A genetic bistable switch utilizing nonlinear protein degradation
© Huang et al.; licensee BioMed Central Ltd. 2012
Received: 6 March 2012
Accepted: 14 June 2012
Published: 9 July 2012
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© Huang et al.; licensee BioMed Central Ltd. 2012
Received: 6 March 2012
Accepted: 14 June 2012
Published: 9 July 2012
Bistability is a fundamental property in engineered and natural systems, conferring the ability to switch and retain states. Synthetic bistable switches in prokaryotes have mainly utilized transcriptional components in their construction. Using both transcriptional and enzymatic components, creating a hybrid system, allows for wider bistable parameter ranges in a circuit.
In this paper, we demonstrate a tunable family of hybrid bistable switches in E. coli using both transcriptional components and an enzymatic component. The design contains two linked positive feedback loops. The first loop utilizes the lambda repressor, CI, and the second positive feedback loop incorporates the Lon protease found in Mesoplasma florum (mf-Lon). We experimentally tested for bistable behavior in exponential growth phase, and found that our hybrid bistable switch was able to retain its state in the absence of an input signal throughout 40 cycles of cell division. We also tested the transient behavior of our switch and found that switching speeds can be tuned by changing the expression rate of mf-Lon.
To our knowledge, this work demonstrates the first use of dynamic expression of an orthogonal and heterologous protease to tune a nonlinear protein degradation circuit. The hybrid switch is potentially a more robust and tunable topology for use in prokaryotic systems.
As is well known, bistability is a fundamental property of a vast array of engineered and natural systems. Bistability confers the ability to switch, to retain state, and to store information, all three comprising a closely related set of operations common to computational systems. Not surprisingly, bistable networks and components are found to be central to many cellular processes, ranging from cell cycle and differentiation, to cell fate determinations and environmental sensing [1–6]. Over the last decade, a great deal of interest has arisen towards the creation of synthetic bistable genetic systems for use as memories, decision making circuits or sustained response devices [7–9]. Many studies have focused on understanding and improving these systems, and creating proper design rules for building synthetic bistable switches and modifying existing systems [10–13].
The most basic bistable switch is a single positive feedback loop. Bistable switches consisting of a single positive feedback loop are rarely observed in nature. The first synthetic bistable genetic switch was a single positive feedback loop constructed with a pair of co-antagonistic repressors . Even in the absence of cooperativity, a single positive feedback loop containing a transcriptional activator and its cognate promoter can exhibit bistable behavior due to transcriptional nonlinearity from cell growth ; employing variations resulting from cell growth, however, has proven difficult to exploit. Both natural and synthetic systems often contain multiple feedback loops for added control and robustness [10, 11, 16].
Protein degradation rates have also been mentioned to be critical in the operation of bistable and bimodal networks ; bimodal gene expression can result simply from changing protein degradation rates [18, 19]. The Vibrio fisheri quorum sensing system is an example from nature that uses nonlinear degradation to create a bistable system. Here nonlinear degradation is achieved through cooperative stability, where proteins are protected against degradation by protein multimerization. The positive transcription factor LuxR turns on the lux promoter, producing more LuxR. LuxR as a monomer is unstable and has a fast degradation rate. The LuxR monomer does not accumulate to high concentrations and also cannot activate the lux promoter. In the presence of the autoinducer AHL, LuxR dimerizes into a stable and slow-degrading complex. The LuxR-AHL complex is highly stable, is able to accumulate to a high concentration and is also able to activate the lux promoter. Varying the levels of AHL can switch the lux promoter between “on” and “off” states. Unfortunately, creating a synthetic bistable system utilizing cooperative stability is difficult, requiring protein engineering to create synthetic proteins with cooperative stability.
Nonlinear degradation conditions can also be achieved through dynamic protein degradation. Dynamic protein degradation has been observed in Xenopus, and is responsible for cell cycle progression. The concentration of Cdc2-cyclin B increases during interphase, but abruptly drops during mitosis. The accumulation of Cdc2-cyclin B actives the anaphase promoting complex (APC), and the APC inactivates Cdc2-cyclin B through proteolysis. A mitotic oscillator is observed in Xenopus during the early embryonic cell cycle , by taking advantage of dynamic degradation of Cdc2-cyclin B.
