Small RNAs OmrA and OmrB promote class III flagellar gene expression by inhibiting the synthesis of anti-Sigma factor FlgM

ABSTRACT

Bacteria can move by a variety of mechanisms, the best understood being flagella-mediated motility. Flagellar genes are organized in a three-tiered cascade allowing for temporally regulated expression that involves both transcriptional and post-transcriptional control. The class I operon encodes the master regulator FlhDC that drives class II gene transcription. Class II genes include fliA and flgM, which encode the Sigma factor σ²⁸, required for class III transcription, and the anti-Sigma factor FlgM, which inhibits σ²⁸ activity, respectively. The flhDC mRNA is regulated by several small regulatory RNAs (sRNAs). Two of these, the sequence-related OmrA and OmrB RNAs, inhibit FlhD synthesis. Here, we report on a second layer of sRNA-mediated control downstream of FhlDC in the flagella pathway. By mutational analysis, we confirm that a predicted interaction between the conserved 5ʹ seed sequences of OmrA/B and the early coding sequence in flgM mRNA reduces FlgM expression. Regulation is dependent on the global RNA-binding protein Hfq. In vitro experiments support a canonical mechanism: binding of OmrA/B prevents ribosome loading and decreases FlgM protein synthesis. Simultaneous inhibition of both FlhD and FlgM synthesis by OmrA/B complicated an assessment of how regulation of FlgM alone impacts class III gene transcription. Using a combinatorial mutation strategy, we were able to uncouple these two targets and demonstrate that OmrA/B-dependent inhibition of FlgM synthesis liberates σ²⁸ to ultimately promote higher expression of the class III flagellin gene fliC.

Introduction

Bacteria are masters of rapid adaptation to changing environmental conditions. For instance, enterobacteria such as Escherichia coli and Salmonella enterica change their lifestyle in response to, e.g. nutritional status to enter a sessile (biofilm) or motile (flagellated) state. These states are generally considered mutually exclusive, which is reflected by complex layers of transcriptional control that promote the establishment of one state while simultaneously prohibiting the other [1–3]. In these decisions, the transcriptional activators FlhDC and CsgD are the master regulators of flagellar and biofilm (curli/cellulose) genes, respectively (Figure 1). Transcriptional control is additionally modulated by the levels of the second messenger cyclic-di-GMP, determined by the opposing activities of diguanylate cyclases (DGCs) and phosphodiesterases (PDEs), and by upstream acting transcription factors (TFs) such as MlrA, OmpR, and the stress/stationary Sigma factor σ^S (for reviews on these topics, see: [2,4-7]). On top of transcriptional control, a second, post-transcriptional level involves a large suite of small RNAs/sRNAs (OmrA, OmrB, McaS, RprA, GcvB, RydC, ArcZ, and OxyS) that, via direct regulation of FlhDC and CsgD, affect biofilm and/or flagellar gene regulation [8–14].

Figure 1.

Effects of OmrA and OmrB in the regulatory networks for motile and sessile lifestyles in E. coli.

In the biofilm pathway, OmrA/B target three genes, csgD, ompR, and dgcM (Figure 1) [10,15–17]. CsgD is the TF responsible for activating csgA and csgB, encoding the structural proteins of curli fibers. OmpR is the response regulator of the two-component system EnvZ/OmpR, induced under osmotic stress, and a direct activator of csgD expression [18,19]. OmpR also activates transcription of omrA/B, thereby forming a negative feedback loop [16]. DgcM is a DGC that activates the TF MrlA [20], which in turn activates transcription of csgD. Though the same sequence motif in the 5ʹ tails of the sRNAs is used for base-pairing to all mRNA targets, the molecular mechanisms of control differ. Canonical translational inhibition works on ompR mRNA, where sRNAs compete against initiating ribosomes [16]. On csgD mRNA, both sRNAs bind far upstream of the ribosome binding site (RBS) to prevent translation initiation by an as yet unknown mechanism [10,21]. Regulation of dgcM mRNA involves Hfq-dependent structure remodelling to facilitate OmrA/B binding, rather than the more common matchmaking activity of this protein [17]. Ultimately, downregulation of these three genes entails inhibition of both curli formation and synthesis of cellulose. Thus, OmrA and OmrB are negative factors for a sessile lifestyle. However, both sRNAs can also inhibit motility by repressing translation of FlhD, the activator of the flagellar gene cascade [9]. This suggests a complex post-transcriptional pattern of regulation potentially affecting both a sessile and a motile lifestyle. In addition, these sRNAs inhibit expression of outer membrane proteins [15,16,22,23]. Thus, OmrA/B-dependent targeting of multiple mRNAs connects various regulatory networks to coordinate bacterial physiology and behaviour.

