acta Biochim. Biophys. Acad. Sci. Hung. 1981, 16 (3−4), 131−133. (188) Arabshahi, A.; Frey, P. A. A Simplified Procedure for Synthesizing Nucleoside 1-Thiotriphosphates: DATP(α)S, DGTP(α)S, UTP-α-S, and DTTP(α)S. Biochem. Biophys. Res. Commun. 1994, 204 (1), 150−155. (189) Eckstein, F. Nucleoside Phosphorothioates. Annu. Rev. Biochem. 1985, 54, 367−402. (190) Ludwig, J. A Simple One Flask Synthesis of Nucleoside 5′Triphosphates from Unprotected Nucleosides via Nucleoside 5′Cyclotriphosphates. In Biophosphates and Their Analogues: Synthesis, Metabolism and Activity; Elsevier: Amsterdam, 1987; Vol. 3, pp 201− 204. (191) Gillerman, I.; Fischer, B. An Improved One-Pot Synthesis of Nucleoside 5′-Triphosphate Analogues. Nucleosides, Nucleotides Nucleic Acids 2010, 29 (3), 245−256. (192) Aketani, S.; Tanaka, K.; Yamamoto, K.; Ishihama, A.; Cao, H. H.; Tengeiji, A.; Hiraoka, S.; Shiro, M.; Shionoya, M. Syntheses and Structure-Activity Relationships of Nonnatural β-C-Nucleoside 5′Triphosphates Bearing an Aromatic Nucleobase with Phenolic Hydroxy Groups: Inhibitory Activities against DNA Polymerases. J. Med. Chem. 2002, 45 (25), 5594−5603. (193) Alexandrova, L. A.; Ivanov, M. A.; Victorova, L. S.; Kukhanova, M. K. Furano- and Pyrrolo 2,3-D Pyrimidine Nucleosides and their 5′O-Triphosphates: Synthesis and Enzymatic Activity. Nucleosides, Nucleotides Nucleic Acids 2007, 26 (8−9), 1083−1086. (194) Balintova, J.; Pohl, R.; Horakova, P.; Vidlakova, P.; Havran, L.; Fojta, M.; Hocek, M. Anthraquinone as a Redox Label for DNA: Synthesis, Enzymatic Incorporation, and Electrochemistry of Anthraquinone-Modified Nucleosides, Nucleotides, and DNA. Chem. - Eur. J. 2011, 17 (50), 14063−14073. (195) Dadova, J.; Vidlakova, P.; Pohl, R.; Havran, L.; Fojta, M.; Hocek, M. Aqueous Heck Cross-Coupling Preparation of Acrylate-Modified Nucleotides and Nucleoside Triphosphates for Polymerase Synthesis of Acrylate-Labeled DNA. J. Org. Chem. 2013, 78 (19), 9627−9637. (196) Hocek, M. Synthesis of Base-Modified 2′-Deoxyribonucleoside Triphosphates and their Use in Enzymatic Synthesis of Modified DNA for Applications in Bioanalysis and Chemical Biology. J. Org. Chem. 2014, 79 (21), 9914−9921. (197) Ivanov, A. A.; Ko, H.; Cosyn, L.; Maddileti, S.; Besada, P.; Fricks, I.; Costanzi, S.; Harden, T. K.; Van Calenbergh, S.; Jacobson, K. A. Molecular Modeling of the Human P2Y(2) Receptor and Design of a Selective Agonist, 2′-Amino-2′-deoxy-2-thiouridine 5′-Triphosphate. J. Med. Chem. 2007, 50 (6), 1166−1176. (198) Kalachova, L.; Pohl, R.; Bednarova, L.; Fanfrlik, J.; Hocek, M. Synthesis of Nucleosides and dNTPs Bearing Oligopyridine Ligands Linked through an Octadiyne Tether, their Incorporation into DNA and Complexation with Transition Metal Cations. Org. Biomol. Chem. 2013, 11 (1), 78−89. (199) Knoblauch, B. H. A.; Muller, C. E.; Jarlebark, L.; Lawoko, G.; Kottke, T.; Wikstrom, M. A.; Heilbronn, E. 5-Substituted UTP Derivatives as P2Y(2) Receptor Agonists. Eur. J. Med. Chem. 1999, 34 (10), 809−824. (200) Maruoka, H.; Jayasekara, M. P. S.; Barrett, M. O.; Franklin, D. A.; de Castro, S.; Kim, N.; Costanzi, S.; Harden, T. K.; Jacobson, K. A. 7895


