Engineering Riboswitches in Vivo Using Dual Genetic Selection and

Aug 17, 2018 - To the best of our knowledge, this is the first report of in vivo directed evolution of an aptamer domain to generate a functional ribo...
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Engineering riboswitches in vivo using dual genetic selection and fluorescence-activated cell sorting Katharine Page, Jeremy Shaffer, Samuel Lin, Mark Zhang, and Jane May Liu ACS Synth. Biol., Just Accepted Manuscript • DOI: 10.1021/acssynbio.8b00099 • Publication Date (Web): 17 Aug 2018 Downloaded from http://pubs.acs.org on August 18, 2018

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Engineering riboswitches in vivo

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Engineering riboswitches in vivo using dual genetic selection and fluorescence-

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activated cell sorting

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Katharine Page, Jeremy Shaffer, Samuel Lin, Mark Zhang and Jane M. Liu*

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Department of Chemistry

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Pomona College

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645 N. College Avenue

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Claremont, CA 91711

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*[email protected]

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(909) 607-8832

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Key words:

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riboswitches, E. coli, genetic selection, cell sorting

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Abstract

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Riboswitches, non-coding RNAs that bind a small molecule effector to control gene

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expression at the level of transcription or translation, are uniquely suited to meet

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challenges in synthetic biology. To expand the limited set of existing riboswitches, we

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developed a riboswitch discovery platform that couples dual genetic selection and

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fluorescence-activated cell sorting to identify novel riboswitches from a 108 random-

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sequence library in which the aptamer domain of the ThiM#2 riboswitch was replaced

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with an N40 sequence. In a proof-of-principle validation, we identified novel riboswitches

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for the small molecule theophylline. Our best riboswitch (Hit 3-5) displays 2.3-fold

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activation of downstream gene expression in the presence of theophylline. Random

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mutagenesis of Hit 3-5, coupled with selections and screens, afforded improved

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riboswitches displaying nearly 3-fold activation. To the best of our knowledge, this is the

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first report of in vivo directed evolution of an aptamer domain to generate a functional

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riboswitch.

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Riboswitches comprise a class of regulatory RNA elements capable of binding small

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molecule ligands. These naturally occurring riboregulators, found across a range of

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prokaryotic organisms, act at the transcriptional or translational level to affect gene

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expression in cis and are mediated not by protein factors, but rather by small molecule

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binding.1,2 There are two functional components that contribute to riboswitch activity.

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The first is an aptamer domain (the sensor) that binds the ligand of interest. The second

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is an expression platform (the actuator), which couples the aptamer’s binding state to

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the enhancement or repression of downstream gene expression. A riboswitch that

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inhibits expression in the presence of its cognate ligand is termed an OFF switch, while

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a riboswitch that augments expression is termed an ON switch. Given that these

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regulators alter gene expression in a ligand-dependent manner and that the sensor and

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actuator domains are considered modular, riboswitches are particularly well suited for

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synthetic biology projects involving RNA devices.3–8 A major limitation in developing

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these RNA tools, however, is the narrow collection of existing riboswitches. Expanding

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the catalog of riboswitches to accommodate a wide variety of ligands would address a

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significant bottleneck in the field.

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Powerful in vitro evolution and selection methods (e.g. SELEX) can rapidly identify high-

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affinity aptamers for small molecules, which can be incorporated as the sensor domain

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of a synthetic riboswitch.9–13 However, cellular screening of these aptamers after

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selection is generally required in order to couple the sensors to appropriate actuators to

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create a functional riboswitch. While this approach to engineering riboswitches from

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synthetic aptamers has been demonstrated, it does not always work reliably, and it

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often requires implementing additional rational design strategies.14–18 The difficulty of

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incorporating an aptamer from SELEX into a genetic switch is not entirely surprising as

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an aptamer selected in vitro does not necessarily bind the ligand in the same manner in

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a cellular environment where other interactions also may occur.19 Moreover, natural

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aptamers that have evolved in a cellular environment typically occupy a set of privileged

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scaffolds that allow for biological activity, whereas high-affinity aptamers developed via

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SELEX often are structurally less complex.20 Indeed, an effective riboswitch must do

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more than just bind its cognate ligand with high affinity; induced changes to secondary

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and tertiary structure must be relayed from the sensor through the actuator, an activity

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not addressed during in vitro selection.

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The rational reprogramming of naturally occurring riboswitches has been one approach

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to address the disparity between in vitro selected aptamers and functional cellular

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riboswitches.14,21,22 Similarly, naturally occurring riboswitches have been tuned through

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dual genetic selection, for example converting the Escherichia coli TPP riboswitch,

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which binds thiamine pyrophosphate, from an OFF switch to an ON switch.23–25 In these

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cases, however, the synthetic riboswitch obtained ultimately recognizes the same ligand

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as the original riboswitch, or a structurally related one.

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In the present study, we present a procedure for the development of riboswitches that

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allows for the creation of riboswitches that recognize, theoretically, any ligand of

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interest. Importantly, the procedure takes place entirely inside a cellular environment,

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thereby bypassing some of the concerns related to the “SELEX-first” approach.

