One challenge for synthetic biologists is the predictable tuning of genetic circuit regulatory components to elicit desired outputs. Gene expression driven by ligand-inducible transcription factor systems must exhibit the correct ON and OFF characteristics: appropriate activation and leakiness in the presence and absence of inducer, respectively. However, the dynamic range of a promoter (i.e., absolute difference between ON and OFF states) is difficult to control. We report a method that tunes the dynamic range of ligand-inducible promoters to achieve desired ON and OFF characteristics. We build combinatorial sets of AraC-and LasR-regulated promoters containing −10 and −35 sites from synthetic and Escherichia coli promoters. Four sequence combinations with diverse dynamic ranges were chosen to build multi-input transcriptional logic gates regulated by two and three ligand-inducible transcription factors (LacI, TetR, AraC, XylS, RhlR, LasR, and LuxR). This work enables predictable control over the dynamic range of regulatory components.
Synthetic gene circuits are constructed by rewiring transcription factors and promoters to create novel regulatory topologies1,2,3,4,5. Promoters, which initiate transcription in response to transcription factors and associated ligands, are typically derived from endogenous components of the host or related species to ensure compatibility with the host transcription machinery. However, transcription rates of native promoters and their responses to inducers vary widely, as they are tuned to respond at rates appropriate to their natural setting6,7,8. This potential incongruity can cause problems when constructing gene circuits, as the fold-change induction of a natural promoter may not allow the synthetic circuit to behave as designed.
The first step in tuning a promoter is generally to change its overall output, i.e., to increase or decrease the amount of protein produced. This can be achieved in several ways. For instance, the copy number of the gene can be changed by placing it on different plasmids or by integrating it multiple times within the chromosome. Libraries of constitutive promoters have also been assembled and tested to achieve target expression levels9. In addition, although not technically part of the promoter, the 5′ untranslated region can be manipulated to alter translation rates and hence protein production9,10,11,12.
Many attempts have been made to engineer transcriptional systems that are better suited for use in synthetic gene circuits13,14,15,16,17,18. Tuning these regulatory pathways involves building and testing circuits with precharacterized −35 and −10 sites19 and Shine–Dalgarno sequences20 of varying strengths until the desired properties (e.g., leakiness, fold induction) are empirically achieved; however, this approach can be extremely labor-intensive and costly.
Furthermore, although these methods can help to control gene expression, they universally alter protein output regardless of inducer concentration and the dynamic range of gene expression may change in unpredictable ways. For example, if one were to increase the copy number of a gene to increase protein production, the rates of production increase for both the OFF state (in the absence of inducer) and the ON state (in the presence of inducer).
To date, hybrid promoters that respond to two or more transcription factors have been constructed in several ways, including: by encoding operator sites for multiple transcription factors into a single promoter21,22; by using two consecutive promoters, each with its own regulatory features and transcription start site18; or by engineering different transcription factors that bind to the same operator23,24. Others have engineered promoters that have altered overall production of either mRNA25,26,27 or protein10. However, the dynamic range of these synthetic promoters can be small—i.e., their outputs often show only a small difference between OFF and ON states in response to signal ligands that bind the transcription factors. Despite these advances in promoter engineering, the dynamic range of synthetic promoters has been difficult to tune. This problem prohibits the facile construction of multi-layer synthetic gene circuits, which require the output dynamic range of an upstream regulator to be compatible with the input dynamic range of a downstream target. Of note, ligand-inducible transcription factor systems can be manipulated at the level of the transcription factor as well as at the level of the promoter. In prior work, the leakiness and inducibility of the ligand-inducible LacI repressor mutants have been quantified and classified28. Such manipulation at the level of the transcription factor is informative and compatible with our promoter engineering approach, and both can be performed in conjunction to enable facile tuning of the dynamic range of synthetic promoters. Additionally, experimental studies have shown that inducibility and dynamic range can be tuned by changing the copy number of the plasmid encoding the transcription factor29,30, mutating the transcription factors31, changing the operator sequence6, mutating the RNA polymerase25, and reducing promoter crosstalk32. In addition, methods have been developed to calculate the probability of RNA polymerase binding at a promoter as a function of the number of regulatory proteins in the cell33,34. Recently, the insulation of minimal promoters was demonstrated to enable precise engineering and biophysical modeling of complex synthetic transcription circuits35. These approaches have inspired our study and are compatible with our promoter engineering approach to accomplish facile tuning of the dynamic range of promoters.