All reported synthetic bistable switches implemented in prokaryotes exclusively use transcriptional components (i.e. transcriptional activators, repressors and their cognate promoters). However, bistable systems can, in principle, be constructed from diverse components and their interactions: transcriptional elements, enzymes, transport proteins, metabolic pathways, ligand binding, etc. A recent report compared bistable switches constructed with enzymatic feedback loops, feedback loops constructed from only transcriptional components and hybrid transcriptional/enzymatic switches . It was found that enzyme-only circuits and hybrid transcriptional/enzymatic circuits showed bistable behavior for a wider parameter range than transcription-only circuits. This implies that hybrid bistable systems would likely be easier to tune and be more robust than systems built only from existing transcriptional components. In natural prokaryotic systems, the lac operon is arguably the most well-studied hybrid transcriptional/enzymatic bistable switch [21–23]. This system incorporates a lactose permease, enzymatic reactions, and transcriptional regulation. Once again, another well-studied hybrid bistable system is the lux operon in Vibrio fischeri, which uses an enzymatic reaction to convert a small molecule into an autoinducer to trigger transcriptional activation.
In this paper, we demonstrate a tunable family of hybrid bistable switches in E. coli using both transcriptional components and an enzymatic component (protease). We utilize standard transcriptional components to create a positive feedback loop. The behavior of the positive feedback loop, which normally does not show bistable behavior, is changed to a bistable network by adding a second feedback loop incorporating the Lon protease found in Mesoplasma florum (mf-Lon). To our knowledge, this work demonstrates the first use of mf-Lon to tune a nonlinear protein degradation circuit.
Other methods for engineering dynamic protein degradation exist but have disadvantages. In E. coli, knocking out the proteins ClpX and ClpP for dynamic expression compromises the fitness of knockout strains . B. subtilis has a similar ssrA system as E. coli and utilizes the same ssrA tags. Dynamic degradation of tagged proteins is possible in B. subtilis by using a mutated ssrA tag and dynamic expression of the E. coli gene, ssbP. Proteins tagged with the mutated ssrA tag will only be degraded when ssbP is expressed. This method is plausible for organisms utilizing a native ssrA system similar to E. coli but missing the ssbP gene. Unfortunately, these conditions are difficult to meet, and may only be possible with B. subtilis. The use of a completely orthogonal tagging and degradation system, such as utilizing mf-Lon in E. coli, is thus superior to previously mentioned methods for engineering dynamic degradation of protein.
The switch is a hybrid of transcriptional components and enzymatic degradation (Figure 1a). It is comprised of two positive feedback loops: a positive auto-regulating loop and a loop with two antagonistic interactions (Figure 1b). Our positive auto-regulating loop is identical to one found in λ phage. The promoter P RM expresses the λ repressor CI. CI is a transcriptional activator of P RM , thus producing positive feedback. The second positive feedback loop uses the tetracycline repressor (TetR) and mf-Lon. TetR is expressed bicistronically with CI in the P RM -CI loop. CI in the autoregulated loop is tagged with mf-ssrA (CI-mf-ssrA), allowing for fast degradation in the presence of mf-Lon. P LtetO-1 promoter  controls mf-Lon production. TetR is a repressor of P LtetO-1 and can stop mf-Lon expression, thus creating the co-antagonistic interaction; mf-Lon expression shuts off CI and TetR expression, while CI and TetR expression shuts off mf- Lon expression.