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Specifically, we constructed a riboswitch plasmid library in which the aptamer domain of

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the ThiM#2 riboswitch23 (an ON switch that responds to TPP) was replaced by a

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randomized region of 40 nucleotides. The plasmids were introduced into E. coli and the

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resulting library was subjected to multiple rounds of dual genetic selection and

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fluorescence-activated cell sorting (FACS) screening to generate riboswitches

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responsive to theophylline. We were able to generate theophylline-responsive

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riboswitches after only three rounds of selections and screens. An additional round of

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mutagenesis, selections and screens of one of the switches further increased its

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activity. Our de novo development of novel theophylline riboswitches provides a general

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platform from which many more synthetic riboswitches may be discovered, addressing a

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major obstacle to broadening the scope of riboswitch-based technology.

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Results and Discussion

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To make a library from which to select and screen for novel ON riboswitches, we started

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with a ThiM#2 riboswitch construct,23 which contains an aptamer region that recognizes

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TPP, an expression platform that allows the riboswitch to function as an ON switch, and

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a tetA-gfp+ fusion that acts as a selectable marker and reporter.24 As our aim was to

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identify novel riboswitches for theophylline, we replaced the aptamer region upstream of

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the ThiM#2 expression platform by cloning in a random 40-nucleotide sequence,

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generating a theoretical diversity of 1024 sequences (Figure 1A; Table S1). The

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expression platform of ThiM#2 between the aptamer and ribosome binding site (RBS)

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was retained. We introduced our plasmid library into E. coli, generating a 108 library of

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transformants.

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Our riboswitch discovery platform consists of genetic selections using the dual

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selectable marker, tetA, and high-throughput fluorescence screens using GFP+.13,23–27

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Bacteria expressing tetA are resistant to tetracycline and susceptible to heavy metal

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toxicity. Thus, in order to identify members of the library that activate gene expression in

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a theophylline-dependent manner, we performed “positive” selections with tetracycline

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and theophylline and “negative” selections with Ni2+ and without theophylline. In addition

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to selections, we performed screens using FACS in which we isolated the most and

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least fluorescent library members following positive and negative selections,

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respectively (Figure S1). FACS has been shown to identify improved riboswitch variants

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and, in addition, provides an opportunity to identify the library members exhibiting the

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most extreme levels of ON and OFF gene expression in a manner not afforded to

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selections.28,29 Thus, we proposed that subjecting our riboswitch library to high-

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throughput screens in addition to genetic selections would increase the robustness of

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our engineering platform.

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We sought to identify theophylline riboswitches from our library by performing three

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complete rounds of selection, incorporating FACS screening (ON-sort) after positive

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selection in rounds two and three (Figure S2). Cultures were supplemented with 1 mM

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theophylline when appropriate. As we were selecting for function from a random-

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sequence library, we incrementally increased the stringency of positive selection by

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starting with a low concentration of tetracycline in round one and increasing the

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tetracycline concentration in rounds two and three, using 30, 40, and 50 µg/mL,

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respectively. Ni2+ concentrations were kept constant at 0.3 mM in each negative

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selection. These chosen concentrations were based on prior selections performed on a

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TPP switch.24 Following the third round of selections and screens, dilutions of the

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surviving library members were plated and eight isolates were randomly selected for

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sequencing and fluorescence assays (Table S2). Of those interrogated, Hit 3-5

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displayed the greatest fold activation (Figure 1, Figure S3). We then repeated the

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selections and FACS screens on our N40 library with one modification. After negative

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selections of rounds two and three, we incorporated an “OFF-sort” through FACS

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screening as a way to identify members with low levels of fluorescence in its “OFF”

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state (Figure S2). After three rounds, eight randomly-selected post-selection library

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members were sequenced and assayed for fluorescence. Hit 3-8 was enriched to half of

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the sequences analyzed and was the only isolate that displayed riboswitch activity

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(Figure 1). Hit 3-5 and Hit 3-8 display a 2.3 and 2.1-fold activation of gene expression,

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respectively (Figures 1B, 1C and S4). Interestingly, Hit 3-8 displays much lower levels

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of gene expression in both its “ON” and “OFF” states compared to Hit 3-5 (Figure 1B).

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We postulate that incorporation of an OFF-sort following negative selection may allow

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the isolation of rare switches that have a low basal level of gene expression. Moreover,

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our platform uncovered theophylline riboswitches with unique aptamer sequences, and

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both of these aptamers are different from the aptamers identified from in vitro selections

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using SELEX (Figure 1A and S5).30

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One of these in vitro selected aptamers, mTCT8-4, has been used to create a

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theophylline-responsive riboswitch.12,31 We replaced the 5’ untranslated region of Hit 3-

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5, up to the ribosome binding site, with a sequence coding for the mTCT8-4-based

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riboswitch and compared the two constructs (Figure 1A). The mTCT8-4-based

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riboswitch displayed an impressive 15.8-fold activation upon ligand addition, compared

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to the 2.3-fold activation achieved by Hit 3-5 (Figure 1B). At the same time, the mTCT8-

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4 aptamer was selected after eight rounds of SELEX, compared to the three rounds of

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dual genetic selection used here. Additional high-throughput screens were also used to

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identify an ideal actuator sequence linking the aptamer to the RBS, a process that is not

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always successful in generating a riboswitch given the difference between the cellular

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milieu in which the aptamer is expected to function and the in vitro conditions from

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which the aptamers was selected.14–18,31 Overall, our results suggest two things: one,

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aptamers engineered in vivo and in vitro may converge to different solutions; and, two,

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certain ligand-binding RNAs capable of eliciting modest biological activity can be

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identified within a cellular environment without the use of in vitro engineering methods.

