Enzymatic Formation of an Injectable Hydrogel from a Glycopeptide

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Cite This: ACS Appl. Mater. Interfaces 2018, 10, 6180−6189

Enzymatic Formation of an Injectable Hydrogel from a Glycopeptide as a Biomimetic Scaffold for Vascularization Jingjing Qi,†,⊥ Yufei Yan,§,⊥ Baochang Cheng,† Lianfu Deng,§ Zengwu Shao,∥ Ziling Sun,*,‡ and Xinming Li*,† †

College of Chemistry, Chemical Engineering and Materials Science, ‡School of Biology and Basic Medical Science, Soochow University, Suzhou 215123, China § Shanghai Key Laboratory for Bone and Joint Diseases, Shanghai Institute of Orthopaedics and Traumatology, Shanghai Ruijin Hospital, Shanghai Jiaotong University, School of Medicine, Shanghai 200025, China ∥ Department of Orthopedic, Union Hospital, Tongji Medical School, Huazhong University of Science and Technology, Wuhan 430022, China S Supporting Information *

ABSTRACT: The construction of functional vascular networks in regenerative tissues is a crucial technology in tissue engineering to ensure the sufficient supply of nutrients. Although natural hydrogels are highly prevalent in fabricating three-dimensional scaffolds to induce neovascular growth, their widespread applicability was limited by the potential risk of immunogenicity or pathogen transmission. Therefore, developing hydrogels with good biocompatibility and cell affinity is highly desirable for fabricating alternative matrices for tissue regeneration applications. Herein, we report the generation of a new kind of hydrogel from supramolecular assembling of a synthetic glycopeptide to mimic the glycosylated microenvironment of extracellular matrix. In the presence of a tyrosine phosphate group, this molecule can undergo supramolecular self-assembling and gelation triggered by alkaline phosphatase under physiological conditions. Following supramolecular self-assembling, the glycopeptide gelator tended to form nanofilament structures displaying a high density of glucose moieties on their surface for endothelial cell adhesion and proliferation. On further incorporation with deferoxamine (DFO), the self-assembled hydrogel can serve as a reservoir for sustainably releasing DFO and inducing endothelial cell capillary morphogenesis in vitro. After subcutaneous injection in mice, the glycopeptide hydrogel encapsulating DFO can work as an effective matrix to trigger the generation of new blood capillaries in vivo. KEYWORDS: glycopeptide, hydrogel, self-assembly, DFO, tissue engineering

1. INTRODUCTION Tissue engineering provides a promising approach to replace or regenerate diseased or damaged tissues.1 The long-term survival of engineered tissues relies on the formation of sufficient microvascular network for nutrient exchange and oxygen delivery.2,3 In vivo, vascularization involves a cascade of events regulated by complex signals from both extracellular matrix (ECM) and growth factors, and the spatial and temporal arrangement of these signals in ECM orchestrated the in situ assembly of endothelial cells into capillary-like structures.4,5 Therefore, designing a scaffold that can mimic the structures and biological functions of native ECM for regulating the spatial arrangement of proangiogenic signals and supporting cell morphogenesis remains a major challenge in tissue engineering. Over the last decade, hydrogels from different origins (e.g., natural and synthetic polymers) have received considerable interest as desirable candidates for fabricating biomaterials to support cell proliferation and growth, owing to their high water content and structural similarity to the natural ECM.6,7 © 2018 American Chemical Society

Although hydrogels derived from natural ECM components (e.g., collagen, laminin, fibronectin, and glycosaminoglycans) exhibited good capabilities of adhering endothelial cells and supporting their transformation to microvessels in vitro,8 their widespread applicability was hindered by the difficulty of purification and the risk of immunogenicity or pathogen transmission. Therefore, development of a hydrogel to mimic the structural morphologies or chemical compositions of ECM is desirable for fabricating alternative matrices for tissue regeneration applications. Peptide-based hydrogels from supramolecular self-assembling have emerged as an important class of biomimetic materials for biomedical applications in recent years because of their inherent biocompatibility, biodegradability, and morphological similarity to fibrous proteins in ECM.9−15 Moreover, further decoration with certain bioactive cues (such as RGD, YIGSR, Received: December 5, 2017 Accepted: January 30, 2018 Published: January 30, 2018 6180

DOI: 10.1021/acsami.7b18535 ACS Appl. Mater. Interfaces 2018, 10, 6180−6189

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ACS Applied Materials & Interfaces

Scheme 1. Illustration of the Molecular Structure of a Glycopeptide Molecule and Its Self-Assembling Process for the Generation of a Supramolecular Hydrogel with Glucose Decoration, Which Could Be Exploited for Inducing Angiogenesis in Vivo

glycopeptide molecule can undergo quick supramolecular selfassembly in water under physiological conditions. Following supramolecular self-assembling, the glucose moiety on the surface of hydrogel can work as biomolecular cues for promoting cell attachment and growth. On further incorporation with deferoxamine (DFO), an organic drug with potential to provoke vascularization, the self-assembled hydrogel can work as an effective matrix to support the rapid formation of blood capillaries both in vitro and in vivo.