Chemical Reviews

Review

Pyrimidine Nucleotides with 4-Alkyloxyimino and Terminal Tetraphosphate δ-Ester Modifications as Selective Agonists of the P2Y(4) Receptor. J. Med. Chem. 2011, 54 (12), 4018−4033. (201) Riedl, J.; Horakova, P.; Sebest, P.; Pohl, R.; Havran, L.; Fojta, M.; Hocek, M. Tetrathiafulvalene-Labelled Nucleosides and Nucleoside Triphosphates: Synthesis, Electrochemistry and the Scope of their Polymerase Incorporation into DNA. Eur. J. Org. Chem. 2009, 2009 (21), 3519−3525. (202) Shi, J.; Zhou, L.; Zhang, H.; McBrayer, T. R.; Detorio, M. A.; Johns, M.; Bassit, L.; Powdrill, M. H.; Whitaker, T.; Coats, S. J.; et al. Synthesis and Antiviral Activity of 2′-Deoxy-2′-fluoro-2′-C-methyl-7deazapurine Nucleosides, Their Phosphoramidate Prodrugs and 5′Triphosphates. Bioorg. Med. Chem. Lett. 2011, 21 (23), 7094−7098. (203) Vasilyeva, S. V.; Budilkin, B. I.; Konevetz, D. A.; Silnikov, V. N. Synthesis of Novel Nucleoside 5′-Triphosphates and Phosphoramidites Containing Alkyne or Amino Groups for the Postsynthetic Functionalization of Nucleic Acids. Nucleosides, Nucleotides Nucleic Acids 2011, 30 (10), 753−767. (204) Wenge, U.; Ehrenschwender, T.; Wagenknecht, H.-A. Synthesis of 2′-O-Propargyl Nucleoside Triphosphates for Enzymatic Oligonucleotide Preparation and “Click” Modification of DNA with Nile Red as Fluorescent Probe. Bioconjugate Chem. 2013, 24 (3), 301−304. (205) Bhushan, R. G.; Vince, R. Synthesis of Conformationally Restricted 2′,3′-exo-Methylene Carbocyclic Nucleosides Built on a Bicyclo[3.1.0]hexane Template. Bioorg. Med. Chem. 2002, 10 (7), 2325−2333. (206) Kovacs, T.; Otvos, L. Simple Synthesis of 5-Vinyl- and 5Ethynyl-2′-Deoxyuridine-5′-Triphophates. Tetrahedron Lett. 1988, 29 (36), 4525−4528. (207) Kore, A. R.; Shanmugasundaram, M.; Senthilvelan, A.; Srinivasan, B. An Improved Protection-Free One-Pot Chemical Synthesis of 2′-Deoxynucleoside-5′-triphosphates. Nucleosides, Nucleotides Nucleic Acids 2012, 31 (5), 423−431. (208) Kore, A. R.; Shanmugasundaram, M.; Senthilvelan, A.; Srinivasan, B. Gram-Scale Chemical Synthesis of 2′-Deoxynucleoside5′-O-Triphosphates. In Current Protocols in Nucleic Acid Chemistry; John Wiley & Sons: New York, 2012; Vol. 49, Unit 13.10. (209) Kore, A. R.; Senthilvelan, A.; Srinivasan, B.; Shanmugasundaram, M. Facile Protection-Free One-Pot Synthesis of 7-Deaza-2′-deoxyguanosine-5′-triphosphateA Versatile Molecular Biology Probe. Can. J. Chem. 2013, 91 (8), 718−720. (210) Kore, A. R.; Srinivasan, B. Efficient Synthesis of 3Cyanovinylcarbazole-1′-β-Deoxyriboside-5′-Triphosphate: A Reversible Photo-Cross-Linking Probe. Tetrahedron Lett. 2012, 53 (31), 4012− 4014. (211) Kore, A. R.; Yang, B.; Srinivasan, B. Concise Synthesis of 5Methyl-, 5-Formyl, and 5-Carboxy Analogues of 2′-Deoxycytidine-5′Triphosphate. Tetrahedron Lett. 2013, 54 (39), 5325−5327. (212) Kore, A. R.; Yang, B.; Srinivasan, B. Short