The bacterial flagellum is a complex organelle that requires coordinated temporal expression of more than 60 genes in multiple operons [24–26]. These genes are organized in a hierarchical cascade (class I–III), with several checkpoints to ensure that flagellar components are expressed and assembled sequentially [24,27,28]. The flhDC operon is at the top of this cascade and encodes the hetero-multimeric activator FlhD₄C₂ that drives σ⁷⁰-dependent transcription of class II genes [29]. Expression of flhDC is tightly controlled at the transcriptional level by more than 10 TFs, and post-transcriptionally by several sRNAs and RNA-binding proteins [2,9,14,26]. Class II gene expression entails assembly of the flagellar motor, often referred to as the hook basal body (HBB). Class III genes are activated by the class II-encoded flagellar Sigma factor, σ²⁸ (encoded by fliA), which initially is neutralized by the anti-Sigma factor FlgM [30] (Figure 1). Upon HBB completion, which results in FlgM secretion [31,32], the liberated σ²⁸ activates transcription of the class III genes, including fliC that forms the flagellar filament [24]. σ²⁸ activity is also linked to FlgM-mediated proteolysis control; FlgM binding not only inhibits σ²⁸ activity but also protects it from degradation by the Lon protease [33]. Degradation of free σ²⁸, once the HBB is complete and FlgM secreted, ensures that class III gene expression is restricted in time to prevent the aberrant formation of flagellar filaments [24].

Despite the extensive study of bacterial motility, the flagellar pathway still holds surprises. By now, post-transcriptional control mediated by sRNAs is known to complement transcriptional regulation of both flagellar and biofilm genes. In the present study, we identified the anti-Sigma factor-encoding flgM mRNA as yet another sRNA target (Figure 1). By translational inhibition of flgM mRNA, OmrA and OmrB help to promote class III flagellar gene expression.

Results

OmrA and OmrB directly inhibit FlgM synthesis by an Hfq-dependent antisense mechanism

Since sRNAs often target several genes in the same pathway [34,35], we hypothesized that OmrA/B may, in addition to flhDC, target other motility-associated mRNAs. Indeed, the IntaRNA algorithm [36,37] predicted base–pair interactions between OmrA/B and the flgM mRNA; the 5ʹ region of OmrA is complementary to the sequence encompassing codons four to nine of the flgM open reading frame (ORF), with codons one to nine matching OmrB (Figure 2(a)).

Figure 2.

OmrA and OmrB cause direct translational inhibition of flgM mRNA in vivo.

To assess whether OmrA/B affect flgM expression in vivo, we measured fluorescence of cells harbouring a plasmid encoding a flgM::gfp translational fusion in the presence or absence of either of the sRNAs; expression is driven by P_LTet0-1 [38] followed by nucleotides +1 to 105 of flgM (relative to transcription start site) joined in frame with gfp after the first 23 codons of FlgM. Congruent with the predicted antisense interaction, overexpression of OmrA or OmrB resulted in five-fold reduced fluorescence, indicating strong repression of FlgM synthesis (Figure 2(b)). Introduction of a single point mutation (M1; Figure 2(a)) in the predicted interaction site in OmrA, OmrB, or flgM mRNA, reduced OmrA/OmrB-mediated repression (Figure 2(b)). Compensatory mutations designed to re-establish OmrA/B base-pairing with the flgM mRNA indeed restored regulation (Figure 2). The position of the OmrA/B target site in the flgM mRNA is further supported by in vitro footprinting experiments (Fig. S1). Taken together, these results strongly indicate that OmrA and OmrB inhibit FlgM synthesis by binding to the early coding region of the flgM mRNA.