IKVAV, REDV, and PHSRN) derived from natural ECM can greatly improve the biological performance of peptide-based hydrogels in inducing cell adhesion, migration, and differentiation.16−20 On the contrary, besides the presence of fibrous proteins to work as structural supports for cells and tissues, the microenvironment of ECM also contains varied glycidic molecules, such as glycosaminoglycans and proteoglycans, which play a significant role in modulating cell adhesion, migration, and proliferation or controlling cellular behaviors via interactions between sugars and cell surface receptors.21,22 Therefore, to generate a hydrogel for mimicking the glycosylated microenvironment of ECM, we designed and synthesized a new kind of glycopeptide molecule, which consisted of a naphthyl group, a tetrapeptide segment (PhePhe-Asp-Tyr(H2PO3)) and a sugar moiety (D-glucosamine) on the side chain of Asp. Then, we used this molecule as building block to prepare a supramolecular hydrogel with glucose decoration on its surface (Scheme 1). The naphthyl moiety and Phe−Phe dipeptide segment acted as a rigid scaffold to drive supramolecular self-assembling of our designed glycopeptide gelator via extended aromatic−aromatic interactions; the Asp group was exploited for site-specific glucose modifications; and the tyrosine phosphate (e.g., Tyr(H2PO3)) worked as an excellent substrate of alkaline phosphatase for catalytic supramolecular gelation. Because of its good sensitivity toward alkaline phosphatase for dephosphorylation reaction, this

2. RESULTS AND DISCUSSION Scheme 2 shows the synthetic route and molecular structure of gelator precursor 1, which was prepared by following solidphase synthesis protocols with the application of FmocTyr(PO3)-OH, Fmoc-Asp(Glc)-OH, Fmoc-Phe-OH, and 2(naphthalen-6-yl) acetic acid. Fmoc-Asp(Glc)-OH was obtained through the coupling reaction between Fmoc-Asp-OtBu and D-Glucosamine (Figure S1).23,24 After high-performance liquid chromatography (HPLC) purification, we obtained gelator precursor 1 in yield around 63%. NMR and MS analyses confirmed the accuracy of the molecular structures of both Fmoc-Asp(Glc)-OH and gelator precursor 1 (Figures S2− S5). After obtaining gelator precursor 1, we tested its solubility in water and its sensitivity toward alkaline phosphatase for supramolecular gelation. Typically, we dissolved 1.2 mg of 1 in water, adjusted the pH of this solution to 7.4, and obtained a 6181


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Scheme 2. Synthetic Routes for the Preparation of Gelator Precursor 1 and Its Corresponding Enzymatic Transition to Gelator 2 by Alkaline Phosphatase

Figure 1. Optical images of (A) the solution of gelator precursor 1 (0.6 wt %, pH = 7.4) and (B) resulting Gp gel triggered by alkaline phosphatase (10 units/mL); (C) TEM and (D) SEM of the self-assembled structures from gelator 2 within Gp gel shown in (B).

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Figure 2. (A) Frequency dependence of the dynamic storage moduli (G′) and loss moduli (G″) of Gp gel shown in Figure 1B. (B) CD and (C) FTIR spectra of the solution of gelator precursor 1 (0.6 wt %, pH = 7.4) and the corresponding Gp gel shown in Figure 1B. (D) Time-dependent course of the digestion of gelator precursor 1 and a peptide derivative without glucose modification by proteinase K.

clear solution with a final concentration at 0.6 wt % (Figure 1A). After the addition of alkaline phosphatase, the solution of 1 transformed to a transparent hydrogel of glycopeptide (namely, Gp gel) in 20 min at room temperature (Figure 1B), which is due to the enzymatic dephosphorylation on 1 and the generation of gelator 2. The afforded gelator 2 then underwent supramolecular self-assembling for the formation of Gp gel, relying on extended aromatic−aromatic and hydrogen bonding interactions between gelator 2. The transmission electron microscopy (TEM) image shown in Figure 1C reveals the formation of one-dimensional nanofibrous structures from gelator 2 during the process of gelation, with several micrometers in length and 5 nm in width. These high-aspectratio nanofibers physically cross-linked with each other to form homogeneous networks as a gel matrix. Scanning electron micrograph (SEM) images showed the presence of threedimensional porous structures self-assembled from gelator 2 at microscales (Figure 1D). Dynamic rheological studies revealed that Gp gel selfassembled from 2 exhibited a dominantly elastic property of hydrogels (Figures 2A and S6), as exemplified by its much higher storage modulus (G′) than its loss modulus (G″) within the investigated oscillating frequency limits (0.1−20 Hz). These results indicated that gelator precursor 1 containing a glucose moiety could work as a good building block for the preparation of a stable supramolecular hydrogel of a glycopeptide via an enzymatic dephosphorylation reaction. Circular dichroism (CD) was used to examine the molecular conformations of gelator 2 during its supramolecular selfassembling. As shown in Figure 2B, the solution of gelator precursor 1 displayed a positive peak at 201 nm and a negative peak at 232 nm, indicating the absence of regular secondary

structures of gelator precursor 1 in a solution without the presence of alkaline phosphatase.25 However, after adding alkaline phosphatase to the solution of 1 for supramolecular gelation, we observed the generation of a negative peak near 217 nm and a positive peak around 192 nm in the CD spectrum of Gp gel, which was consistent with the characteristic of a β-sheet conformation.26 In addition, the additional negative peak at 204 nm and bisignated Cotton effects around 279 and 297 nm could be ascribed to the highly ordered arrangements of carbonyl groups and phenyl residues within its selfassembled structures.27 Fourier transform infrared (FTIR) analysis provided further information about the secondary structures of gelator 2 during the process of supramolecular assembling. For example, its FTIR spectrum showed a major amide I peak at 1629 cm−1 and a shoulder peak at around 1665 cm−1, indicating the formation of a typical β-sheet structure, together with a small amount of α-helixlike conformation (Figure 2C).28,29 The absorption at 1591 cm−1 was ascribed to the vibration of aromatic rings. The broad peak near 1458 cm−1 was assigned to the bending and stretching absorptions of N− H and C−N groups on gelator 2.30 One of the important features of peptide glycosylation in nature is to increase the biostability of peptide residues by resisting proteolytic digestion.31,32 From the biostability tests shown in Figure 2D, we found that gelator precursor 1 showed a good resistance to proteinase K digestion, as more than 61% of 1 remained intact after 24 h of incubation with proteinase K. In contrast, the peptide moiety without glucose modification (e.g., NapFFDYp) was hydrolyzed completely in 8 h by proteinase K, indicating the important role of a glucose moiety on gelator precursor 1 for protecting its peptide backbone from proteinase digestion. 6183