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We also attempted to obtain riboswitches responsive to theophylline from our starting

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108 library using a “selection-only” or a “sort-only” approach. None of the randomly

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selected eight clones that survived three rounds of selection in the selection-only

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method demonstrated any fold-activation in response to theophylline (data not shown).

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Intriguingly, the sort-only protocol resulted in enrichment of ThiM#2 clones to five of the

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seven sequenced isolates. As our N40 library was constructed using a ThiM#2 construct

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as a template, it is not surprising that there may have been residual copies of the parent

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plasmid that were not detected when we sequenced only 8 of the initial library members

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(Table S1). It is unclear, however, why ThiM#2 was able to become enriched through

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FACS screening as theophylline does not appear to induce the TPP riboswitch to

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activate gene expression (Figure 1C). Regardless, our results indicate that the

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combination of genetic selection with FACS screening is an efficacious method for

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identifying new riboswitches from random-sequence libraries.

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Following the identification of Hits 3-5 and 3-8, we tested whether riboswitch activity

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was retained in different genetic constructs. First, we cloned the lacZ gene in place of

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the tetA-gfp+ fusion. Hits 3-5 and 3-8 demonstrate a 1.9 and 1.7-fold activation,

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respectively, in this pLac-rbsw-lacZ context (Figure 2A). We then tested riboswitch

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activity in a construct with an arabinose-inducible promoter, replacing the pLac promoter

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that was used in our original library construction and in pLac-rbsw-lacZ. In beta-

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galactosidase assays, Hits 3-5 and 3-8 both display a 1.7-fold activation in this pBAD-

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rbsw-lacZ construct (Figure 2B). These results demonstrate that our engineered

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riboswitches function in diverse contexts and that their switching activity is independent

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of the genes that they regulate.

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To characterize the specificity of Hits 3-5 and 3-8, we tested riboswitch activity to

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caffeine and TPP. Caffeine is structurally similar to theophylline and only differs by a

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methyl group on N-7. TPP, on the other hand, is structurally distinct from theophylline.

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Using the pLac-rbsw-tetA-gfp+ constructs, neither Hits 3-5 nor 3-8 display activity to

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TPP (Figure 1C). However, both hits show slightly increased activity to caffeine

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compared to theophylline (Figure 1C). Because we did not incorporate into our platform

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a feature that identifies theophylline binders and simultaneously excludes caffeine

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binders, this finding is unsurprising. As a comparison, experiments of previously

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reported theophylline aptamers isolated by SELEX incorporated three rounds of a

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“counterselection” in which RNA library members capable of binding both theophylline

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and caffeine were discarded, resulting in sequences with a 1000-fold selectivity for

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theophylline over caffeine.30 When those SELEX-selected aptamers were incorporated

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into riboswitches, they maintained selectivity.12 While our hits do show promiscuity to

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the general methylxanthine structure, they are able to discriminate against a distinctly

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different target compound.

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The dose-responses of Hits 3-5 and 3-8 to theophylline and caffeine were examined in

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fluorescence assays using the pLac-rbsw-tetA-gfp+ constructs. The EC50 values of Hit

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3-8 to theophylline (0.9 mM) and caffeine (0.8 mM) are slightly lower than those of Hit 3-

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5 (6.6 and 1.0 mM, respectively) (Figure 3). For comparison, a riboswitch developed

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using the mTCT8-4 aptamer was reported to have an EC50 of 0.25 mM.12 Using a SYBR

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Green I assay,32,33 the Kd of the full-length 5’ UTR of Hit 3-5 for theophylline and

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caffeine was determined to be 238 and 299 µM, respectively (Figure S6). Using the

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same assay, we determined the Kd of the mTCT8-4 aptamer to be 373 nM, in line with

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previously measured values.34

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The switching activity of the original ThiM#2 in response to TPP is thought to be a result

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of translational regulation;23 however, northern analysis indicates that for Hit 3-5

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addition of theophylline to the growth medium increased tetA-gfp+ mRNA levels ~3-fold,

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indicative of regulation of gene expression via effects on either transcriptional read

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through or mRNA stability (Figure S7). The relatively low binding affinity of Hits 3-5 and

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3-8 may be a result of a mechanism that relies more on fast binding to allow for

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increased transcription processivity, rather than a highly stable binding-event that would

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be needed to affect translation.18

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We set out to determine if our platform could be used to improve the activity of Hit 3-5.