The RNA chaperone Hfq is required for the regulatory activity of most trans-encoded sRNAs in enterobacteria [35,39]. Hfq stabilizes sRNAs (e.g. OmrA and OmrB levels are strongly reduced in absence of Hfq [10]), but also acts as a matchmaker platform to promote sRNA–mRNA interaction [35,39–42]. To investigate whether regulation of flgM by OmrA and OmrB requires Hfq, a ∆hfq strain was transformed with the flgM::gfp translational fusion and OmrA/B-overexpressing vectors. As expected, the hfq deletion totally abolished the sRNA-mediated repression of flgM::gfp (Figure 2(c)), confirming that Hfq is required for regulation.

OmrA and OmrB inhibit FlgM translation by competing for ribosome binding

The binding of OmrA/OmrB close to the AUG start codon on flgM mRNA suggested that repression of FlgM synthesis involves inhibition of translation initiation [43]. We performed a toeprint analysis to evaluate whether formation of the 30S initiation complex (30S-IC) on flgM mRNA was affected by the sRNAs. As expected, the presence of both 30S and tRNA^fmet resulted in a reverse transcription stop 15 nucleotides downstream of the flgM start codon, indicative of stable 30S-IC formation [44,45] (Figure 3(a)). Addition of either OmrA or OmrB completely abolished the toeprint signal. This strong repression is specific; addition of the unrelated sRNA IstR1 [46,47] did not affect 30S-IC formation.

Figure 3.

Binding of OmrA and OmrB inhibit translation of flgM mRNA.

OmrA/OmrB-dependent inhibition of flgM translation was further validated using an in vitro translation assay. Translation rates of flgM-3xflag and ompA-3xflag mRNAs (the latter was an internal, non-target control) were monitored by Western blot using anti-FLAG antibodies. Uponaddition of OmrA or OmrB, the accumulation of the FlgM-3xFLAG protein decreased slightly, with OmrA being more effective than OmrB, as also seen on other targets [10] (Figure 3(b)). However, in the presence of Hfq, both sRNAs strongly repressed FlgM-3xFLAG synthesis.

Altogether, the in vitro data corroborate the in vivo results on flgM regulation by OmrA and OmrB, suggesting direct translational inhibition via sRNA base-pairing. Moreover, the stronger inhibition observed in the presence of Hfq suggests that, in the context of active translation, Hfq facilitates sRNA–mRNA interaction.

Mutations in OmrA abolish regulation of FlhD while supporting maintained FlgM control

OmrA/B inhibits synthesis of both FlhD [9] and FlgM (Figures 1–3). With respect to flagellar class II and class III genes, these regulations should have distinct effects (see Figure 4(a)). Inhibition of FlhD should reduce expression of class II genes and, indirectly via σ²⁸, of class III genes. In contrast, inhibition of FlgM should promote class III transcription by increasing the cellular concentration of active σ²⁸, but have little or no effect on class II genes [32,33]. To test this, we first investigated the effect of FlgM on class II and class III genes. The motile E. coli strain BW25113 and an isogenic strain carrying a flgM in-frame deletion were transformed with plasmids carrying transcriptional fusions between the promoters of fliE (class II) or fliC (class III) and gfp. As expected, the fliC promoter was strongly activated in the ∆flgM strain compared to wild type, whereas the absence of FlgM had no significant effect on fliE promoter activity (Figure 4(b), Fig. S2). These results are in line with previous reports showing that FlgM-mediated control of σ²⁸ specifically impacts class III genes [25,32].

Figure 4.

In-frame deletion of flgM affects class III (fliC) but not class II (fliE) flagellar gene expression.