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Figure 3. (A) Fluorescence images of the live/dead assays of HUVECs cultured on the surface of Gp gel over the course of 5 days. (B) Cytoskeletal F-actin staining of HUVECs cultured on the surface of Gp gel by fluorescein (FITC)-phalloidin. (C) A high-magnification image of the boxed area shown in (B). (D) Cell densities of HUVECs determined by cell counting with a hemocytometer over the course of 5 day culture on Gp gel.

adhesion, proliferation, differentiation, and vascular formations.35,36 Although hydrogels derived from different naturally occurring polymers are highly prevalent in fabricating threedimensional scaffolds for neovascular growth, their applicability was limited by the risk of potential immunogenicity or pathogen transmission. Because of the high affinity of Gp gel to HUVECs for cell adhesion and proliferation, we further examined the potential of Gp gel to support microvasculature formations from HUVECs in the presence of a proangiogenic agent. Deferoxamine (DFO) is a clinical drug originally used for treating diseases of excess iron, but recent studies revealed that DFO can also work as a proangiogenic agent to promote the formation of new blood vessels by upregulating the expression of HIF-1α and vascular endothelial growth factor. 37,38 In comparison with naturally occurring or recombinant growth factors, DFO exhibited numerous advantages in inducing angiogenesis, such as quick angiogenic process, long-term stability, and efficiency.39,40 In addition, encapsulation of DFO in hydrogels can regulate the spatial and temporal delivery of DFO through sustained release.41 The proangiogenic activity of DFO released from Gp gel was checked by an in vitro tube formation assay. After HUVECs were seeded on the surface of Gp gel encapsulating DFO (1 mg/mL), the morphogenetic changes of cells were examined over time. As shown in Figure 4A, HUVECs attached well on the surface of Gp gel and tended to form cell clusters and capillary sprouts in 1 day. With the extension of incubation time to 2 and 3 days, most of the cells underwent microvascular morphogenesis and formed capillary tube networks. Quantitative analysis revealed the gradual increase of closed meshes, junctions, and total tubule length with time (Figure 4B−D). For example, the average numbers of meshes, junctions, and tubule length were about 6, 59, and 4922 μm at day 1, respectively, which gradually increased to 41, 142, and 8394 μm at day 3, respectively. In comparison, no obvious capillary tubes or short cord structures were observed in Gp gel without encapsulating DFO over the course of the 3 day culture,

The ECM microenvironment is composed of a variety of glycidic molecules ranging from glycosaminoglycans to proteoglycans, which play a significant role in modulating cell adhesion, migration, proliferation, and other cellular processes via the interactions between carbohydrate epitopes and cell surface receptors.33,34 Because of the high densities of glucose moieties on the scaffold of Gp gel, we decided to examine the effects of glucose decoration on cell adhesion and proliferation when using Gp gel as a cell culturing matrix. Cell viability assays confirmed the good biocompatibility of 1 toward human umbilical vein endothelial cells (HUVECs) (Figure S7). In vitro gel stability tests indicated that Gp gel could maintain good stability in cell culture media for more than 7 days (Figure S8). After planting HUVECs on the surface of Gp gel, we examined cell attachment and proliferation behaviors of HUVECs over the course of 5 day culture. On the basis of live−dead assays shown in Figure 3A, HUVECs were able to adhere and proliferate well on the surface of Gp gel, as exemplified by the polyhedral and spindlelike morphologies of cells after one day of incubation and the steady increase of cell densities over the course of 5 day culture. Cytoskeletal F-actin staining assays revealed the formation of well-defined and elongated stress actin filaments inside HUVECs (Figure 3B,C) due to the establishment of glucose-mediated interactions between HUVECs and the gel matrix. Quantitative analysis confirmed the gradual increase of cell numbers of HUVECs from day 1 (1.53 × 104 cm−2) to day 5 (4.57 × 104 cm−2) when they were cultured on the surface of Gp gel (Figure 3D). Therefore, the supramolecular hydrogel from gelator precursor 1 can work as an effective scaffold to promote endothelial cell adhesion and proliferation via glucose-mediated cell interactions. Establishing vascular systems in tissue constructs is a key challenge in tissue engineering for the survival and function of regenerative tissues.2 The angiogenic process in nature is achieved by complex interactions among endothelial cells, ECM, and growth factors.4,5 Particularly, physical interactions between endothelial cells and ECM play a critical role in cell 6184


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Figure 4. (A) Light microscopy images of the morphologies of HUVECs cultured on the surface of blank Gp gel and Gp gel loaded with DFO over the course of a 72 h culture. Scale bar = 50 μm. Quantitative analysis of the numbers of (B) meshes, (C) numbers of junctions, and (D) total length of vessels formed on the surfaces of Gp gel and Gp gel loaded with DFO over the course of a 72 h culture. The error bars indicate the standard deviation.