Here we built a library of Escherichia coli promoters that have a spectrum of dynamic ranges. To do so, we used a modular approach in which promoters were assembled from libraries of five main components: (1) the region upstream of the −35 site (in which an operator site for a transcriptional activator can reside); (2) the spacer region between the −10 and −35 sites (in which an operator site for a repressor can reside); (3) the −10 site; (4) the −35 site; and (5) the downstream region encoding the gene of interest. The fold-change induction of the promoters was tuned using a variety of −10 and −35 sites. We also developed a thermodynamic model that predicted the contribution of free energy of binding to the overall transcriptional initiation rate, which we measured in a fluorescence-based plate reader experiment.
Our prediction and identification of the dynamic range allowed us to identify the ideal promoters for building multi-input hybrid promoters that can be used to make transcriptional logic gates. To build transcriptional AND gates with high signal-to-noise ratios, we perused our screened promoter library to identify two members that exhibited high fold-change induction and used their −35 and −10 cores to build hybrid promoters that respond to a variety of small-molecule inducers. Each hybrid promoter exhibited robust AND gate behavior—i.e., strong expression in the presence of all inducers and negligible expression in the absence of one or more inducers.
Overall, our results provide a method for efficiently altering the dynamics range of ligand-inducible promoters. This ability is key for constructing synthetic gene regulatory circuits that require precise input and output relationships and will allow researchers to tune complex synthetic gene regulatory circuits in a facile fashion. This paper provides a simple, cost-effective means of engineering promoters that provide user-defined dynamic ranges, which will enable the fine-tuning of the metabolic flux within synthetic biological and chemical circuits inside living cells.
Predictable promoter behavior by motif-based construction
In growing E. coli cells, most promoters are regulated by σ70, a housekeeping transcription factor that binds the −10 and −35 sites of a promoter and enables RNA polymerase to bind and initiate transcription36. Transcription rates have been shown to be highly dependent on the sequences of the −10 and −35 sites for promoters regulated by σE and σ70, and certain −10 and −35 site combinations are associated with known transcription rates19,37,38.
Here we characterize the relationship between the free energy of σ70 binding to the −10 and −35 sites and the dynamic range of a library of promoters. We first formulated a thermodynamic model for transcriptional initiation based on the probability of σ70 binding to DNA13,14,15,16,17,18,34,39,40,41. First, predicted transcription rates were derived from the probability of σ70 binding, with the assumption that, in the presence of inducer, the probability of activator and σ70 both binding DNA is much higher than the probability of σ70 alone binding. Second, to describe the fold change in expression upon induction, the logarithms of the predicted transcription rates were fitted to the experimentally measured transcription rates, with the assumption that recorded fluorescence is proportional to the transcription rate. To account for the different regulatory architectures in this work, this thermodynamic model was modified to consider the additional binding states of the different transcription factors. Specifically, thermodynamic models were made for single (activator alone) and multiple (activator and repressor) transcription factors with different states of binding (+/+, +/−, −/+, −/−) modeled in order to capture the entire range of possible biochemical interactions (see Supplementary Note 1 for more details).
Our model predicted that the dynamic range of a promoter could be tuned by varying the sequences of the −10 and −35 sites of the promoter (Fig. 1). We assumed that changes at these sites affected the equilibrium constant, K eq, of σ70 binding to DNA: If K eq is low, σ70 binds poorly and the promoter will exhibit low leakiness but poor induction (bottom curve in Fig. 1b). If K eq is high, σ70 binds tightly and the promoter will exhibit good induction but high leakiness (top curve in Fig. 1b). We postulated that, for a range of moderate K eq values, a promoter can be made to exhibit low leakiness and high induction, i.e., a large dynamic range (middle curve in Fig. 1b).
To test our hypothesis that the dynamic range of a ligand-inducible promoter could be tuned by varying the K eq values of the −35 and −10 sites, we constructed a library of promoters (Fig. 2a), each of which contained: (1) a proximal operator-binding site for either AraC or LasR (immediately upstream of the −35 site); (2) various −10 and −35 sites derived from E. coli promoter consensus sequences, native promoters, synthetic promoters13,14, and arbitrary sequences; and (3) a fixed downstream reporter sequence encompassing the +1 site, a ribosome-binding site and the gene encoding yellow fluorescent protein (YFP). AraC and LasR were chosen because they are both ligand-inducible transcriptional activators but come from two different transcription factor families42,43. In addition, a LacI-binding site (LacO1) was encoded in the spacer region between the −10 and −35 sites to examine the influence of repressors on the behavior of these promoters.