and Straightforward Synthesis of Triphosphates of Artificial Nucleobase Pairs Displaying Unconventional Pairing Scheme. Nucleosides, Nucleotides Nucleic Acids 2014, 33 (12), 767−773. (213) Shanmugasundaram, M.; Senthilvelan, A.; Xiao, Z.; Kore, A. R. An Efficient Protection-Free One-Pot Chemical Synthesis of Modified Nucleoside-5′-Triphosphates. Nucleosides, Nucleotides Nucleic Acids 2016, 1. (214) Moffatt, J. G. A General Synthesis of Nucleosides-5′ Triphosphates. Can. J. Chem. 1964, 42 (3), 599−604. (215) Li, Y.; Mao, S.; Hager, M. W.; Becnel, K. D.; Schinazi, R. F.; Liotta, D. C. Synthesis and Evalution of 2′-Substituted Cyclobutyl Nucleosides and Nucleotides as Potential Anti-HIV Agents. Bioorg. Med. Chem. Lett. 2007, 17 (12), 3398−3401. (216) Hoard, D. E.; Ott, D. G. Conversion of Mono- and Oligodeoxyribonucleotides to 5′-Triphosphates. J. Am. Chem. Soc. 1965, 87 (8), 1785−1788. (217) Bogachev, V. S. Synthesis of Deoxynucleoside 5′-Triphosphates Using Trifluoroacetic Anhydride as an Activating Reagent. Bioorg. Khim. 1996, 22 (9), 699−705 (in Russian).

(218) Wu, W. D.; Freel Meyers, C. L.; Borch, R. F. A Novel Method for the Preparation of Nucleoside Triphosphates from Activated Nucleoside Phosphoramidates. Org. Lett. 2004, 6 (13), 2257−2260. (219) Sun, Q.; Edathil, J. P.; Wu, R.; Smidansky, E. D.; Cameron, C. E.; Peterson, B. R. One-Pot Synthesis of Nucleoside 5′-Triphosphates from Nucleoside 5′-H-Phosphonates. Org. Lett. 2008, 10 (9), 1703−1706. (220) Sun, Q.; Liu, S.; Sun, J.; Gong, S.-S. An H-Phosphonate Strategy for the Synthesis of 2′,3′-Dideoxynucleoside Triphosphates and Homodinucleotides. Chin. Chem. Lett. 2014, 25 (3), 427−430. (221) Sun, Q.; Sun, J.; Gong, S.-S.; Wang, C.-J.; Pu, S.-Z.; Feng, F.-D. Efficient Synthesis of 5-Hydroxymethyl-, 5-Formyl-, and 5-Carboxyl-2′Deoxycytidine and their Triphosphates. RSC Adv. 2014, 4 (68), 36036− 36039. (222) Ludwig, J.; Eckstein, F. Rapid and Efficient Synthesis of Nucleoside 5′-O-(1-Thiotriphosphates), 5′-Triphosphates and 2′,3′Cyclophosphorothioates Using 2-Chloro-4H-1,3,2-benzodioxaphosphorin-4-one. J. Org. Chem. 1989, 54 (3), 631−635. (223) Hollenstein, M. Synthesis of Deoxynucleoside Triphosphates That Include Proline, Urea, or Sulfonamide Groups and Their Polymerase Incorporation into DNA. Chem. - Eur. J. 2012, 18 (42), 13320−13330. (224) Hollenstein, M.; Wojciechowski, F.; Leumann, C. J. Polymerase Incorporation of Pyrene-Nucleoside Triphosphates. Bioorg. Med. Chem. Lett. 2012, 22 (13), 4428−4430. (225) Xie, L.; Yang, X.; Pan, D.; Cao, Y.; Cao, M.; Lin, G.; Guan, Z.; Guo, Y.; Zhang, L.; Yang, Z. Synthesis and Anti-HIV Activity of a Series of 6-Modified 2′,3′-Dideoxyguanosine and 2′,3′-Didehydro-2′,3′dideoxyguanosine Analogs. Chin. J. Chem. 2013, 31 (9), 1207−1218. (226) Caton-Williams, J.; Lin, L.; Smith, M.; Huang, Z. Convenient Synthesis of Nucleoside 5′-Triphosphates for RNA Transcription. Chem. Commun. 