than its loss modulus (G″), indicating the dominantly elastic property of Gp gel at a low oscillatory strain. After the shear amplitude was increased to 100%, both G′ and G″ decreased significantly to 27.6 and 12.6 Pa, due to the disruption of physically cross-linked networks of Gp gel. However, when the amplitude of oscillatory strain was changed back to 1%, both G′ and G″ values recovered to 85% of their original values, suggesting the sheer-recovery property of GP gel. In addition, Gp gel loaded with DFO (1 mg/mL) also exhibited similar sheer-recovery properties to Gp gel, but its G′ value was 10 times higher than that of Gp gel without DFO (Figures 5C and S12), implying that the incorporation of DFO could enhance the mechanical strength of Gp gel via intermolecular interactions. These results indicated that Gp gel possessed tunable shear-shining and recovery properties (Figure S13) which could be exploited for injectable applications. After DFO-loading Gp gel was implanted into the dorsal side of mice through subcutaneous injection, its biodegradability, biocompatibility, and capabilities of inducing microvascularization in vivo were evaluated at days 3, 7, and 10. The DFOloaded hydrogel remained localized in the implantation site and was easily identifiable through 10 days, but its volume or size decreased gradually with time (Figure S14). H&E staining

indicating the bioactivity of DFO for inducing capillary morphogenesis of endothelial cells. During this process, Gp gel can not only provide a suitable growth support for effective cell attachment and colonization, but also serve as a reservoir for sustained DFO delivery to induce the formation of capillary tubes (Figure S11). Injectable hydrogels from different origins (e.g., natural and synthetic polymers) have received increasing interests in recent years for drug delivery, cell encapsulation, and wound dressings because of numerous advantages such as in situ formability, simple incorporation of drugs/cells, and minimally invasive delivery.42,43 The in situ gelation property of gelator precursor 1 under the catalysis of alkaline phosphatase encouraged us to explore the potentials of Gp gel for injectable applications in inducing microvascularization in vivo. First, we prepared a Gp gel (0.6 wt %) and loaded it in a 1 mL syringe. After extrusion through a needle with diameter 0.4 mm, the sample was collected in a vial and it can transform into a stable gel properly within 15 min (Figure 5A). Its sheer-recovery property was further tested by a dynamic shear-shining and recovery experiment. As shown in Figure 5B, when Gp gel (0.6 wt %) was subject to a dynamic oscillatory deformation at a low strain amplitude (1.0%), its storage modulus (G′) was much higher 6185


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Figure 5. (A) Optical images of (A) Gp gel (0.6 wt %), (B) process of extruding Gp gel through a needle with a diameter of 0.4 mm, (C) state of sample collected from the process shown in (B), and (D) Gp gel recovered from the sample shown in Figure 3C. Time-dependent repetitive cycles of the step−strain analysis of (E) blank Gp gel and (F) Gp gel encapsulating DFO (1 mg/mL).

Figure 6. (A), (B), and (C) H&E stained sections of the implanted Gp gel without loading DFO at days 3, 7, and 10, respectively; (D), (E), and (F) high-magnification images of the boxed areas in (A), (B), and (C), respectively. (G), (H), and (I) H&E stained sections of Gp gel loaded with DFO at days 3, 7, and 10, respectively; (J), (K), and (L) high-magnification images of the boxed areas in (G), (H), and (I), respectively. Scale bars = 100 μm. Arrows indicate blood vessels.

good biostability in vivo. Meanwhile, we also identified the presence of red blood cells within these blood vessels, indicating the biofunctionality of these newly generated blood vessels. Immunohistochemical staining with CD31 antibodies indicated that the blood vessels identified in the periphery of the implanted gel constructs originated from endothelial cells (Figure 7). Quantitative analyses confirmed the steady increase of blood vessels over the course of implantation of DFOloading Gp gel. For example, the average areas of blood vessels for DFO-loading group were around 1.98% per observed field at day 3 and increased to 3.3% at day 10 (Figure S16). In comparison, the groups implanted with the blank Gp gel showed much lower vessel densities (e.g., 0.50% at day 3 and 1.06% at day 10) over the course of 10 day implantation. These results suggested that Gp gel can work as an effective matrix for

confirmed that the areas of implanted Gp gel decreased gradually with time due to slow bioresorption and degradation of Gp gel and cell invasion and tissue growth (Figure S15). In addition, within the course of implantation, the implanted Gp gel did not induce significant inflammatory responses to the surrounding tissue, such as the absence of red or swollen features on mice, suggesting a negative inflammatory response. More importantly, after implantation of DFO-loading Gp gel, we observed an obvious increase in numbers of blood vessels in connective tissues surrounding DFO-loading Gp gel at day 3, compared to those in the group injected with blank Gp gel (Figure 6). In addition, the densities of blood capillaries in connective tissues were further increased within the course of 10 day implantation, which could be ascribed to the long bioavailability of DFO sustainably released from Gp gel and its 6186