List of Plasmids (accession numbers are listed in the supplemental section S.5)
GFP reporter expressed from P RM
GFP reporter expressed from P LtetO-1
IPTG inducible CI-wt
IPTG inducible CI-ec- ssrA
IPTG inducible CI-mf-ssrA
P LtetO-1 mf-lon (trunc) mCherry with RBS1
P LtetO-1 mf-lon (trunc) mCherry with RBS2
P LtetO-1 mf-lon (trunc) mCherry with RBS3
P LtetO-1 mf-lon (trunc) mCherry with RBS4
P LtetO-1 mf-lon (trunc) mCherry with RBS5
P LtetO-1 mf-lon (trunc) mCherry with RBS6
P LtetO-1 mf-lon (trunc) mCherry with RBS7
Full switch with 5-UTR1
Full switch with 5-UTR2
Full switch with 5-UTR3
Full switch with 5-UTR4
Full switch with 5-UTR5
Full switch with 5-UTR6
Full switch with 5-UTR7
CI-wt and TetR expressed from P RM
CI-ec-ssrA and TetR expressed from P RM
CI-mf-ssrA and TetR expressed from P RM
IPTG inducible mf-Lon
The use of TetR allows for induction using anhydrous tetracycline (aTc). When TetR is bound by aTc, TetR is rendered inactive and can no longer repress P LtetO-1 and results in mf- Lon expression. This causes CI degradation and forces the switch into the “off” state. CI expression can be forced with IPTG induction using a separate inducible plasmid (PLlacO-1-CImf). Inducing with IPTG forces the switch into the “on” state. Some previous systems incorporating CI in bistable networks invoked the SOS response to degrade CI to either flip states or reset the network as CI is quickly degraded through RecA mediated degradation [14, 32]. Unfortunately, methods evoking the SOS response such as heat shock  or UV exposure  may be detrimental to cultures. Our system of utilizing mf-Lon allows for fast degradation of CI without evoking the SOS response.
CI also acts as a negative autoregulator at high concentrations  (Figure 1c). P RM is half of a bidirectional promoter (Figure 1c) in λ phage. The complete promoter consists of three binding sites, OR1, OR2 and OR3. CI preferentially binds to OR1 and OR2, repressing the constitutive promoter, P R . In high concentrations, CI binds to OR3 and acts as a repressor to P RM . We used a mutated OR3 , in order to prevent autorepression.
The complete switch was constructed on a plasmid with a pSC101 origin and a kanamycin marker (Figure 1d). Both TetR and mf-Lon were tagged with a fast degradation ec-ssrA tag to allow for fast turnover rates for the proteins. P LtetO-1 has been placed serially next to P R without separation by a terminator. It is unnecessary to use a terminator between these two promoters, because when the switch is in the “on” state, CI and TetR represses both P R and P LtetO-1 , respectively, and mf-Lon production is stopped. When the switch is in the “off” state both P R and P LtetO-1 are not blocked and mf-Lon production is resumed. The serial placement of P LtetO-1 and P R should not affect the basic principles governing the design of our switch.
A rate-balance plot  highlights the important differences between a fully transcriptional bistable switch (TS) (Supplemental Information S.1.5), and the hybrid transcriptional-enzymatic switch (TES) (Figure 1e). Both a TS and a TES use two linked positive feedback loops. The difference between the two topologies lies in the second positive feedback loop. In the TS, the second positive feedback loop uses two repressors. In the TES, the second positive feedback loop uses a repressor and a protease. The solid line on the rate balance plot (Figure 1e), represents the transcriptional activator production rate and the dashed curves represents the transcriptional activator degradation rate. A monostable system contains only one stable steady-state, represented by one intersection between the protein production and degradation curves. A bistable system requires two stable steady states (closed circles) and one unstable steady state (open circle), for a total of three intersections. In the “classic” TS, the addition of a second positive feedback loop adds nonlinearity to the CI production curve, resulting in a higher apparent Hill coefficient in the CI production curve (Additional file 1: S.1.5). Degradation rates for CI remain the same without the extra feedback loop and the degradation curve remains completely linear. In the TES, the addition of the second positive feedback loop, which contains the protease, changes the protein degradation from linear (dotted-dash line) to nonlinear (dashed line) while the CI production curve (solid line) remains unchanged (Figure 1e). The rate-balance plots show two different paradigms for creating bistable switches. One paradigm adds nonlinearity to activator production (TS), while the other adds nonlinearity to the activator degradation (TES).