Each promoter in the library was cloned into identical plasmid backbones (pMB1 origin, kanamycin resistance) and transformed into E. coli strain CY015, which is a ΔlacI ΔaraC strain that also constitutively expressed genomically encoded araC and lasR. We expected the promoters to be activated upon addition of their corresponding inducers, i.e., arabinose for AraC, and 3O-C12-HSL for LasR. To measure the relative promoter units (RPU), we used a standardized method that has been adopted by the research community19,44. We measured the transcription rate of each promoter in the library with and without inducer and observed that rankings of the −10 and the −35 sites were consistent between AraC- and LasR-regulated promoters regardless of the identity and presence of each inducer (Fig. 2b). For certain combinations of −10 and −35 sites, the promoters achieved a maximum expression level (~105 RPU)—an observation that is consistent with that of prior reports14,44. Fold-change induction heat maps were consistent between AraC- and LasR-regulated promoters (Fig. 2c), indicating that the dynamic ranges of ligand-inducible promoters are predominantly controlled by the sequences of the −35 and −10 sites.
To better understand the behavior of the promoters within the library, we fit our thermodynamic model to the experimentally observed transcription rates (see Supplementary Information). The experimental results supported the predicted effects of K eq on transcription rates (Fig. 3a, d) and fold-change induction (Fig. 3b, e). Of note, promoters exhibit a range of leakiness and inducibility depending on the free energy of σ70 binding, as shown in the induction curves for three different combinations of −10 and −35 sites (bD, dE, and eG) in the AraC- (Fig. 3c) and LasR-regulated (Fig. 3f) promoters.
To demonstrate that our method applies not only to activators but also extends to other mechanisms of transcriptional regulation such as repression, we next investigated the behavior of hybrid promoters that respond to both an activator (either AraC or LasR) and a repressor (LacI) (Fig. 4a). To this end, we tested our promoter library in strain CY012, which is genetically identical to CY015 with the exception of a constitutively expressed genomically encoded lacI. The promoters were characterized under four conditions: in the presence of (a) neither inducer, (b) inducer of the activator only (arabinose or 3O-C12-HSL), (c) inducer of the repressor only (isopropyl β-d-1-thiogalactopyranoside (IPTG)), and (d) both inducers. The results were similar to those obtained in the absence of lacI—the ordering of −10 and −35 sites based on measured transcription rates was consistent under all four conditions. This data was also consistent with our two-input thermodynamic model in which extra states were included to account for repressor binding (Fig. 4b, c; Supplementary Information).
Engineering responsive hybrid promoters
To demonstrate the utility of our predictive model and experimental dataset for the construction of synthetic ligand-inducible promoters that behave as desired, we opted to perform a logic operation that required high inducibility and low leakiness (Supplementary Figure 3). Thus we decided to build AND gates using −35 and −10 combinations that were predicted and observed to exhibit the largest dynamic range. We assembled hybrid promoters that are tightly controlled by multiple ligand inputs beyond those tested above (Fig. 5). Specifically, these hybrid promoters contained operator sequences (upstream of the −35 site) that bind a variety of ligand-inducible transcriptional activators: AraC (arabinose), XylR (xylose), RhlR (C4-HSL), LasR (3O-C12-HSL), and LuxR (3O-C6-HSL). Additionally, we included operator sites for either LacI (LacOsym) or TetR (TetO2) in the spacer region to allow repression by these proteins6,13. For the −35 site, we chose to characterize version “d” (TTTACA) further because it provided medium affinity for σ70. First, we slightly modified version “d” (TTTACA) to TTTACT because the terminal nucleotide, T, (a) is the second most common base pair at that position45, (b) creates a one base pair overlap with the LacOsym operator site, (c) is known to decrease the leakiness of the promoters in the presence of the repressor6,13, and (d) the nature of this DNA substitution mutation does not alter the binding affinity of σ70 for this −35 site25. As for the −10 sites, we chose versions “E” (GATACT) and “F” (GATAAT), because both of these sequences possess a 2 bp overlap with the TetO2-binding site (allowing facile integration of the TetO2 site) while providing different dynamic ranges. We posited that the difference in dynamic ranges would manifest as differences in the leakiness (basal transcription rates) and inducibility (induced transcription rates) of the AND gates built with these sequences. Specifically, version E that exhibited lower leakiness and lower inducibility was expected to provide tighter repression and lower induction, while version F that exhibited higher leakiness and higher inducibility was expected to provide leakier repression and higher induction. Two additional LacO1 and TetO2 sites were also added (one downstream and one ~400 bp upstream of the +1 site) to achieve further repression46.