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We re-synthesized the 40 nt aptamer domain and the 16 nt expression platform of Hit 3-

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5 with a 24% mutagenesis rate, which would theoretically result in an average of 13

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point mutations per sequence. This new library was incorporated into the pLac-tetA-gfp+

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backbone and introduced into E. coli, resulting in a 107 library. Prior to selections and

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screens on this library, we sequenced eight clones and measured activity to

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theophylline (Table S3, Figure S8). As expected, random mutagenesis generally ablates

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riboswitch activity. This library was then subjected to three rounds of selection, including

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both ON- and OFF-sorting from the second round, forward. The concentrations of

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theophylline (1 mM), tetracycline (30, 40, and 50 μg/mL), and Ni2+ (0.3 mM) used were

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the same as those used in the original selections that yielded Hits 3-5 and 3-8. After just

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two rounds, the activity of several isolates had improved, compared to the parent. One

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isolate demonstrated nearly 3-fold activation, a 35% increase from Hit 3-5 (Figure 4A).

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While one additional round of dual selection and sorting did result in enrichment of

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specific sequences, the fold-activation did not significantly improve (data not shown).

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The seven isolated sequences each had on average two mutations in the expression

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platform region of the original ThiM#2 template (Table S4). It is expected that efficient

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coupling of the sensor and the actuator would be required for an effective riboswitch.

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Additional analysis of the isolates that demonstrated improved activation, along with Hit

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3-5, point to specific nucleotides that are strictly conserved in the 56 nt region that

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includes the aptamer domain and expression platform [e.g. nucleotides 9-13 (GUCAA)

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and 39-42 (UUGC)] (Figure 4B). Overall, in the analyzed active isolates, 27 out of 56 nt

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are strictly conserved, whereas the randomly selected and sequenced members of the

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mut389 starting library only have 7 nt that are “conserved” by chance (Table S3). The

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strictly conserved residues in the active isolates, as well as other residues that are

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highly conserved, likely contribute to riboswitch function.

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We have presented a platform to discover new riboswitches in which the selection of the

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sensor and actuator domains takes place inside the cell. Thus, from the start, the

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complexities of the cellular environment and how it may impact RNA folding and RNA-

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ligand binding are factored in to the selection process. The starting 108 library size was

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likely critical to the success of our approach.15 Previous efforts to identify riboswitches

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through dual genetic selection or FACS-screens involved starting libraries on the order

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of 104-105.23–25,28,29 In each of those cases, however, the starting library included an

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aptamer domain either provided by nature or selected via SELEX. The complexity of the

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problem we addressed – identifying an aptamer domain in vivo – warranted a larger

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starting library, which are typically limited by the transformation efficiency of bacteria to

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~109. In comparison, in vitro selections of aptamers often start with libraries of at least

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1013 unique molecules.35–37 At the same time, solution frequencies as low as 1 in 108

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have been previously observed for in vitro selection of aptamers against small

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molecules.36,37 In the example presented here, the solution-frequency we encountered

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deemed a 108 library adequate for identifying aptamer domains for the small molecule

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theophylline via an in vivo platform. An additional round of mutagenesis of one of our

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original hits, which increased the total numbers of sequences sampled, was able to

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further improve the activity of our selected riboswitch.

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The choice of theophylline as the ligand of interest to validate our approach is grounded

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upon the following rationale: First, since theophylline is a molecule with a known

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riboswitch, we reasoned that a riboswitch ‘solution’ was indeed possible. Second, the

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existing theophylline riboswitch has been extensively studied and reengineered by

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many different research groups, giving us additional opportunities for comparison of

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potential hits using our platform.12,28–31,38 Indeed, the riboswitches that we identified

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contain sequences entirely distinct from previously studied theophylline riboswitches

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and affect transcription of downstream genes, rather than translation.12,26,31 We

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anticipate that the general platform provided here, involving the combination of a large

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(108-109) starting library to identify modest initial hits, followed by additional directed

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evolution, will serve as a template for identifying other novel riboswitches.

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Methods

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Reagents. All oligonucleotides were purchased from Integrated DNA Technologies;

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primers used in this study are listed in Table S5. All cloning enzymes were purchased

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from New England Biolabs. All PCR reactions were performed using Q5 DNA

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Polymerase. Gibson Assembly Master Mix or Hi-Fi DNA Assembly Master Mix was

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used for DNA fragment assembly to generate plasmid constructs. Theophylline,

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caffeine, and thiamine were purchased from Sigma Aldrich.

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Bacterial Strains and Growth Conditions. All strains used in this study are described

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in Table S6. Strains were grown at 37 °C with orbital shaking at 250 rpm in LB broth or

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M9 minimal medium containing 0.8% w/v glycerol. Unless otherwise stated, the minimal

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medium source was supplemented with 0.1% casamino acids, 0.1 mM CaCl2, 2 mM

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MgSO4, and 0.1 mM thiamine. Carbenicillin was used as an antibiotic at 50-100 μg/mL.