Next, we sought to construct a regulatory circuit in which we could analyse the effects of OmrA/B-dependent regulation of FlgM, and its consequences for class III transcription, in the absence of OmrA/B’s effect on FlhD. We first tested how OmrA/B and mutants thereof affected the expression from a translational flhD::gfp fusion. While wild-type sRNAs and M1 mutant RNAs (see Figure 2(b)) repressed flhD::gfp expression, a second mutant variant, M2 (CC to GG mismatch at positions 2 and 3 of OmrA/B; Figure 5(a)), failed to do so (Figure 5(b), Fig. S3). Moreover, OmrA-mediated inhibition of FlhD translation was stronger than that of OmrB (Fig. S2). Since this paralleled the stronger OmrA effect on FlgM in the in vitro translation assay (Figure 3(b)), we focused on OmrA-mediated regulation of flagellar genes from now on. We monitored the effect of the same OmrA mutant RNAs, M1 and M2, on expression from the target site-mutated translational flgM_M1::gfp fusion. OmrA_M1 strongly repressed flgM_M1::gfp translation, while both the wild-type OmrA and the mutant OmrA_M2 maintained about two-fold repression (Figure 5(b)). Thus, a circuit in which flgM carries the M1 mutation, and OmrA carries the M2 mutation, allows uncoupling of the OmrA-dependent regulation of FlhD and FlgM (Figure 5(c)). This in turn enabled us to specifically monitor the consequences of OmrA-dependent regulation of FlgM alone on flagellar gene expression.

Figure 5.

Uncoupled regulation of flhD and flgM_M1 by mutant versions of OmrA.

Repression of FlgM synthesis by OmrA/B increases class III flagellar gene expression

To understand how OmrA/B-mediated regulation of flgM impacts class III gene expression, scarless mutagenesis was used to introduce the M1 mutation into the chromosomal flgM locus. Wild type, flgM_M1, and ∆flgM strains were transformed with the PfliC-gfp transcriptional fusion plasmid together with a plasmid constitutively expressing OmrA_M2, or an empty control plasmid. In strains carrying the control plasmid, absolute fluorescence levels were comparable between wild-type and flgM_M1, indicating that the silent M1 mutation neither affects FlgM expression nor activity whereas, in contrast, the ∆flgM strain exhibited increased fluorescence (Fig. S2). This is in agreement with Figure 4. Importantly, the strain carrying the flgM_M1 mutation and OmrA-M2 showed two-fold higher fluorescence, compared to the strain with the control plasmid. By contrast, neither the strain with wild-type flgM, nor the ∆flgM strain, exhibited OmrA_M2-dependent effects on the fliC reporter (Figure 6). Since flhD and flgM_M1 regulation is uncoupled in this background (Figure 5), and since FlgM and FlgM_M1 proteins are similarly active, we conclude that OmrA/B-mediated regulation of FlgM translation positively contributes to flagella expression, and/or its timing, independently of flhD post-transcriptional regulation by the same sRNAs.

Figure 6.

OmrA-mediated regulation of flgM promotes class III flagellar gene expression.

Discussion

In this report, we show that the E. coli sRNAs OmrA and OmrB negatively control the expression of the anti-Sigma factor FlgM. This frees up α²⁸, thereby indirectly promoting the expression of the flagellar class III genes. In vivo, overexpression of either sRNA decreased fluorescence from a translational flgM::gfp reporter, and mutational analysis, supports that regulation is Hfq-dependent, direct, and requires an anti-sense interaction between OmrA or OmrB and the flgM mRNA (Figures 1 and 2). Toeprint analysis and in vitro translation assays suggested sRNA binding-dependent canonical translational inhibition (Figure 3). As previously reported [32], deletion of flgM activates a fliC transcriptional fusion by approximately four-fold compared to that of a wild-type strain (Figure 5). To monitor the impact of OmrA on class III gene expression only via FlgM, uncoupling of its regulatory effect on flgM from that on flhD was required. The OmrA_M2 mutant RNA could no longer regulate flhD (Figure 5) but still repressed a flgM_M1 mutant mRNA, albeit at half the efficiency as that of a fully matched pair of RNAs. This experimental setup ensured that the master regulator FlhD₄C₂ was expressed and could initiate flagella synthesis even during constitutive OmrA_M2 expression. Hence, we could specifically monitor the effect of OmrA_M2-dependent regulation of flgM_M1 on class III genes (Figure 5). The results confirmed that OmrA_M2 control of flgM_M1 did indeed increase fliC expression (by two-fold; Figure 6). This is less than the four-fold increased expression obtained by deleting flgM (Figure 4), which may be explained by the only 50% inhibition of the flgM_M1 mRNA by OmrA_M2 (Figure 5). Taken together, OmrA/B not only repress the initial step of the flagellar pathway via FlhDC, but also activate subsequent class III gene expression via FlgM.