As desired, all combinations of the hybrid promoters exhibited high induction only in the presence of both inducers and low signal in the presence of neither inducer (Fig. 5a). As expected, the “dE” combination of −10 and −35 sites provided tighter transcriptional regulation than the “dF” combination, which provided higher induction but was slightly more leaky than promoters with the “dE” combination (Fig. 5a).
To demonstrate that the high-inducibility and low-leakiness properties of these −35 and −10 combinations extend to multi-input hybrid promoters that are more complex, we constructed hybrid promoters that respond to three different inputs. For each three-input hybrid promoter, we included the “dE” or “dF” site, an activator-binding site (for AraC, XylR, RhlR, LasR, or LuxR), a LacOsym-binding site in the spacer region, and two TetO2 sites at the +1 position and upstream (~ −400 bp) region. Of note, the TetO2 site at the +1 position provided more repression capacity than the upstream TetO2 site. We observed that these hybrid promoters exhibited high gene expression if and only if all three inducers were present (Fig. 5b). These hybrid promoters demonstrate the utility of our experimental dataset for identifying the optimal −35 and −10 combinations for engineering gene expression.
Finally, to demonstrate the utility of our method for engineering synthetic promoters with desired dynamic ranges, we tested the bD and eG promoters, which possess distinct ON and OFF characteristics compared to dE and dF. Specifically, in contrast to the low-leak and high-signal performance of dE and dF (Supplementary Figure 3), promoter bD has low leak and low signal while promoter eG has high leak and high signal (Fig. 3c). As expected, the two-input (Fig. 5a) and three-input (Fig. 5b) hybrid promoters that contain the bD and eG sequences exhibit low leak and low signal as well as high leak and high signal, respectively (Fig. 5).
To date, synthetic gene circuits have been constructed primarily by cobbling together regulatory parts drawn from disparate pathways. For instance, the original genetic toggle switch1 contained the repressors LacI (which regulates lactose metabolism) and TetR (which regulates the response to tetracycline). Because the lac and tet systems evolved separately, the promoters that respond to LacI and TetR are tuned to transcribe downstream genes at rates appropriate to their original setting. This tuning incongruity can cause problems for synthetic biologists, as the transcriptional response of a promoter needs to match the synthetic context of the circuit. Unfortunately, traditional strategies of testing −35 and −10 combinations and Shine–Dalgarno sequences of varying strengths to empirically achieve desired properties (with respect to, say, leakiness and inducibility) can be extremely time-consuming and labor-intensive.
In this study, we developed a method for tuning the difference between the ON and OFF states of a regulated promoter. We created a library of −10 and −35 sites that exhibit a wide range of fitted binding energies (inferred by fitting transcriptional data to a mathematical model) for σ70 and characterized how the fitted binding energies affect the uninduced vs induced transcription rates of ligand-inducible promoters. Despite the relatively small number of examined −10 and −35 sites (a total of 48 combinations), our library members spanned the full range of possible input and output relationships, i.e., the data points span the entire breadth of the dynamic range curves shown in Figs. 3a, b and 4b, c. We further demonstrated the utility of our method for building synthetic gene circuits by using it to select optimal −35 and −10 combinations for building two- and three-input hybrid promoters with high inducibility and low leakiness.
Note that our model for transcriptional repression is not as quantitatively accurate as our model for transcriptional activation, possibly because our model does not account for additional biophysical states that may be assumed by the DNA during transcriptional repression (e.g., DNA looping41). Therefore, in the absence of inducers that bind the transcriptional repressors, the predicted transcription rates can deviate from the data for higher values of ln(K eq) (see gray plots in Fig. 4b, c).
Since the characteristics of each −10 and −35 site combination were independent of the transcription factor(s) being used to regulate the promoter (Figs. 3a, d and 4b, d), this approach should apply to the host of novel transcription factors that have been developed to regulate σ70-based synthetic gene circuits23,47 (provided the transcription factors have known ligands). Additionally, when used in conjunction with methods for controlling protein production rates, our approach should provide exquisite control over the dynamic range of gene expression in synthetic gene circuits.