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Library Construction and Plasmid Cloning. In order to amplify pthiM#2-tetA-gfp+, a

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variant of pthiM#2-tetA-gfpuv,24 without its 34-base pair aptamer domain, PCR was

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performed with primers pthiM#2tetAgfp forward and pthiM#2tetAgfp reverse (0.5 μM,

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each), using the pthiM#2-tetA-gfp+ template (0.5 – 1 ng/μL). PCR was performed with

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an initial denaturation step of 30 s at 98 °C followed by 25 cycles of 10 s at 98 °C, 30 s

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at 67 °C, and 2.5 min at 72° C. The PCR product was treated twice, consecutively, with

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DpnI (40 units at 37 °C for 60 min, each). The DNA was purified using the QIAquick

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PCR Purification kit (QIAGEN) and quantified by gel electrophoresis. This backbone

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was assembled (3:1 insert to vector ratio) with an oligonucleotide containing a

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randomized (machine-mixed) 40 base pair region (5’-

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CGTGAAGGCTGAGAAATACCCGNNNNNNNNNNNNNNNNNNNNNNNNNNNNNNNN

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NNNNNNNNGCTATTACAAGAAGATCAGGAGCAAAC-3’). The assembled product

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(Figure S9) was purified using the QIAquick PCR Purification kit and eluted in 40 μL

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water. Transformation of the plasmid library into TOP10 E. coli cells (Invitrogen) was

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performed by electroporation at 2000 V. Transformed cells were recovered in 2x YT for

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30 minutes at 37 °C with aeration at 250 rpm. Dilutions (10-3, 10-4, and 10-5) of the

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transformed cells were plated on LB agar plates containing 50 μg/mL carbenicillin and

313

library size was estimated from the number of colonies formed. The remaining library

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was grown overnight in 2x YT with 50 μg/mL carbenicillin and then stored at -80 °C in

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20% glycerol the following day. The 10-5 plate contained 1880 colonies, providing an

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Engineering riboswitches in vivo

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estimate of library size of 1 x 108. Sequencing of 8 randomly-selected isolates afforded

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eight unique sequences (Table S1), none of which were the starting pthiM#2-tetA-gfp+

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plasmid.

319 320

To construct the mutagenized Hit 3-5 (m389) library, the same procedure as above was

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used, but using the following machine-mixed oligonucleotide during DNA assembly: 5’ -

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GCTGAGAAATACCCGCACTGTTCGTCAAGAAAGCATCATTGTGACTGTGTAGATTG

323

CTATTACAAGAAGATCAGGAGCAAACTATG, in which the underlined sequence,

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corresponding to the aptamer and expression platform regions, was mutagenized at a

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24% rate. The resulting library was transformed into E. coli, plated and recovered, as

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above. The 10-4 and 10-5 plates contained 1100 and 142 colonies, respectively,

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providing an estimate of library size of 1 x 107. Sequencing of 8 randomly-selected

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isolates afforded eight unique sequence, each of which was different from the parental

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sequence (Table S3).

330 331

Dual Genetic Selection and Fluorescence-Activated Cell Sorting. The library was

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diluted to an optical density (OD600) of 0.05 (~108 cells) in 20 mL M9 medium with 100

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μg/mL carbenicillin. Prior to positive and negative selections, the cultures were

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incubated at 37 °C with aeration at 250 rpm for 4-6 hours with or without a ligand of

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interest (1 mM). The incubated cultures were diluted to an OD600 of 0.05 (~108 cells) in

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20 mL fresh M9 medium containing either the ligand of interest (1 mM) and tetracycline

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(30–50 μg/mL) for positive selections or nickel chloride (0.3 mM) for negative selections

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and incubated at 37 °C with orbital shaking at 250 rpm for 12-20 hours.

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Fluorescence-activated cell sorting (FACS) was performed following selections in the

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second and third rounds. Selection cultures were washed and subsequently diluted

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1:100 (~107 cells/mL) in 1 x M9 salts. FACS was carried out using a Biorad S3™ Cell

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Sorter with excitation using a 488 nm laser and fluorescence detected using a 525/30

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bandpass filter. Approximately 106 cells were interrogated and of those, the 5-10% most

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(ON) or least (OFF) fluorescent were collected in LB broth with 50 μg/mL carbenicillin

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and recovered at 37 °C with aeration at 250 rpm for 12-20 hours.

347 348

Fluorescence Assays. Fluorescence assays were performed following rounds of

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selections and screens. Strains were incubated overnight in M9 medium. Cultures were

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diluted to an OD600 of 0.05 and incubated until they reached an OD600 of ~0.2-0.3. The

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cultures were split into two fractions and incubated with or without theophylline (1 mM),

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caffeine (1 mM), or thiamine (0.1 mM) for 1-2 hours. Cultures were either diluted 1:5-

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1:10 in 1 X PBS or 0.5-1 mL were pelleted (8,000 x g, 5 min) and resuspended in 1 x

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PBS. Samples (200 μL) were transferred to a 96-well optical-bottom plate and relative

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fluorescence (excitation at 480 nm, emission at 520 nm) and OD600 were measured

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using a Biotek Synergy 4 plate-reader. The relative fluorescence units (RFU) of each

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sample were normalized to the OD600 reading of each sample to provide the reported

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RFU/OD600 value. Assays were performed with three or five biological replicates in

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technical duplicate or triplicate. For fluorescence assays testing the dose response of

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potential riboswitches, concentrations of theophylline ranged from 0.025 - 2 mM.