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Figure 7. (A) and (B) Representative images of the sections of Gp gel without loading DFO at days 3 and 10, which were stained with CD31 antibodies (red). Nuclei were stained with DAPI (blue); (C) and (D) high-magnification images of the boxed areas in (A) and (B), respectively. (E) and (F) Representative images of the sections of implanted Gp gel loaded with DFO at days 3 and 10, which were stained with CD31 antibodies (red); (G) and (H) high-magnification images of the boxed areas in (E) and (F), individually. Scale bar = 50 μm. (400 MHz, DMSO-d6): 8.30−8.22 (s, 4H), 8.14−8.09 (d, 1H), 7.83− 7.79 (d, 1H), 7.76−7.72 (d, 1H), 7.72−7.65 (d, 1H), 7.58−7.52 (s, 1H), 7.47−7.39 (m, 3H), 7.24−7.02 (m, 14H), 7.02−6.96 (m, 1H), 4.58−4.38 (m, 4H), 3.58−3.15 (m, 14H), 3.04−2.84 (m, 4H), 2.80− 2.57 (m, 4H). MS: calcd M+ = 999.3, obsd (M + H)+ = 1000.3. 4.2. TEM and SEM Characterizations. First, 10 μL of Gp gel (0.6 wt %) was loaded on a carbon-coated Cu grid, followed by phosphotungstic acid (1.0%) staining. Then, TEM images of the nanostructures within Gp gel were recorded on a transmission electron microscope (Tecnai G220). The sample for SEM characterization was prepared by loading 5 μL of Gp gel (0.6 wt %) on a single-crystal silica plate and dried under vacuum, followed by coating with a thin layer of gold before SEM measurement. SEM images of the microstructures within Gp gel were obtained from a scanning electron microscope (Hitachi S-4800). 4.3. Rheological Tests. First, 200 μL of Gp gel (0.6 wt %) was loaded on a 20 mm parallel plate and subjected to rheological experiments on a Thermo Scientific HAAKE ReoStress 6000 rheometer. Dynamic strain sweep experiments were carried out from 0.1 to 10% strain with a fixed frequency at 6.282 rad/s at 25 °C. Dynamic frequency sweep tests were conducted from 20 to 0.1 rad/s with a fixed strain at 0.5% to ensure dynamic viscoelastic linearity. Shear-shining and recovery tests were first performed at low oscillatory strain amplitude (1.0%) with a fixed frequency at 6.28 rad/s, followed by the application of a high oscillatory strain at 100% for 30 s. Then, the amplitude of oscillatory strain was changed back to 1% for gel recovery. 4.4. Circular Dichroism and FTIR Characterizations. First, 20 μL of Gp gel (0.6 wt %) was placed evenly on a 1 mm quartz cuvette and analyzed on a Jasco J-810 spectrometer from 185 to 400 nm. The FTIR spectrum of Gp gel (0.6 wt %) was collected on a Perkin-Elmer spectrophotometer by loading 20 μL of the hydrogel into a KBr cuvette. The hydrogel for FTIR characterization was prepared by using deuterium oxide, deuterium chloride, and deuterium hydroxide as reagents. 4.5. In Vitro Biostability Assays. Initially, 1.0 mg of gelator precursor 1 was dissolved in 5 mL of a N-(2-hydroxyethyl)piperazineN′-ethanesulfonic acid buffer solution (pH = 7.4), followed by treatment with proteinase K (3.2 units/L). Then, the mixed solution was incubated at 37 °C for 24 h. At each specific time, 100 μL of solution was taken out from the sample and analyzed by HPLC. 4.6. Cytocompatibility Tests in Vitro. Cytocompatibility assays were carried out by following CCK-8 protocols. Human umbilical vein endothelial cells (HUVECs) were seeded in a 96-well microplate at a density of 4 × 104 cells/mL and incubated in a 5% CO2 humidified incubator at 37 °C. After 24 h, the medium was replenished with complete media supplementation with varied concentrations of gelator precursor 1 (10.0, 20.0, 50.0, 100.0, and 200.0 μM) and incubated for 24 and 72 h. Then, the fresh medium containing 10% CCK-8 solution

supporting microvasculature formations in vivo through efficient encapsulation and sustained deliveries of DFO.

3. CONCLUSIONS In summary, we reported the generation of a new selfassembled hydrogel from a glycopeptide for mimicking the highly glycosylated microenvironment of ECM. In the presence of tyrosine phosphate group, this molecule can undergo in situ supramolecular self-assembly and gelation triggered by alkaline phosphatase under physiological condition. Following supramolecular self-assembling, the glucose moieties on the surface of the hydrogel worked as biomolecular cues for improving cell attachment and growth of HUVECs via sugar−receptor interactions. On further incorporation with a proangiogenic factor (DFO), the self-assembled Gp gel served as a reservoir for sustainably releasing DFO and inducing endothelial cell capillary morphogenesis in vitro. After subcutaneous injection in mice, the self-assembled Gp gel encapsulating DFO can trigger the generation of new blood capillaries in vivo. The results of this study suggested that glucose decoration of a peptide gelator proved to be an effective means for the generation of a novel supramolecular hydrogelator and hydrogel with improved cell adhesion properties for regenerative medicine applications. 4. EXPERIMENTAL SECTION 4.1. Synthesis of Gelator Precursor 1. Gelator precursor 1 was synthesized by following standard solid-phase peptide synthesis protocols with the application of Fmoc-Tyr(H2PO3)-OH, FmocAsp(Glc)-OH, Fmoc-Phe-OH, and 2-(naphthalen-6-yl) acetic acid. Fmoc-Asp(Glc)-OH was prepared according to a previously reported method. First, 2-chlorotritylchloride resin (1.0 g) was suspended in dry dichloromethane (DCM) with N2 bubbling for 30 min and then was washed by dry dimethylformamide (DMF) three times. Afterward, the solution containing Fmoc-Tyr(H2PO3)-OH and N,N-diisopropylethylamine (DIEA) in DMF was added to a reactor. After reaction for 1 h, the resin was washed by dry DMF three times and quenched by a blocking solution (80:15:5 of DCM/methanol/DIEA) for 10 min. Then, the resin was treated with 20% piperidine in DMF for 0.5 h to remove Fmoc-protecting groups on amino acids. The designed peptide chain was elongated step by step using HBTU as a coupling reagent and following standard Fmoc solid phase peptide synthesis protocols. Finally, the synthetic glycopeptide was removed from the resin and purified with HPLC using H2O−CH3CN as eluents (from 80:20 to 0:100). The final yield of gelator precursor 1 is around 63%. 1H NMR 6187