Conceptually, TES topologies have the benefit of a larger bistable parameter space, allowing for increased robustness and easier parameter tuning . Furthermore, enzymatic reactions have faster response times compared to transcriptional interactions. Enzymatic reactions directly deactivate proteins, by dephosphorylation, proteolysis, etc. In TS topologies, protein removal is also required to flip state after the deactivation of a promoter; this usually occurs through dilution by cell division or targeted protein degradation (e.g. ssrA tags). Increasing the rate of protein degradation in TS topologies allows for faster switching speeds, however, this further limits the already narrow parameter space of TS topologies.
Synthetic TS have been dominant in prokaryotic systems. This is likely due to the higher modularity and orthogonality that transcriptional parts have relative to enzymatic parts. Interconnections between transcriptional devices (a transcription factor and its cognate promoter) are simply created by adjacent placement in the DNA sequence of a regulated promoter and a transcription factor from two transcriptional devices. This allows for virtually any transcriptional device to serve as an input or output to any other transcriptional device. This contrasts with creating interconnections to inputs and outputs of enzymatic steps, where a common molecule is required and generally this need for a shared molecule greatly limits the number of parts an enzyme can be connected to. Moreover, many of the characterized enzymes are responsible for global housekeeping or are involved in metabolic pathways, limiting the applicability of any prokaryotic TES system relying on these enzymes. Proteases that are targeted to proteins with specific terminal sequences are not as constrained as other enzymes with respect to their modularity, as this class of proteases are not restricted to a single substrate, but can be used with any protein that will retain activity with the addition of the protease targeting signal.
First, it is necessary to check that the addition of the mf-ssrA tag onto the C-terminus of CI does not interfere with activation of P RM by CI. The N-terminal domain of CI contains a DNA binding domain, and the C-terminal domain includes a dimerization domain . CI first dimerizes and then binds onto OR1 and OR2 to activate P RM and repress P R . Under normal physiological expression levels of CI the C-terminal domain is necessary for dimerization. Dimerization in turns helps with DNA binding. When using CI with a truncated C-terminal domain, higher concentrations of CI are necessary for dimerization to occur and thus higher CI concentration is necessary for DNA binding . The addition of a degradation tag may interfere with proper protein interactions, and thus needs to be tested.
As stated above, the activity of P RM is not monotonic with CI concentration; above a threshold concentration of CI the activity of P RM decreases with increasing CI. However, even for the P RM promoter with mutated OR3 operator site, all three CI variants showed slight repression of P RM at high levels of CI. CI-wt showed the highest degree of repression.
These results show the ability for CI-mf-ssrA to activate P RM , and thereby CI-mf-ssrA is usable for the proposed the TES. The results also show CI-mf-ssrA behavior slightly deviates from wild-type function; this will be discussed below.
The P RM -CI positive feedback loop was functional using all three variants of CI (Figure 3b). All three CI variants, in the positive feedback loop configuration, showed strong levels of GFP expression (reporting with PRM-GFP). Expression of mf-Lon was only able to degrade CI-mf-ssrA and thus turn “off” the P RM -CI loop, resulting in greatly decreased GFP production. CI-wt and CI-ec-ssrA could not be degraded by mf- Lon and the GFP production did not change as drastically. This shows mf- Lon specificity to its cognate ssrA tag. In both the CI-wt and CI-ec-ssrA circuits, when IPTG addition was added, the P RM -CI loop remained “on,” however there was a measurable decrease in GFP expression. The decrease in GFP expression can probably be attributed to the increased metabolic burden from the expression of mf-Lon on a plasmid with a ColE1 origin of replication.
The PLtetO-1-GFP reporter tested TetR production level. TetR is biscistronically expressed with CI and the concentration of TetR should be approximately proportional to CI concentrations. When using the PLtetO-1GFP reporter, GFP expression increased only in the PRM-CImf-TetR test circuit (Figure 3c). This result again confirmed the specificity of mf- Lon to the mf-ssrA tag. GFP expression decreased with mf-Lon induction from test circuits expressing CI-wt and CI-ec-ssrA (Figure 3c). Once again, the decrease in GFP expression is likely due to increased metabolic load from mf-Lon induction.