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Nonlinear regression and statistical analyses were performed using Prism GraphPad.

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362 363

Beta-Galactosidase Assays. Strains were grown, as above for the fluorescence

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assays. After 1-2 h of treatment of with ligand of interest, OD600 measurements of

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cultures (250 μL) were recorded in clear 96-well plates (Costar) using a Biotek Synergy

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4 plate-reader. Cells (100 μL) were lysed for at least 25 minutes with lysis buffer (10 μL)

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containing PopCulture Reagent (Novagen) and lysozyme (ThermoFisher). Cell lysate

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(30 μL) was incubated (28 °C) with substrate solution (150 μL; 60 mM Na2HPO4, 40 mM

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NaH2PO4, 1 mg/mL o-nitrophenyl-β-D-Galactoside (ONPG), 2.7 μL/mL β-

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mercaptoethanol) and absorbance at 420 nm was recorded every 30 seconds for 1 hour

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using a Biotek Synergy 4 plate-reader. Reported values are in units of mean

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OD420/min/OD600. Results are representative of at least three biological replicates.

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Statistical analyses were performed using Prism GraphPad.

374 375

Author Contributions

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K.P, J.S. and J.M.L. performed all of the experiments with assistance from S.L and M.Z.

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K.P. and J.M.L wrote the paper, with editorial assistance from all authors. J.M.L.

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conceived and supervised the study.

379 380

Supporting Information


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The Supporting Information is available free of charge on the ACS Publications website

382

at DOI: XXXXX.

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Further experimental details, including plasmid cloning, sequencing and RNA analysis;

384

additional figures, tables, and their references (PDF)

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385 386

Acknowledgements

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We would like to thank Dr. Yohei Yokobayashi for providing the original plasmid

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expressing a thiM#2-tetA-gfpuv fusion. The research was funded by Pomona College

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and an NSF grant to J.M.L. (CBET-1258307). J.M.L. is a Henry-Dreyfus Teacher-

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Scholar. We thank Erick Velasquez and Marek Zorawski for their technical assistance at

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the start of this project and Greg Copeland for critical readings of the manuscript.

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References

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(1) Serganov, A., and Nudler, E. (2013) A decade of riboswitches. Cell 152, 17–24. (2) Mehdizadeh Aghdam, E., Hejazi, M. S., and Barzegar, A. (2016) Riboswitches: From living biosensors to novel targets of antibiotics. Gene 592, 244–259. (3) Zhou, L.-B., and Zeng, A.-P. (2015) Exploring lysine riboswitch for metabolic flux control and improvement of L-lysine synthesis in Corynebacterium glutamicum. ACS Synth. Biol. 4, 729–734. (4) Blount, K. F., Wang, J. X., Lim, J., Sudarsan, N., and Breaker, R. R. (2007) Antibacterial lysine analogs that target lysine riboswitches. Nat. Chem. Biol. 3, 44. (5) Weigand, J. E., and Suess, B. (2009) Aptamers and riboswitches: perspectives in biotechnology. Appl. Microbiol. Biotechnol. 85, 229. (6) Fowler, C. C., Brown, E. D., and Li, Y. (2010) Using a riboswitch sensor to examine coenzyme B12 metabolism and transport in E. coli. Chem. Biol. 17, 756–765. (7) Bell, C. L., Yu, D., Smolke, C. D., Geall, A. J., Beard, C. W., and Mason, P. W. (2015) Control of alphavirus-based gene expression using engineered riboswitches. Virology 483, 302–311. (8) Michener, J. K., and Smolke, C. D. (2014) Synthetic RNA switches for yeast metabolic engineering. Methods Mol. Biol. Clifton NJ 1152, 125–136. (9) Werstuck, G., and Green, M. R. (1998) Controlling gene expression in living cells through small molecule-RNA interactions. Science 282, 296–298. (10) Weigand, J. E., Sanchez, M., Gunnesch, E.-B., Zeiher, S., Schroeder, R., and Suess, B. (2008) Screening for engineered neomycin riboswitches that control translation initiation. RNA 14, 89–97. (11) Hanson, S., Berthelot, K., Fink, B., McCarthy, J. E. G., and Suess, B. (2003) Tetracycline-aptamer-mediated translational regulation in yeast. Mol. Microbiol. 49, 1627–1637. (12) Desai, S. K., and Gallivan, J. P. (2004) Genetic screens and selections for small molecules based on a synthetic riboswitch that activates protein translation. J. Am. Chem. Soc. 126, 13247–13254.