What is the biological role of OmrA/B-dependent indirect activation of class III flagellar genes? One rationale is stabilization of states. Keeping a biofilm program OFF, and motility ON, largely depends on layers of transcriptional control, which also counter-regulate the opposite program [1–3]. The biofilm-OFF program is reinforced by many inhibitory sRNAs converging on csgD expression [2,35,48]. As discussed elsewhere, silent states are difficult to maintain by transcriptional repressors [34,49,50]. Conversely, post-transcriptional inhibition by sRNAs can maintain a silent state by scavenging mRNAs that have escaped transcriptional repression [35,51]. Simultaneously, reinforcing the motility ON program also involves sRNAs, such as McaS that activates FlhD translation [14] and – as we show here – OmrA/B that repress the anti-Sigma factor FlgM. Both McaS and OmrA/B are also known inhibitors of csgD [14].

OmrA/B, via downregulation of the anti-Sigma factor FlgM which frees up σ²⁸, act within the second tier of flagellar gene regulation, and promote an overall increase in class III flagellar gene expression. Since these sRNAs also inhibit flhD, which should decrease both class II and III flagellar gene expression, this may seem counterintuitive. We note however that FlhD₄C₂ and σ²⁸ control different regulons [25,52]. The class III flagella genes require σ²⁸ for expression and encode proteins required for late flagella assembly (flagellar filament and motor) as well as chemotaxis. Therefore, once flagella synthesis is initiated, OmrA/B might favour the completion of the pathway rather than the abortion of an energetically costly process. σ²⁸ also drives expression of trg, tar, and aer [25]. While not classified as class III flagella genes, they are sensory proteins involved in chemotaxis. Modulation of FlhD₄C₂ (as well as DgcM and CsgD) levels under osmotic stress conditions, when OmrA and OmrB expression is activated via the OmpR/EnvZ two component system, could be of importance when assembly of large structures such as flagella (and curli-fibres) at the cell membrane might have detrimental effects on cell survival [53]. However, the new layer provided by the regulation of flgM could help the bacteria to integrate multiple environmental signals, and combine McaS and OmrA/B to coordinate and promote bacterial motility in response to osmotic and low nutrient stress. This might simultaneously boost their combined negative effect on biofilm formation, tipping the balance towards motility under specific conditions [10,14,17,21].

The experiments conducted in this paper were carried out in liquid medium. Though cell cultures faithfully recapitulate the temporal patterns of hierarchical flagellar gene expression [27,54], structured enterobacterial biofilms on solid media display features that cannot be assessed in liquid. Foremost, though cells in the biofilm structure show nutrient-gradient-depending differences in activity of the key regulators (e.g. PDEs, DGCs, σ^S, FhlDC, CsgD), cell states in middle layers indicate microheterogeneity [54,55]. It would be an interesting question to ask whether, for instance, the balance of OmrA/B-mediated effects on flgM, and fhlD, which oppositely affect flagellar gene expression, are dependent on external or internal factors in a structured biofilm. The complexity of flagellar gene regulation, with regulatory motifs that may generate enforcement of an ongoing program but also cell-to-cell variation, remains a great challenge.