The addition of aTc showed high GFP expression levels in all three experimental strains containing the three variants of CI (reporting with PLtetO-1-GFP). The addition of aTc inactivates TetR and P LtetO-1 becomes fully active regardless of mf-Lon or CI expression. Even when the PRM-CI positive feedback loop was shut “off” (resulting from CI-mf-ssrA degradation by mf-Lon), there was always basal TetR expression, which kept P LtetO-1 partially off. Only when aTc was added would P LtetO-1 become fully active. It is important to keep in mind that in these test circuits the TetR expression level is always high enough to have measurable effect on P LtetO-1 regardless of the P RM -CI state.
From these experiments we concluded that CI-mf-ssrA could indeed be degraded by mf- Lon. Just as important, mf- Lon specifically degrades proteins tagged with mf- ssrA and does not degrade proteins tagged with ec-ssrA.
Switch behavior (in the absence of inducers)
SW7 was assayed using with the PRM-GFP reporter plasmid and showed monostable behavior; the switch was always off unless high levels of IPTG were used to induce high levels of CI production (Figure 5c).
Activation deactivation times for 3 biological replicates
Activation was dependent on CI accumulation rate. To first order, the CI accumulation rate is dependent on CI production rate. All strains had the same inducible CI plasmid, and identical P RM -CI positive feedback loops. As a result, all three switches should have the same CI production rates. As observed, ACT½ for all three strains did not differ by much (as compared to DCT½). Protein degradation rate is dependent on protease concentration, giving the expected results for deactivation time. Once again when we reported SW4, SW5 and SW6 with PLtetO-1-GFP (Figure 8c and d), no hysteresis was observed. The curves in the “on” state or “off” state are identical.
Given the fast deactivation of SW6, the dynamic measurements of SW6 were repeated using flow cytometry (Supplemental Information S.3.1) to ensure that the “on” state and “off” state were each composed of a unimodal distribution of cells in that state. The flow cytometry data confirms that each state contains a unimodal distribution of cells.
We present a new bistable topology in E. coli. Our system specifically uses an ssrA degradation system orthogonal to the native E. coli system. The usage of the mf- Lon protease and mf- ssrA tag in a useful circuit had not previously been explored. The usage of nonlinear protein degradation in a bistable switch has mainly been a theoretical discussion and has not been synthetically employed. In this paper we experimentally tested the effect of using nonlinear protein degradation in a synthetic prokaryotic system.
We found that CI-wt activates P RM the most strongly as compared to CI with ssrA tags (Figure 2b). It is known that the CI dimer is extremely stable and has a long half-life ; even with low expression rates CI-wt can quickly accumulate and activate P RM . The mf- ssrA tag should be completely orthogonal to the ec-ssrA tag . In E. coli, the half-life of proteins tagged with mf-ssrA should be unaffected since they will not be targeted for degradation. We report that CI-mf-ssrA has a different behavior than CI-wt. CI-mf-ssrA requires a higher expression rate to activate P RM compared to CI-wt. It requires a higher expression rate than even CI-ec-ssrA. This implies that CI-mf-ssrA is intrinsically unstable and degrades quickly, even when it is not targeted for degradation. Most likely the addition of 27 aa ssrA tag interferes with the C-terminal domain of the lambda repressor, as opposed to the 13 aa ec-ssrA tag. The mf-ssrA tag disrupts the C-terminal domain dimerization of CI, requiring a higher concentration of CI for dimerization. Furthermore, CI dimers are cooperatively stabilized. Unless there are high expression levels of CI, few CI dimers are formed and the unstable CI monomers are quickly degraded . Since mf- ssrA can interfere with protein functionality, this implies that the number of proteins that can be used with the mf- ssrA degradation system may be limited.
Enzyme substrate reaction rates are dependent on both the concentration of the enzyme and the substrate. The maximum reaction rate, Vmax, is directly proportional to enzyme concentrations. If switching speeds need to be modified, adjusting protease expression levels provides an easy way to tune the switching speed. In our reported TES, changing protease expression levels only changed the deactivation speed. The activation speed is most likely controlled by changing the CI expression rate on the PLlacO-1-CImf plasmid (this was not explicitly tested).