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(13) Jang, S., Jang, S., Xiu, Y., Kang, T. J., Lee, S.-H., Koffas, M. A., and Jung, G. Y. (2017) Development of artificial riboswitches for monitoring of naringenin in vivo. ACS Synth. Biol. 6, 2077–2085. (14) Wu, M.-C., Lowe, P. T., Robinson, C. J., Vincent, H. A., Dixon, N., Leigh, J., and Micklefield, J. (2015) Rational re-engineering of a transcriptional silencing PreQ1 riboswitch. J. Am. Chem. Soc. 137, 9015–9021. (15) Jijakli, K., Khraiwesh, B., Fu, W., Luo, L., Alzahmi, A., Koussa, J., Chaiboonchoe, A., Kirmizialtin, S., Yen, L., and Salehi-Ashtiani, K. (2016) The in vitro selection world. Methods 106, 3–13. (16) Berens, C., and Suess, B. (2015) Riboswitch engineering—making the allimportant second and third steps. Curr. Opin. Biotechnol. 31, 10–15. (17) Groher, Florian, Bofill-Bosch, C., Schneider, C., Braun, J., Jager, S., Geißler, K. H., and Seuss, B. (2018) Riboswitching with ciprofloxacin—development and characterization of a novel RNA regulator. Nucleic Acids Res. 46, 2121-2132. (18) Etzel, M., and Mörl, M. (2017) Synthetic riboswitches: from plug and pray toward plug and play. Biochemistry 56, 1181–1198. (19) Kim, Y.-B., Wacker, A., Laer, K. von, Rogov, V. V., Suess, B., and Schwalbe, H. (2017) Ligand binding to 2΄-deoxyguanosine sensing riboswitch in metabolic context. Nucleic Acids Res. 45, 5375–5386. (20) Porter, E. B., Polaski, J. T., Morck, M. M., and Batey, R. T. (2017) Recurrent RNA motifs as scaffolds for genetically encodable small-molecule biosensors. Nat. Chem. Biol. 13, 295–301. (21) Dixon, N., Duncan, J. N., Geerlings, T., Dunstan, M. S., McCarthy, J. E., Leys, D., and Micklefield, J. (2010) Reengineering orthogonally selective riboswitches. Proc. Natl. Acad. Sci. 107, 2830–2835. (22) Robinson, C. J., Vincent, H. A., Wu, M.-C., Lowe, P. T., Dunstan, M. S., Leys, D., and Micklefield, J. (2014) Modular riboswitch toolsets for synthetic genetic control in diverse bacterial species. J. Am. Chem. Soc. 136, 10615–10624. (23) Nomura, Y., and Yokobayashi, Y. (2007) Reengineering a natural riboswitch by dual genetic selection. J. Am. Chem. Soc. 129, 13814–13815. (24) Muranaka, N., Sharma, V., Nomura, Y., and Yokobayashi, Y. (2009) An efficient platform for genetic selection and screening of gene switches in Escherichia coli. Nucleic Acids Res. 37, e39–e39. (25) Zhou, L.-B., and Zeng, A.-P. (2015) Engineering a lysine-ON riboswitch for metabolic control of lysine production in Corynebacterium glutamicum. ACS Synth. Biol. 4, 1335–1340. (26) Sharma, V., Nomura, Y., and Yokobayashi, Y. (2008) Engineering complex riboswitch regulation by dual genetic selection. J. Am. Chem. Soc. 130, 16310–16315. (27) Nomura, Y., and Yokobayashi, Y. (2007) Dual selection of a genetic switch by a single selection marker. Biosystems 90, 115–120. (28) Lynch, S. A., and Gallivan, J. P. (2009) A flow cytometry-based screen for synthetic riboswitches. Nucleic Acids Res. 37, 184–192. (29) Fowler, C. C., Brown, E. D., and Li, Y. (2008) A FACS-based approach to engineering artificial riboswitches. ChemBioChem 9, 1906–1911. (30) Jenison, R. D., Gill, S. C., Pardi, A., and Polisky, B. (1994) High-resolution molecular discrimination by RNA. Science 263, 1425–1429.

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(31) Lynch, S. A., Desai, S. K., Sajja, H. K., and Gallivan, J. P. (2007) A high-throughput screen for synthetic riboswitches reveals mechanistic insights into their function. Chem. Biol. 14, 173–184. (32) McKeague, M., Velu, R., Hill, K., Bardóczy, V., Mészáros, T., and DeRosa, M. C. (2014) Selection and characterization of a novel DNA aptamer for label-free fluorescence biosensing of ochratoxin A. Toxins 6, 2435–2452. (33) McKeague, M., De Girolamo, A., Valenzano, S., Pascale, M., Ruscito, A., Velu, R., Frost, N. R., Hill, K., Smith, M., and McConnell, E. M. (2015) Comprehensive analytical comparison of strategies used for small molecule aptamer evaluation. Anal. Chem. 87, 8608–8612. (34) Chang, A. L., McKeague, M., Liang, J. C., and Smolke, C. D. (2014) Kinetic and equilibrium binding characterization of aptamers to small molecules using a label-free, sensitive, and scalable platform. Anal. Chem. 86, 3273–3278. (35) Ruscito, A., and DeRosa, M. C. (2016) Small-molecule binding aptamers: Selection strategies, characterization, and applications. Front. Chem. 4. (36) Ellington, A. D., and Szostak, J. W. (1990) In vitro selection of RNA molecules that bind specific ligands. Nature 346, 818-822. (37) Ellington, A. D., and Szostak, J. W. (1992) Selection in vitro of single-stranded DNA molecules that fold into specific ligand-binding structures. Nature 355, 850-852. (38) Zimmermann, G. R., Jenison, R. D., Wick, C. L., Simorre, J.-P., and Pardi, A. (1997) Interlocking structural motifs mediate molecular discrimination by a theophyllinebinding RNA. Nat. Struct. Mol. Biol. 4, 644–649.