Materials and methods

Chemicals, reagents and oligodeoxyribonucleotides

Growth media components were purchased from Oxoid. Chemicals and oligodeoxyribonucleotides (Table S1) were bought from Sigma-Aldrich, and all reagents from ThermoFisher Scientific, unless otherwise stated. Plasmid DNA and PCR products were purified with the mini prep kit (K0503) and the PCR clean up kit (K0702) from Thermo Scientific.

Growth conditions

Cells were routinely grown aerobically at 37°C in L Broth (5 g/L yeast extract, 10 g/L NaCl, 10 g/L tryptone). When required, antibiotics were added at 100 µg/ml (ampicillin), 50 µg/ml (kanamycin), and 15 µg/ml (chloramphenicol, tetracycline).

Bacterial strains and plasmids

Strains and plasmids are listed in Table S2 and Table S3, respectively. Plasmids pOmrA and pOmrB were previously published [10]. Plasmid pFlgM::GFP was constructed by inserting a NsiI/NheI-digested PCR product (primers EHO-671/EHO-433) into NsiI/NheI-digested plasmid pXG-10 [38]. Plasmids pFlgM_M1, pOmrA_M1 and pOmrB_M1 were created by site-directed mutagenesis (QuickChange II, Stratagene), using primer pairs EHO-696/EHO697, EHO-698/EHO-699 or EHO-700/EHO-701, and plasmids pFlgM::GFP, pOmrA or pOmrB as templates, respectively. Chemically competent E. coli Top10 cells were used for all transformations (C404003, Invitrogen). In-frame deletions of flgM and flgM_M1 were obtained using the Lambda red scarless mutagenesis method as described in [17]. For flgM-3xflag transcription, a plasmid with a T7 promoter, the flgM ORF, a 3xflag sequence, and T7 terminator was created using the pET52-b vector from Novagen as backbone. The plasmid was linearized by PCR using primers MHO-238 and MHO-239, introducing a 3xflag sequence and XhoI/AatII restriction sites while simultaneously deleting the His-tag and multiple cloning site. The flgM 5ʹ UTR and ORF up to the stop codon were PCR-amplified with primers MHO-240/MHO-241 to introduce XhoI/AatII restriction sites. After digestion (fast-digest, Thermo Scientific), vector and flgM insert were ligated using ready-to-go T4 ligase (Amersham, 27-0361-01), resulting in the pflgM-3xflag plasmid.

In vitro transcription and labelling of RNA

OmrA and OmrB small RNAs were generated as previously described [10]. To generate the flgM mRNA fragment (nucleotides 1–200), DNA templates containing a T7 promoter sequence were generated by PCR using primers EHO-714/MHO-200 with E. coli MC4100 relA+ DNA as a template. DNA templates for ompA-3xflag and flgM-3xflag mRNA transcription were obtained by PCR with primers MHO-207 and MHO-230 using E. coli MC4100 ompA-3xflag (E397) as a template, and with primers MHO-244/MHO-245 with pflgM 3xflgM as template, respectively. The resulting PCR products were used for in vitro transcription using the Megascript kit (Life technologies, AM1330) according to the manufacturer’s instructions. Full-length mRNAs were purified using denaturing polyacrylamide-urea gel electrophoresis. After detection by UV-shadowing, RNA was eluted by incubation of the gel slice in elution buffer (300 mM sodium acetate, 0.1% SDS, 1 mM EDTA). After phenol-chloroform extraction, RNAs were precipitated with cold ethanol, centrifuged, and finally dissolved in sterile water. RNA concentration and quality were assessed by Nanodrop and denaturing PAGE.

5ʹ end labelling was performed on RNA pre-treated with CIAP (Invitrogen™, #18,009-019) with T4 PNK (Thermo Scientific, #EK0031) and [γ-P³²]ATP (10 mCi/ml, 3000 Ci/mmol). Labelled RNAs were gel-purified as described above.

Before use and unless specified otherwise, RNAs were denatured separately in water for 1 min at 95°C followed by 1 min incubation on ice, and renatured 5 min at 37°C in renaturation buffer (100 mM potassium acetate, 10 mM magnesium acetate, 50 mM Tris-HCl pH 7,5).