It should be noted that on TS, changing the expression levels of transcriptional activators and repressors does not change the activation and deactivation speeds significantly, because protein degradation is the limiting factor and is unchanged by protein expression rates. The addition of degradation tags in a TS may not be an option due to parameter constraints. In our TES, protein degradation is not a limiting factor, because proteins are either tagged with a fast degradation tag or dynamically degraded by a protease, which allows for flexibility in changing activation and deactivation speeds.
The TES topology presented can be rendered modular by using two input promoters. One promoter would express CI and the other would express mf-Lon. In this scheme DCT½ would depend on both the expression rate of mf- Lon from the linking circuit as well as the expression rate on the switch itself. Depending on relative rates within the switch and on the input, the faster rate would dominate the other. The switching “on” rate would be dominated by CI production rate on the input circuit.
Both the hysteresis data and transient behavior data confirmed the lack of hysteresis from P LtetO-1 . When using the PLtetO-1-GFP reporter, flow cytometry experiments showed that in the absence of inducers, cells in either the “on” or “off” state had identical GFP expression levels (Additional file 1: S.3.3). With the addition of aTc we observed high levels of GFP expression in a tightly distributed unimodal population (Additional file 1: S.3.2). When IPTG was added, there appeared to be a bimodal population of cells; one population did not express GFP, the other population expressed low levels of GFP. The bimodal population of cells implied that TetR did not completely repress PLtetO-1. However, TetR production was clearly high enough to prevent a fully active P LtetO-1 promoter. We saw that even when the switch was “off,” there was enough TetR expression to keep P LtetO-1 partially off and only with the addition of aTc would P LtetO-1 be fully active. It is unknown why the addition of IPTG was unable to completely shut off P LtetO-1 .
One last observation is that the observed lack of hysteresis in mf-Lon concentration may make it unnecessary to add a second positive feedback loop to create a bistable network. Instead, bistable behavior may be possible using only a single positive feedback loop along with constitutive expression of mf-Lon. The simplified circuit would consist of a P RM -CI positive feedback back loop, with CI tagged with mf-ssrA. The expression level of mf-Lon would determine the degradation rate of CI-mf- ssrA (Supplemental Information S.4.3). Using the literature values of the reported Michaelis constant for mf-Lon (Km)  and the literature value for the dissociation constant of CI-wt to P RM binding (KdCI) , bistable behavior cannot be obtained with a single positive feedback loop. Using modified Km where K dCI >K m , bistability is analytically observed using a rate balance plot (Additional file 1: S.4.4).
The literature value for K m may be inaccurate, since Km was measured in vitro. The in vivo value may actually be lower value than the measured in vitro K m value. The native function of mf-Lon is to rescue stalled transcription events. With a high K m , stalled events cannot be rescued efficiently. Natively, mf-Lon is a housekeeping gene, and expression of the protease is probably low. The in vivo functioning of mf-Lon is most likely fast and efficient, even at low protease concentrations. In order to create the bistable rate-balance plot, K m needs to be decreased by three orders of magnitude, and this shift in value is also highly doubtful. The lack of hysteresis for P LtetO-1 and its implications require more tests to be fully understood.
The principal benefit of the protein degradative interaction in the TES is the tunability of switching speeds due to active removal of proteins through a protease. In the TS, removal of proteins is through dilution by cell division. The original toggle  switch required 3–4 hrs for to begin switching, and over 5 hours for the switch to completely change states. Switching states in the linked double positive feedback loop reported by Chang et al. required the dilution of both proteins and the small molecule IPTG. In this case switching required a 1 million-fold cell dilution for proper switching. With active protein removal through a protease we were able to complete switching in approximately 3 cell divisions (~2.5 hr). In theory, switching could be accomplished within one cell division. This would require the simultaneous tuning of the RBS for all three proteins (CI, TetR and mf-Lon) to optimize deactivation time.