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Figure 1. Selections and screens on a riboswitch library uncovered two unique theophylline riboswitches. (A) The N40 plasmid library consists of a degenerate 40nucleotide sequence, the ThiM#2 expression platform, RBS, and tetA-gfp+ fusion. (B) Hit 3-5, Hit 3-8, and mTCT8-4 regulate expression of the tetA-gfp+ fusion in response to theophylline (1 mM) and display a 2.3, 2.1, and 15.8-fold activation, respectively. (C) Within the context of pLac-rbsw-tetA-gfp+, Hits 3-5 and 3-8 exhibit a 3.3 and 2.9-fold activation to caffeine (1 mM), respectively, and do not exhibit activity to thiamine (0.1 mM). Data are representative of three biological replicates. Bars indicate mean values and error bars indicate standard deviation. *** p < 0.001, **** p < 0.0001 by two-tailed ttest. “rbsw” stands for riboswitch and is indicative of the ThiM#2, 3-5, 3-8, or mTCT8-4 riboswitches in the construct.

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505 506 507 508 509 510 511 512

Figure 2. Hits 3-5 and 3-8 regulate lacZ expression in response to theophylline indendent of promoter. (A) Hits 3-5 and 3-8 display a 1.9 and 1.7-fold activation, respectively, in the context of pLac-rbsw-lacZ. (B) Hits 3-5 and 3-8 display a 1.7 -fold activation in the context of pBAD-rbsw-lacZ. Data are representative of three biological replicates. Bars indicate mean values and error bars indicate standard deviation. * p < 0.05, ** p < 0.01, *** p < 0.001, **** p < 0.0001 by two-tailed t-test comparing ON and OFF states.

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Engineering riboswitches in vivo

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A

B 5

513 514 515 516 517 518 519 520

4

pLac-3-5-tetA-gfp+

4

caffeine

3

theophylline

2 1

Fold Activation

Fold Activation

1 2 3 4 5 6 7 8 9 10 11 12 13 14 15 16 17 18 19 20 21 22 23 24 25 26 27 28 29 30 31 32 33 34 35 36 37 38 39 40 41 42 43 44 45 46 47 48 49 50 51 52 53 54 55 56 57 58 59 60

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pLac-3-8-tetA-gfp+ caffeine

3

theophylline

2 1

0 10-5 10-4.5 10-4 10-3.5 10-3 10-2.5

0 10-5 10-4.5 10-4 10-3.5 10-3 10-2.5

log[Ligand], M

log[Ligand], M

Figure 3. Hits 3-5 and 3-8 display a dose-response to theophylline and caffeine. EC50 values of riboswitches were obtained from fitting of the fold activation to log[Ligand]. EC50 of Hits 3-5 and 3-8 are, 6.6 mM and 0.9 mM, respectively, to theophylline and 1.0 mM and 0.8 mM, respectively, to caffeine. Data are representative of three biological replicates. Bars indicate mean values and error bars indicate standard deviation.

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Fold Activation

A

B

4 3

24

*

**

**

2 1 0

m ut 38 m 9-2 ut 38 -1 m 9-2 ut 38 -2 m 9-2 ut 38 -3 m 9-2 ut 38 -4 m 9-2 ut 38 -5 m 9-2 ut 38 -7 92H 8 it 35

1 2 3 4 5 6 7 8 9 10 11 12 13 14 15 16 17 18 19 20 21 22 23 24 25 26 27 28 29 30 31 32 33 34 35 36 37 38 39 40 41 42 43 44 45 46 47 48 49 50 51 52 53 54 55 56 57 58 59 60

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Isolate

Figure 4. Two rounds of selections and sorts on the mutagenized Hit 3-5 library resulted in riboswitch variants, several of which had improved fold-activation compared to the parental sequence (average fold-activation of 2.2 in these assays, as indicated by the dotted line). (A) Bars indicate mean values and error bars represent standard deviation of 2-3 biological replicates. * p < 0.05, ** p < 0.01 by two-tailed t-test compared to fold-activation of Hit 3-5. (B) Multiple sequence alignment of mut389-2-1, 2, 3, 4, 5, 7 and 8, along with Hit 3-5. Highlighted nucleotides indicate differences from Hit 3-5.

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Engineering riboswitches in vivo using dual genetic selection and fluorescenceactivated cell sorting Katharine Page, Jeremy Shaffer, Samuel Lin, Mark Zhang and Jane M. Liu Table of contents graphic:

+ ON 1. Nickel 2. Cell Sorting (OFF)

Selections + FACS

1. Tetracycline 2. Cell Sorting (ON)

OFF

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