RNA secondary structure probing

Structural probing was carried out on 5ʹ end labelled flgM RNA (10 nM, 50 000 cpm) with or without OmrA/B (10 µM final concentration) at 37°C, with carrier yeast tRNA. After renaturation, mRNAs and sRNAs were incubated together for 15 min. Enzymatic probing was done with 0.1 unit of RNase T1 (Invitrogen™, AM2283) for 5 min and stopped by addition of cold sodium acetate immediately followed by phenol/chloroform/isoamyl alcohol (25/24/1) extraction and RNA precipitation. RNA pellets were dried and dissolved in loading dye. Samples were resolved by 8% denaturing urea-PAGE. The gel was fixed for 5 min at r.t. (10% ethanol, 6% acetic acid), transferred to a 3 mm Whatman filter, then dried at 80°C for 1 h. Radioactive signals were detected using PhosphorImager screens and a PMI scanner™ (Biorad).

Toeprinting assay

Toeprinting reactions and 30S ribosome preparations were carried out as in [56]. Final concentrations of reaction components were: 20 nM mRNA, 100 nM 30S, 300 nM initiator tRNA, 0.5 mM dNTPs, and 10 µM sRNAs (OmrA/B or IstR1).

In vitro translation assay

For in vitro translation assays, the PURExpress® In Vitro Protein Synthesis Kit (New England Biolabs, E6800 S [57]) was used. Final concentrations: 50 nM flgM-3xflag, 0.03 nM ompA-3xflag, 2.5 µM OmrA or OmrB, and 18 nM Hfq (prepared as in [58]). After renaturation, mRNAs (± Hfq and/or OmrA/B), were pre-incubated in pre-mixed PURExpress solution A and B. Translation was carried out for 30 min at 37°C, followed by addition of Laemmli sample buffer (Biorad, 1610747) supplemented with 1/10th volume of 2-mercaptoethanol. Samples were kept on ice, before boiling at 95°C for 5 min. Proteins and ladder (PageRuler™ Prestained Protein Ladder, 26616, Thermo Scientific) were separated on an Any kD™ Mini-PROTEAN® TGX Stain-Free™ Gel (Biorad, 4509036). Proteins were transferred to a Trans-Blot Turbo™ Mini PVDF membrane (Biorad, 1704156) using the Trans-Blot Turbo Transfer System (Biorad, ‘Any Kd’ preset program). After o.n. blocking in Odyssey® Blocking Buffer (PBS) (LI-COR) at 4°C, translation products were detected with monoclonal ANTI-FLAG M2-Peroxidase (HRP) antibody (Sigma, A8592). After 1 h of incubation with the antibody at r.t., membranes were washed 3x with PBS-Tween 20 (0.1%) followed by two washes with PBS. Blots were developed using Amersham™ ECL™ Prime Western Blotting Detection Reagent (GE Healthcare, RPN2109) and imaged on a ChemiDoc™ MP (Biorad). Images were analysed with Image lab software (version 4.0 built 16).

Fluorescence measurements

Bacterial cultures grown overnight from single colonies were diluted 1:100 in fresh LB medium and grown in black 96-well plates with clear flat bottom (Costar®) at 37°C. Fluorescence (GFP: excitation 480 nm, emission 520 nm) and optical density (600 nm) were measured for 23 h at 5 min intervals in a plate reader (Tecan infinite pro). Fluorescence values were divided by optical density and corrected for media background. Background-subtracted GFP/OD₆₀₀ from each strain and time point were averaged and expressed relative to the relevant control strain.

Funding Statement

This work was supported by The Swedish Research Council (to EGHW and EH) and the Swedish Foundation for Strategic Research (to EH),Stiftelsen för Strategisk Forskning[ICA16-0021]; Vetenskapsrådet [2016-03656]; Vetenskapsrådet [2016-03765]

Disclosure of potential conflicts of interest

No potential conflict of interest was reported by the authors.

Supplemental material

Supplemental data for this article can be accessed here.