Another benefit of our TES compared to a TS is the increased robustness of the TES. It has been previously shown that these types of hybrid circuits are more robust than transcription-only circuits . Adding a protease introduces nonlinear degradation and thereby adds nonlinearity into the system. In classic TS systems, some nonlinearity can be added by increasing the apparent cooperativity in the main positive feedback loop. Additionally, it is difficult to add ec-ssrA tags in the TS, since the parameter space is already very small. Shortening the protein lifetime also decreases the robustness of the circuit. In the TES, the parameter space was broad enough to allow for the addition of ec-ssrA tags. It can be argued that increased bistable parameter space contributes to the tunability of switching time.
We have demonstrated a hybrid bistable switch using both transcriptional components and an enzyme. Bistable behavior is achieved through nonlinear degradation of the transcriptional activator. A dynamically expressed ssrA protease orthogonal to the E. coli system was used in order to achieve nonlinear protein degradation. Use of a protease allows for an easy way to tune switching speed in bistable circuits. This is a new method of creating synthetic bistable networks, which have been theoretically proposed, but have not been tried experimentally.
Cloning steps and experiments were performed with E. coli strain DH10B. Overnight cultures were performed in Luria-Bertani (LB) medium at 37°C. All experiments were performed in EZ-rich media with 1% glucose, purchased from Teknova and were grown at 37°C. Antibiotics were used with the following concentrations: kanamycin at 40 μg/mL, chloramphenicol at 20 μg/mL, ampicillin at 100 μg/mL, carbenicillin at 100 μg/mL. Experiments used carbenicillin in lieu of ampicillin. Cloning steps used ampicillin instead of carbenicillin. Restriction enzymes were purchased from Fermentas Inc. Polymerases were purchased from Finnzymes and Stratagene. Media, antibiotics and enzymes were used according to manufacturer recommendations.
Table 1 lists all the plasmids used in this study. All cloning plasmids in this study have the BglII/BamHI BglBrick sites . Ribosome binding sites (RBS) were added using ‘Round-the-horn site directed mutagenesis (RTH) and its respective primers . RBS were designed using the RBS calculator. IPTG inducible plasmids with Cm marker were constructed by inserting the respective genes into BglBrick sites using the XhoI and BglII restriction sites. Mf-ssrA and ec-ssrA tags (AANDENYALVA)  were added using RTH and its respective primers. CI-ec-ssrA, sfGFP, TetR and mf-Lon were destabilized with the addition of a ec-ssrA tag.
Mf-lon was obtained from Addgene (Plasmid 21867: pBAD33-mf-lon) . The sequence was amplified with PCR adding BglBrick sites then added into a high copy cloning plasmid with pUC19 origin of replication and ampicillin marker. Superfolder GFP (sfGFP) is the same as described by Pedelacq et al.. The RFP, mCherry, is described by Shaner et al..
Endpoint measurements started with a 5 mL LB overnight culturing with 200 rpm of continuous shaking. After overnight culturing each sample was subcultured with a 100 fold dilution into 5 mL of EZ-rich media and regrown to an OD600 of 0.4. The cultures were then subcultured into EZ-rich media to an OD of 0.05 with added inducers. Florescence measurements were measured by transferring 150μL of culture into a 96 well microplate to measure OD600 and fluorescence on a Molecular Devices Spectramax M2. GFP measurements used 485 nm for excitation and 538 nm for emission. RFP measurements used 584 nm for excitation and 612 nm for emission. All fluorescence measurements were normalized to OD600. All reported measurements were repeated in triplicate by using three different colonies.