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was added to each well and incubated for 2 h. The optical absorbance at 450 nm was read using a Thermo Scientific Varioskan Flash spectral scanning multimode reader. Cell viabilities were expressed as a percentage of the control (untreated) cells, and viabilities in the control group were designated as 100%. All experiments were performed in triplicate. 4.7. Cell Viability in Vitro. The viability of HUVEC planted on Gp gel was examined by live−dead assays according to manufacturer’s procedures. Approximately, 100 μL of a sterilized solution containing both gelator precursor 1 (0.6 wt %) and alkaline phosphatase (5 unit/ mL) was added in a 48-well plate. After gelation, the hydrogel sample was subjected to buffer exchange with 200 μL of Dulbecco’s Modified Eagle’s medium. After incubation for 24 h, the medium was replaced with fresh medium. Then, 200 μL of cell suspension (8 × 104 cells/ mL) was transferred into each well and placed in an incubator at 37 °C under 5% CO2 atmosphere. The medium was changed every other day. After incubation for 1, 3, and 5 days, the cells were stained with calcein-AM/propidium iodide and imaged by an Olympus IX71 fluorescence microscope. 4.8. Microfilament Staining. Morphologies and cytoskeleton structures of HUVEC cultured on the surface of Gp gel (0.6 wt %) were examined with FITC-phalloidin staining according to manufacturer’s instruction. After 1 day of culture, the cells on the surface of Gp gel were washed by phosphate-buffered saline (PBS, pH = 7.4) and fixed by 4% paraformaldehyde. After incubation at room temperature for 10 min, the fixed cells were washed three times with PBS buffer containing 0.1% triton X-100 (5 min each) and then stained with a mixed solution containing FITC-phalloidin (40 μg/mL) and Hoechst (20 μM) for 60 min. The stained cells were imaged by a confocal laser scanning microscopy with excitation filters at 488 nm (green, FITC) and 346 nm (blue, Hoechst). 4.9. In Vitro Angiogenesis Tests. First, 100 μL of Gp gel (0.6 wt %) containing DFO (1 mg/mL) was coated on a 48-well plate, and then 200 μL of cell suspension (8.0 × 103 cells) was seeded on the surface of Gp gel (0.6 wt %) in each well and incubated at 37 °C under 5% CO2 atmosphere. Cell status and morphologies were recorded by an OLYMPUS IX71 fluorescence microscope every 12 h. The numbers of meshes, junctions, and length of each tubule formed by HUVECs were quantified by using Image J software in 5 random fields. 4.10. Evaluation of DFO Release Behaviors in Vitro. Three groups of Gp gel (500 μL, 0.6 wt %) encapsulating DFO (0.5 mg) were immersed in 2 mL of PBS buffer (pH = 7.4) and incubated at 37 °C for DFO release. At each specific time (1, 2, 4, 8, 12, 24, 48, 72, and 96 h), 200 μL of PBS buffer was taken and treated with a certain amount of FeCl3. The amount of DFO released was determined by UV absorbance at 485 nm and a standard DFO calibration curve. 4.11. In Vivo Angiogenesis Tests. Mice were purchased from laboratory animal center of Soochow University, and in vivo tests were performed in full compliance with the Animal Care and Use regulations of Soochow University. Each experimental group consisted of 9 female BALB/c mice (8 weeks old). Mice were anesthetized with 4% chloral hydrate before in vivo tests. Then, 100 μL of Gp gel (0.6 wt %) encapsulating 100 μg of DFO was subcutaneously injected into the dorsal side of mice with a 1 mL syringe. After 3, 7, and 10 days, the mice were sacrificed and subcutaneous tissues containing implanted gels were excised, fixed in formaldehyde solution (4%), processed to paraffin blocks, and sectioned and stained with hematoxylin and eosin (H&E) or anti-CD31 antibody. Blood vessel areas in surrounding tissues were determined by using Image Pro Plus software from three different fields. 4.12. Statistical Analysis. All of the data were averaged from the measurements in more than three groups, and analyzed by using GraphPad Prism version (6.00) software. Values were displayed as mean ± standard deviation of the mean. The statistical significance of the difference was measured by using a Student’s t-test and one-way ANOVA (*P < 0.05, **P < 0.01, and ***P < 0.001). P < 0.05 was considered significant.

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ASSOCIATED CONTENT

S Supporting Information *

The Supporting Information is available free of charge on the ACS Publications website at DOI: 10.1021/acsami.7b18535. Materials and methods, synthesis and characterizations of gelator precursor 1, sustained release behavior of DFO from Gp gel (PDF)

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AUTHOR INFORMATION

Corresponding Authors

*E-mail: [email protected] (Z.S.). *E-mail: [email protected] (X.L.). ORCID

Xinming Li: 0000-0003-3251-1051 Author Contributions ⊥

J.Q. and Y.Y. authors contributed equally.

Notes

The authors declare no competing financial interest.

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ACKNOWLEDGMENTS This work was supported financially by the National Key R&D Program of China (Ministry of Science and Technology of China, 2016YFC1100100); the National Natural Science Foundation of China (51673142) to X.L.; the Natural Science Foundation of Jiangsu Province (BK20151218) to X.L.; and the Priority Academic Program Development of Jiangsu Higher Education Institutions (PAPD).