Strains and plasmids
We performed our experiments in E. coli strains derived from wild-type MG1655. To minimize interference of endogenous LacI with our exogenous LacI repressor, we performed lambda Red recombination48,49 to prepare a LacI- strain—CY011 (E. coli strain MG1655 ∆lacI). In addition, since an E. coli LuxR homolog, sdiA, can partially activate Prhl 50, we knocked out sdiA from CY011 to create CY013 (CY011 ∆sdiA). In order to test our −35 and −10 combinations in the context of three different promoters and transcription regulators, we built a plasmid pCH035 encoding wild-type araC, P trc* -rhlR (cloned from ATCC #47085), and P Iq -lasR (cloned from ATCC #47085) and performed lambda Red recombination to integrate these genes into the genome of CY013 to obtain CY015 (CY013 wt-araC, P trc* -rhlR, P Iq -lasR). Next, to test repressor function, we integrated P Iq -LacI and P N25 -TetR into the original LacI site of CY013 and CY015 via lambda Red recombination to obtain CY019 (CY013 P Iq -LacI P N25 -TetR) and CY021 (CY015 P Iq -LacI P N25 -TetR), respectively. After each recombination, antibiotic markers were removed by FLP-FRT recombination.
To construct the promoter library, we used a modified Golden Gate strategy51 wherein BsaI was used to create a specific restriction site in the spacer region. The first segment contains the activator-binding site and the −35 site; the second segment contains the −10 site, a ribosome-binding site, and yfp (T203Y mutant of sfGFP) reporter gene9. After PCR amplification of each segment, all segments were ligated to the plasmid backbone (KanR and pMB1 +rop origin) in all possible combinations. We used a similar strategy to construct the two- and three-input hybrid promoters. The genomic copy of XylR was used, but the majority of the activators were either integrated into the genome (AraC, LasR, and RhlR) or supplied on a separate plasmid (LuxR) (ChlorR and pSC101 origin).
All strains, plasmids, and promoter sequences used in this research are listed in Supplementary Tables 1–4. Key plasmids and strains are listed in Supplementary Table 5 and will be available by request on Addgene (https://www.addgene.org/Matthew_Bennett/) under the publication identifier corresponding to this manuscript.
Promoter strength assay
To measure the strengths of each −35 and −10 combination for promoters of the three activators, we first transformed the reporter plasmids encoding our library of promoters into strain CY015. We used the PBAD, Plas, and Prhl promoters as reference standards against which we standardized the strengths of each member of the promoter library52. To measure the strengths of each −35 and −10 combination for promoters of the two repressors, we used strain CY021, a LacI, and TetR knock in strain. In the two- and thre-input hybrid promoter assay, we transformed plasmids encoding the additional activator (LuxR) and hybrid promoters into CY015.
The strains were cultured overnight in LB media with 50 μg/mL kanamycin (and 25 μg/mL chloramphenicol as needed). The overnight cultures were inoculated at 1% volume per volume into 100 μL M9 media supplemented with 0.4% glycerol and 0.2% casamino acids and transferred into a 96-well plate. After growth with shaking at 37 °C for 2 h, 100 μL M9 media with 2× inducer was added to the cultures. The final concentrations of all inducers were as follows: C4-HSL (10 μM), 3O-C6-HSL (0.1 μM), 3O-C12-HSL (0.1 μM), arabinose (5 mM), xylose (5 mM), IPTG (1 mM), and ATc (100 ng/mL). Cultures were grown at 37 °C and 800 rpm in a plate shaker. The fluorescence of YFP was measured after 2 h using a plate reader (Tecan Infinite M1000; excitation 515 ± 5 nm, emission 528 ± 5 nm; PMT gain of 100) and reported as Fluotest_promoter = (fluorescence4h−fluorescence2h) per OD600 52. Reference standards were included on each 96-well plate. The final promoter strength was calculated in RPU using the equation RPUtest_promoter = Fluotest_promoter×RPUreference_standard)×Fluoreference_standard −1.
Commented code and all collected coding data are available in the Github repository at https://github.com/josic/Promoter-Engineering.
We thank Dr. Mengyang Cao for his kind advice. This work was funded by the National Institutes of Health, through the joint NSF/NIGMS grant R01GM104974 (M.R.B., K.J., W.O.) and the NIGMS grant R01GM117138 (to M.R.B., K.J., W.O.); the National Science Foundation grant DMS-1122094 (to K.J.); and the Robert A. Welch Foundation grant C-1729 (to M.R.B.).
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