2011, 47 (28), 8142−8144. (227) Caton-Williams, J.; Smith, M.; Carrasco, N.; Huang, Z. Protection-Free One-Pot Synthesis of 2′-Deoxynucleoside 5′-Triphosphates and DNA Polymerization. Org. Lett. 2011, 13 (16), 4156−4159. (228) Toti, K. S.; Derudas, M.; Pertusati, F.; Sinnaeve, D.; Van den Broeck, F.; Margamuljana, L.; Martins, J. C.; Herdewijn, P.; Balzarini, J.; McGuigan, C.; et al. Synthesis of an Apionucleoside Family and Discovery of a Prodrug with Anti-HIV Activity. J. Org. Chem. 2014, 79 (11), 5097−5112. (229) Li, P.; Dobrikov, M.; Liu, H. Y.; Shaw, B. R. Synthesis of Acyclothymidine Triphosphate and α-P-Boranotriphosphate and their Substrate Properties with Retroviral Reverse Transcriptase. Org. Lett. 2003, 5 (14), 2401−2403. (230) Mohamady, S.; Desoky, A.; Taylor, S. D. Sulfonyl Imidazolium Salts as Reagents for the Rapid and Efficient Synthesis of Nucleoside Polyphosphates and their Conjugates. Org. Lett. 2012, 14 (1), 402−405. (231) Makaev, F.; Styngach, E.; Shargarovskii, V.; Bets, L.; Vlad, L.; Barba, A. Imidazolium Salts with a Free Carboxy Group as New Catalysts of the Biginelli Reaction. Russ. J. Org. Chem. 2010, 46 (4), 610−611. (232) Zhan, T.; Guo, Y.; Xu, L.; Zhang, W.; Sun, W.; Hou, W. Electrochemistry and Electrocatalysis of Myoglobin Intercalated in Mg2Al-Cl Layered Double Hydroxide and Ionic Liquid Composite Material. Talanta 2012, 94, 189−194. (233) Eriksson, S. Enzymatic Synthesis of Nucleoside Triphosphates. In Nucleoside Triphosphates Their Analogs; Vaghefi, M. M., Ed.; CRC Press: Boca Raton, FL, 2005; pp 23−37. (234) Wu, W.; Bergstrom, D. E.; Davisson, V. J. Chemoenzymatic Preparation of Nucleoside Triphosphates. In Current Protocols in Nucleic Acid Chemistry; John Wiley & Sons: New York, 2004; Vol. 16, Unit 13.2. (235) Hennig, M.; Scott, L. G.; Sperling, E.; Bermel, W.; Williamson, J. R. Synthesis of 5-Fluoropyrimidine Nucleotides as Sensitive NMR Probes of RNA Structure. J. Am. Chem. Soc. 2007, 129 (48), 14911− 14921. (236) Kalia, D.; Merey, G.; Nakayama, S.; Zheng, Y.; Zhou, J.; Luo, Y.; Guo, M.; Roembke, B. T.; Sintim, H. O. Nucleotide, c-di-GMP, c-diAMP, cGMP, cAMP, (p)ppGpp Signaling in Bacteria and Implications in Pathogenesis. Chem. Soc. Rev. 2013, 42 (1), 305−341. 7896


Chemical Reviews

Review

(256) Ostash, B.; Yan, X.; Fedorenko, V.; Bechthold, A. Chemoenzymatic and Bioenzymatic Synthesis of Carbohydrate Containing Natural Products. Top. Curr. Chem. 2010, 297, 105−148. (257) Rupprath, C.; Schumacher, T.; Elling, L. Nucleotide Deoxysugars: Essential Tools for the Glycosylation Engineering of Novel Bioactive Compounds. Curr. Med. Chem. 2005, 12 (14), 1637− 1675. (258) Wagstaff, B. A.; Rejzek, M.; Pesnot, T.; Tedaldi, L. M.; Caputi, L.; O’Neill, E. C.; Benini, S.; Wagner, G. K.; Field, R. A. Enzymatic Synthesis of Nucleobase-Modified UDP-Sugars: Scope and Limitations. Carbohydr. Res. 2015, 404, 17−25. (259) White-Phillip, J.; Thibodeaux, C. J.; Liu, H.-w. Enzymatic Synthesis of TDP-Deoxysugars. Methods Enzymol. 2009, 459, 521−544. (260) Chen, K.-H.; Fang, W.-F.; Chen, Y.-T.; Fang, J.-M.; Yang, J.