A single colony was picked out a plate transformed with the relevant plasmids and cultured overnight in both 5 mL LB with IPTG (.0625 mM) and 5 mL LB with saturating aTc (100 ng/mL) to force them into the high and low state respectively. Generally 1 mM of IPTG was used for saturating conditions. We found that reduced levels of IPTG were sufficient to induce high levels of CI and push switches into the “on” state. The reduced levels of IPTG also allowed for easier removal of IPTG. The overnight cultures were washed three times with EZ-rich media and split into multiple subcultures on a 96 deep well plate. Each subculture was grown with a total of 1 mL of media and the plate was shaken at 250 rpm. More specifically each overnight sample was subcultured into 7 different IPTG conditions (ranging from 0 mM to .25 mM) and 7 different aTc conditions (ranging from 0 ng/mL to 100 ng/mL). After cell growth reached mid-log (~8 hrs), each sample on the 96 well plate was recultured on a new 96 well plate with fresh media using exactly the same inducer concentrations as the previous 96 well plate. This step ensured complete removal of the initial inducer. After the samples reached mid-log again, GFP output was measured. For each switch, GFP output was measured for both PLtetO-1-GFP and PRM-GFP reporters. Each data point was replicated three times using three individual bacterial colonies.
The long term stability test was performed only on SW4 with the PRM-GFP reporter. SW4 was grown in 5 mL LB overnight with saturating IPTG (.0625 mM). The overnight culture was washed three times and recultured in fresh EZ-medium using a 1000 fold dilution. After an OD600 of 0.5 was reached the culture was then split into two subcultures. Both were cultured with 1000 fold dilutions. One culture had 100 ng/mL of aTc added in order to switch in to the “off” state. The other culture was grown without aTc. After 8 hr of growth, both samples were washed and subcultured in fresh media without any inducer, again with a 1000 fold dilution. Both samples were grown an additional 32 hr, washing and subculturing every 8 hr, again using 1000 fold dilutions. GFP measurements are taken every eight hours before each subculturing event. The doubling time was approximately 45 minutes, giving approximately 10 doubling every 8 hr. The total experiment had 40 doublings throughout the stability measurement. Each data point was repeated three times using three separate colonies.
Transient measurements started with overnight cultures in 5 mL LB. One colony was picked from an agar plate to inoculate two 5 mL LB culture tubes. One culture tube had 100 ng/mL of aTc, and the other tube had 0.0625 mM of IPTG. After overnight growth (16 hr), the overnight cultures were washed three times in EZ-rich media and subcultured with 1000 fold dilution in EZ-rich media and regrown to an OD600 of approximately 0.8. Each culture was split into three separate subcultures each with a different inducer (0.25 mM IPTG, 100 ng/mL aTc, and no inducer) and diluted down to an OD600 of 0.05. The three different inducer conditions represent three transient conditions (change, reinforce, and persist). “Change” is when an inducer is added to alter the state. “Reinforce” is when the inducer used is the same as the overnight inducer. “Persist” is when no inducer is added and switches are allowed to keep their prior state. Fluorescence measurements were taken every 30 minutes. Measurements were all performed in triplicate using three separate colonies. GFP expression was reported using both reporters.
To measure 50% activation (ACT½), we measured the time it took for a strain, initially in the “off” state, to reach 50% of maximum GFP expression. Because the baseline “on” and “off” GFP expression changes over time as OD increases, the 50% level also changes with OD. The 50% level is found by taking the average value between the “on persist state” and “off persist state” for each time point. The 50% deactivation (DCT½) level is found in a similar fashion as the 50% activation calculation. ACT½ and DCT½ were only measured using PRM-GFP. ACT½ and DCT½ were measured three times using three separate colonies.
Cultures to be measured were diluted 1:2000 in phosphate buffered saline (from Teknova) with 50 μg/mL of streptomycin. 150 mL of the diluted sample was placed in a 96 well microplate, and then measured on a Milipore guava easyCyte HT. For each sample approximately 2000 events were counted.
DH and WH conceived of the experiments. DH performed the experiments. DH, WH and MM wrote the manuscript. All authors read and approved the final manuscript.
We would like to thank Justin Hsia and Murat Arcak for help with the analytical modeling and for comments on the manuscript. We would also like to thank Colin Lam for help with the flow cytometry data collection. Furthermore special thanks to the Joint Bioenergy Institute support staff for helping to make all experiment run faster and smoother. The funding for this work was provided by the Synthetic Biology Engineering Research Center (SynBERC), grant number 0540879, and by an NSF CAREER grant to M.M.M., grant number ECCS 0846618.
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