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REFERENCES

(1) Vacanti, J. P.; Langer, R. Tissue Engineering: the Design and Fabrication of Living Replacement Devices for Surgical Reconstruction and Transplantation. Lancet 1999, 354, SI32−SI34. (2) Jain, R. K.; Au, P.; Tam, J.; Duda, D. G.; Fukumura, D. Engineering Vascularized Tissue. Nat. Biotechnol. 2005, 23, 821−823. (3) Levenberg, S.; Rouwkema, J.; Macdonald, M.; Garfein, E. S.; Kohane, D. S.; Darland, D. C.; Marini, R.; van Blitterswijk, C. A.; Mulligan, R. C.; D’Amore, P. A.; Langer, R. Engineering Vascularized Skeletal Muscle Tissue. Nat. Biotechnol. 2005, 23, 879−884. (4) Phelps, E. A.; Garcia, A. J. Engineering More Than a Cell: Vascularization Strategies in Tissue Engineering. Curr. Opin. Biotechnol. 2010, 21, 704−709. (5) Rouwkema, J.; Khademhosseini, A. Vascularization and Angiogenesis in Tissue Engineering: Beyond Creating Static Networks. Trends Biotechnol. 2016, 34, 733−745. (6) Peppas, N. A.; Hilt, J. Z.; Khademhosseini, A.; Langer, R. Hydrogels in Biology and Medicine: From Molecular Principles to Bionanotechnology. Adv. Mater. 2006, 18, 1345−1360. (7) Seliktar, D. Designing Cell-Compatible Hydrogels for Biomedical Applications. Science 2012, 336, 1124−1128. (8) Moon, J. J.; Saik, J. E.; Poche, R. A.; Leslie-Barbick, J. E.; Lee, S.H.; Smith, A. A.; Dickinson, M. E.; West, J. L. Biomimetic Hydrogels with Pro-Angiogenic Properties. Biomaterials 2010, 31, 3840−3847. (9) Schneider, J. P.; Pochan, D. J.; Ozbas, B.; Rajagopal, K.; Pakstis, L.; Kretsinger, J. Responsive Hydrogels from the Intramolecular Folding and Self-Assembly of a Designed Peptide. J. Am. Chem. Soc. 2002, 124, 15030−15037. (10) Kiyonaka, S.; Sada, K.; Yoshimura, I.; Shinkai, S.; Kato, N.; Hamachi, I. Semi-Wet Peptide/Protein Array Using Supramolecular Hydrogel. Nat. Mater. 2004, 3, 58−64. (11) Zhou, J.; Li, J.; Du, X.; Xu, B. Supramolecular Biofunctional Materials. Biomaterials 2017, 129, 1−27. (12) Cui, H.; Webber, M. J.; Stupp, S. I. Self-Assembly of Peptide Amphiphiles: From Molecules to Nanostructures to Biomaterials. Biopolymers 2010, 94, 1−18. 6188


Research Article

ACS Applied Materials & Interfaces (13) Hauser, C. A. E.; Zhang, S. Designer Self-Assembling Peptide Nanofiber Biological Materials. Chem. Soc. Rev. 2010, 39, 2780−2790. (14) Wang, Y.-L.; Lin, S.-P.; Nelli, S. R.; Zhan, F.-K.; Cheng, H.; Lai, T.-S.; Yeh, M.-Y.; Lin, H.-C.; Hung, S.-C. Self-Assembled PeptideBased Hydrogels as Scaffolds for Proliferation and Multi-Differentiation of Mesenchymal Stem Cells. Macromol. Biosci. 2017, 17, No. 1600192. (15) Hsu, S.-M.; Wu, F.-Y.; Cheng, H.; Huang, Y.-T.; Hsieh, Y.-R.; Tseng, D. T.-H.; Yeh, M.-Y.; Hung, S.-C.; Lin, H.-C. Functional Supramolecular Polymers: A Fluorescent Microfibrous Network in a Supramolecular Hydrogel for High-Contrast Live Cell-Material Imaging in 3D Environments. Adv. Healthcare Mater. 2016, 5, 2406−2412. (16) Du, X.; Zhou, J.; Guvench, O.; Sangiorgi, F. O.; Li, X.; Zhou, N.; Xu, B. Supramolecular Assemblies of a Conjugate of Nucleobase, Amino Acids, and Saccharide Act as Agonists for Proliferation of Embryonic Stem Cells and Development of Zygotes. Bioconjugate Chem. 2014, 25, 1031−1035. (17) Sur, S.; Pashuck, E. T.; Guler, M. O.; Ito, M.; Stupp, S. I.; Launey, T. A Hybrid Nanofiber Matrix to Control the Survival and Maturation of Brain Neurons. Biomaterials 2012, 33, 545−555. (18) Moore, A. N.; Hartgerink, J. D. Self-Assembling Multidomain Peptide Nanofibers for Delivery of Bioactive Molecules and Tissue Regeneration. Acc. Chem. Res. 2017, 50, 714−722. (19) Jung, J. P.; Jones, J. L.; Cronier, S. A.; Collier, J. H. Modulating the Mechanical Properties of Self-Assembled Peptide Hydrogels via Native Chemical Ligation. Biomaterials 2008, 29, 2143−2151. (20) Zhou, M.; Smith, A. M.; Das, A. K.; Hodson, N. W.; Collins, R. F.; Ulijn, R. V.; Gough, J. E. Self-Assembled Peptide-Based Hydrogels as Scaffolds for Anchorage-Dependent Cells. Biomaterials 2009, 30, 2523−2530. (21) Sasisekharan, R.; Raman, R.; Prabhakar, V. Glycomics Approach to Structure-Function Relationships of Glycosaminoglycans. Annu. Rev. Biomed. Eng. 2006, 8, 181−231. (22) Kim, S.-H.; Turnbull, J.; Guimond, S. Extracellular matrix and cell signalling: the dynamic cooperation of integrin, proteoglycan and growth factor receptor. J. Endocrinol. 2011, 209, 139−151. (23) Liu, J.; Xu, F.; Sun, Z.; Pan, Y.; Tian, J.; Lin, H.-C.; Li, X. A Supramolecular Gel Based on a Glycosylated Amino Acid Derivative with the Properties of Gel to Crystal Transition. Soft Matter 2016, 12, 141−148. (24) Liu, J.; Sun, Z.; Yuan, Y.; Tian, X.; Liu, X.; Duan, G.; Yang, Y.; Yuan, L.; Lin, H.-C.; Li, X. Peptide Glycosylation Generates Supramolecular Assemblies from Glycopeptides as Biomimetic Scaffolds for Cell Adhesion and Proliferation. ACS Appl. Mater. Interfaces 2016, 8, 6917−6924. (25) Whitmore, L.; Wallace, B. A. Protein Secondary Structure Analyses from Circular Dichroism Spectroscopy: Methods and Reference Databases. Biopolymers 2008, 89, 392−400. (26) Chen, Y. H.; Yang, J. T.; Martinez, H. M. Determination of Secondary Structures of Proteins by Circular-Dichroism and Optical Rotary Dispersion. Biochemistry 1972, 11, 4120−4131. (27) Zhang, Y.; Yang, Z. M.; Yuan, F.; Gu, H. W.; Gao, P.; Xu, B. Molecular Recognition Remolds the Self-Assembly of Hydrogelators and Increases the Elasticity of the Hydrogel by 10(6)-Fold. J. Am. Chem. Soc. 2004, 126, 15028−15029. (28) Hughes, M.; Debnath, S.; Knapp, C. W.; Ulijn, R. V. Antimicrobial Properties of Enzymatically Triggered Self-Assembling Aromatic Peptide Amphiphiles. Biomater. Sci. 2013, 1, 1138−1142. (29) Xu, X.-D.; Liang, L.; Cheng, H.; Wang, X.-H.; Jiang, F.-G.; Zhuo, R.-X.; Zhang, X.-Z. Construction of Therapeutic Glycopeptide Hydrogel as a New Substitute for Antiproliferative Drugs to Inhibit Postoperative Scarring Formation. J. Mater. Chem. 2012, 22, 18164− 18171. (30) Hamley, I. W.; Brown, G. D.; Castelletto, V.; Cheng, G.; Venanzi, M.; Caruso, M.; Placidi, E.; Aleman, C.; Revilla-Lopez, G.; Zanuy, D. Self-Assembly of a Designed Amyloid Peptide Containing the Functional Thienylalanine Unit. J. Phys. Chem. B 2010, 114, 10674−10683.