-T. Microflow Synthesis of Saccharide Nucleoside Diphosphate with CrossCoupling Reactions of Monophosphate Components. Chem. Eng. J. 2012, 198-199, 33−37. (261) Dabrowski-Tumanski, P.; Kowalska, J.; Jemielity, J. Efficient and Rapid Synthesis of Nucleoside Diphosphate Sugars from Nucleoside Phosphorimidazolides. Eur. J. Org. Chem. 2013, 2013 (11), 2147−2154. (262) Marlow, A. L.; Kiessling, L. L. Improved Chemical Synthesis of UDP-Galactofuranose. Org. Lett. 2001, 3 (16), 2517−2519. (263) Timmons, S. C.; Jakeman, D. L. Stereospecific Synthesis of Sugar-1-Phosphates and their Conversion to Sugar Nucleotides. Carbohydr. Res. 2008, 343 (5), 865−874. (264) Tsukamoto, H.; Kahne, D. N-Methylimidazolium ChlorideCatalyzed Pyrophosphate Formation: Application to the Synthesis of Lipid I and NDP-Sugar Donors. Bioorg. Med. Chem. Lett. 2011, 21 (17), 5050−5053. (265) Meyers, C. L. F.; Borch, R. F. Novel Method for the Preparation of Nucleoside Diphosphates. Org. Lett. 2001, 3 (23), 3765−3768. (266) Hofer, A.; Cremosnik, G. S.; Mueller, A. C.; Giambruno, R.; Trefzer, C.; Superti-Furga, G.; Bennett, K. L.; Jessen, H. J. A Modular Synthesis of Modified Phosphoanhydrides. Chem. - Eur. J. 2015, 21 (28), 10116−10122. (267) Wendicke, S.; Warnecke, S.; Meier, C. Efficient Synthesis of Nucleoside Diphosphate Glycopyranoses. Angew. Chem., Int. Ed. 2008, 47 (8), 1500−1502. (268) Wolf, S.; Berrio, R. M.; Meier, C. Synthesis of Nonnatural Nucleoside Diphosphate Sugars. Eur. J. Org. Chem. 2011, 2011 (31), 6304−6313. (269) Tanaka, H.; Yoshimura, Y.; Hindsgaul, O. A Simple Chemical Synthesis of Sugar Nucleoside Diphosphates in Water. In Current Protocols in Nucleic Acid Chemistry; John Wiley & Sons: New York, 2013; Vol. 54, Unit 13.12. (270) Tsybulskaya, I.; Kulak, T.; Baranovsky, A.; Golubeva, M.; Kuzmitsky, B.; Kalinichenko, E. Synthesis and In Vitro Cytostatic Activity of 1,2-and 1,3-Diacylglycerophosphates of Clofarabine. Bioorg. Med. Chem. 2013, 21 (17), 5414−5419.

(237) Smith, M.; Khorana, H. G.; Drummond, G. I. Cyclic Phosphates. IV. Ribonucleoside-3′,5′ Cyclic Phosphates. A General Method of Synthesis and some Properties. J. Am. Chem. Soc. 1961, 83 (3), 698− 706. (238) Genieser, H. G.; Butt, E.; Bottin, U.; Dostmann, W.; Jastorff, B. Synthesis of the 3′,5′-Cyclic Phosphates from Unprotected Nucleosides. Synthesis 1989, 1989 (1), 53−54. (239) Rozniewska, M.; Stawinski, J.; Kraszewski, A. Nucleoside 3′,5′Cyclic H-Phosphonates, New Useful Precursors for the Synthesis of Nucleoside 3′,5′-Cyclic Phosphates and their Analogues. Org. Lett. 2013, 15 (16), 4082−4085. (240) Rapaport, E.; Zamecnik, P. C. Presence of Diadenosine 5′,5‴P1,P4-Tetraphosphate (Ap4A) in Mammalian Cells in Levels Varying Widely with Proliferative Activity of Tissue: A Possible Positive “Pleiotypic Activator”. Proc. Natl. Acad. Sci. U. S. A. 1976, 73 (11), 3984−3988. (241) Huang, K. S.; Frey, P. A. Engineering Human Fhit, a Diadenosine Triphosphate Hydrolase, into an Efficient Dinucleoside Polyphosphate Synthase. J. Am. Chem. Soc. 2004, 126 (31), 9548−9549. (242) Sun, Q.; Gong, S.