(31) Solá, R. J.; Griebenow, K. Effects of Glycosylation on the Stability of Protein Pharmaceuticals. J. Pharm. Sci. 2009, 98, 1223− 1245. (32) Culyba, E. K.; Price, J. L.; Hanson, S. R.; Dhar, A.; Wong, C.-H.; Gruebele, M.; Powers, E. T.; Kelly, J. W. Protein Native-State Stabilization by Placing Aromatic Side Chains in N-Glycosylated Reverse Turns. Science 2011, 331, 571−575. (33) Taylor, M. E.; Drickarner, K. Paradigms for Glycan-Binding Receptors in Cell Adhesion. Curr. Opin. Cell Biol. 2007, 19, 572−577. (34) Hughes, R. C. Complex Carbohydrates of Mammalian-Cell Surfaces and Their Biological Roles. Essays Biochem. 1975, 11, 1−36. (35) Strömblad, S.; Cheresh, D. A. Integrins, Angiogenesis and Vascular Cell Survival. Chem. Biol. 1996, 3, 881−885. (36) Strömblad, S.; Cheresh, D. A. Cell Adhesion and Angiogenesis. Trends Cell Biol. 1996, 6, 462−468. (37) Jiang, X.; Malkovskiy, A. V.; Tian, W.; Sung, Y. K.; Sun, W.; Hsu, J. L.; Manickam, S.; Wagh, D.; Joubert, L.-M.; Semenza, G. L.; Rajadas, J.; Nicolls, M. R. Promotion of Airway Anastomotic Microvascular Regeneration and Alleviation of Airway Ischemia by Deferoxamine Nanoparticles. Biomaterials 2014, 35, 803−813. (38) Ikeda, Y.; Tajima, S.; Yoshida, S.; Yamano, N.; Kihira, Y.; Ishizawa, K.; Aihara, K.-I.; Tomita, S.; Tsuchiya, K.; Tamaki, T. Deferoxamine Promotes Angiogenesis via the Activation of Vascular Endothelial Cell Function. Atherosclerosis 2011, 215, 339−347. (39) Chen, H.; Jia, P.; Kang, H.; Zhang, H.; Liu, Y.; Yang, P.; Yan, Y.; Zuo, G.; Guo, L.; Jiang, M.; Qi, J.; Liu, Y.; Cui, W.; Santos, H. A.; Deng, L. Upregulating Hif-1 by Hydrogel Nanofibrous Scaffolds for Rapidly Recruiting Angiogenesis Relative Cells in Diabetic Wound. Adv. Healthcare Mater. 2016, 5, 907−918. (40) Wahl, E. A.; Schenck, T. L.; Machens, H.-G.; Balmayor, E. R. VEGF Released by Deferoxamine Preconditioned Mesenchymal Stem Cells Seeded on Collagen-GAG Substrates Enhances Neovascularization. Sci. Rep. 2016, 6, No. 36879. (41) Chen, H.; Guo, L.; Wicks, J.; Ling, C.; Zhao, X.; Yan, Y.; Qi, J.; Cui, W.; Deng, L. Quickly Promoting Angiogenesis by Using a DFOLoaded Photo-Crosslinked Gelatin Hydrogel for Diabetic Skin Regeneration. J. Mater. Chem. B 2016, 4, 3770−3781. (42) Yu, L.; Ding, J. Injectable Hydrogels as Unique Biomedical Materials. Chem. Soc. Rev. 2008, 37, 1473−1481. (43) Bidarra, S. J.; Barrias, C. C.; Granja, P. L. Injectable Alginate Hydrogels for Cell Delivery in Tissue Engineering. Acta Biomater. 2014, 10, 1646−1662.

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Enzymatic Formation of an Injectable Hydrogel from a Glycopeptide

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