-S.; Liu, S.; Sun, J.; Liu, G.-D.; Ma, C. 4,5Dicyanoimidazole-Promoted Synthesis of Dinucleoside Polyphosphates and Their Analogs. Tetrahedron 2014, 70 (30), 4500−4506. (243) Douglass, J. G.; Patel, R. I.; Yerxa, B. R.; Shaver, S. R.; Watson, P. S.; Bednarski, K.; Plourde, R.; Redick, C. C.; Brubaker, K.; Jones, A. C.; et al. Lipophilic Modifications to Dinucleoside Polyphosphates and Nucleotides that Confer Antagonist Properties at the Platelet P2Y(12) Receptor. J. Med. Chem. 2008, 51 (4), 1007−1025. (244) Ko, H.; Carter, R. L.; Cosyn, L.; Petrelli, R.; de Castro, S.; Besada, P.; Zhou, Y.; Cappellacci, L.; Franchetti, P.; Grifantini, M.; et al. Synthesis and Potency of Novel Uracil Nucleotides and Derivatives as P2Y(2) and P2Y(6) Receptor Agonists. Bioorg. Med. Chem. 2008, 16 (12), 6319−6332. (245) Pendergast, W.; Yerxa, B. R.; Douglass, J. G.; Shaver, S. R.; Dougherty, R. W.; Redick, C. C.; Sims, I. F.; Rideout, J. L. Synthesis and P2Y Receptor Activity of a Series of Uridine Dinucleoside 5′Polyphosphates. Bioorg. Med. Chem. Lett. 2001, 11 (2), 157−160. (246) Yanachkov, I. B.; Dix, E. J.; Yanachkova, M. I.; Wright, G. E. P1,P2-Diimidazolyl Derivatives of Pyrophosphate and Bis-PhosphonatesSynthesis, Properties, and Use in Preparation of Dinucleoside Tetraphosphates and Analogs. Org. Biomol. Chem. 2011, 9 (3), 730− 738. (247) Mohamady, S.; Taylor, S. D. General Procedure for the Synthesis of Dinucleoside Polyphosphates. J. Org. Chem. 2011, 76 (15), 6344− 6349. (248) Han, Q. W.; Gaffney, B. L.; Jones, R. A. One-Flask Synthesis of Dinucleoside Tetra- and Pentaphosphates. Org. Lett. 2006, 8 (10), 2075−2077. (249) Ahmadibeni, Y.; Parang, K. Solid-Phase Synthesis of Symmetrical 5′,5′-Dinucleoside Mono-, Di-, Tri-, and Tetraphosphodiesters. Org. Lett. 2007, 9 (22), 4483−4486. (250) Mohamady, S.; Taylor, S. D. Synthesis of Nucleoside Tetraphosphates and Dinucleoside Pentaphosphates via Activation of Cyclic Trimetaphosphate. Org. Lett. 2013, 15 (11), 2612−2615. (251) Mohamady, S.; Taylor, S. D. Synthesis of Nucleoside Triphosphates from 2′-3′-Protected Nucleosides Using Trimetaphosphate. Org. Lett. 2016, 18 (3), 580−583. (252) Sun, Q.; Sun, J.; Gong, S.-S.; Wang, C.-J.; Wang, X.-C. One-Pot Synthesis of Symmetrical Dinucleoside Polyphosphates and Analogs via 4,5-Dicyanoimidazole-Promoted Tandem P−O Coupling Reactions. Tetrahedron Lett. 2014, 55 (42), 5785−5788. (253) Wang, Q.; Gong, S.; Sun, Q. Synthesis of Dinucleoside Triphosphates with Pyrimidine Bases. Adv. Mater. Res. 2014, 1023, 91− 94. (254) Friedrich, S.; Hahn, F. Opportunities for Enzyme Catalysis in Natural Product Chemistry. Tetrahedron 2015, 71 (10), 1473−1508. (255) Gantt, R. W.; Peltier-Pain, P.; Singh, S.; Zhou, M.; Thorson, J. S. Broadening the Scope of Glycosyltransferase-Catalyzed Sugar Nucleotide Synthesis. Proc. Natl. Acad. Sci. U. S. A. 2013, 110 (19), 7648−7653. 7897


Recent Trends in Nucleotide Synthesis - Chemical Reviews (ACS

Recommend Documents