Two nucleotide second messengers regulate the production of the Vibrio cholerae colonization factor GbpA
BMC Microbiology volume 15, Article number: 166 (2015)
The nucleotide second messengers cAMP and c-di-GMP allow many bacteria, including the human intestinal pathogen Vibrio cholerae, to respond to environmental stimuli with appropriate physiological adaptations. In response to limitation of specific carbohydrates, cAMP and its receptor CRP control the transcription of genes important for nutrient acquisition and utilization; c-di-GMP controls the transition between motile and sessile lifestyles often, but not exclusively, through transcriptional mechanisms. In this study, we investigated the convergence of cAMP and c-di-GMP signaling pathways in regulating the expression of gbpA. GbpA is a colonization factor that participates in the attachment of V. cholerae to N-acetylglucosamine-containing surfaces in its native aquatic environment and the host intestinal tract.
We show that c-di-GMP inhibits gbpA activation in a fashion independent of the known transcription factors that directly sense c-di-GMP. Interestingly, inhibition of gbpA activation by c-di-GMP only occurs during growth on non-PTS dependent nutrient sources. Consistent with this result, we show that CRP binds to the gbpA promoter in a cAMP-dependent manner in vitro and drives transcription of gbpA in vivo. The interplay between cAMP and c-di-GMP does not broadly impact the CRP-cAMP regulon, but occurs more specifically at the gbpA promoter.
These findings suggest that c-di-GMP directly interferes with the interaction of CRP-cAMP and the gbpA promoter via an unidentified regulator. The use of two distinct second messenger signaling mechanisms to regulate gbpA transcription may allow V. cholerae to finely modulate GbpA production, and therefore colonization of aquatic and host surfaces, in response to discrete environmental stimuli.
Nucleotide second messengers in bacteria play a key role in relaying information from the extracellular environment to intracellular effectors, resulting in an adaptive physiological response. Production of these intracellular nucleotides, which include c-di-GMP, c-di-AMP, cGMP, cAMP, and (p)ppGpp, regulates fundamental processes relating including biofilm formation, motility, nutrient acquisition, stress responses, sporulation and, in some pathogens, virulence factor production (reviewed in [1–4]).
C-di-GMP, utilized by many Gram-negative and Gram-positive bacteria, usually regulates transitions between motile and non-motile lifestyles. Specifically, c-di-GMP negatively regulates flagellar motility by inhibiting flagellum biosynthesis or function, and positively regulates adherence and biofilm development in many species . The intracellular levels of c-di-GMP are regulated by the opposing activities of diguanylate cyclase (DGC) biosynthetic enzymes and phosphodiesterase (PDE) hydrolytic enzymes [6–12]. Many organisms contain numerous genes that encode proteins with known or predicted functions as DGC and/or PDE enzymes. To date there are several known intracellular c-di-GMP receptors, including protein and RNA-based sensors. Proteins that directly sense c-di-GMP include transcription factors, proteins containing the well-characterized PilZ domain, and others such as catalytically inactive PDEs that retain the capacity to bind c-di-GMP . In addition, two distinct classes of c-di-GMP sensing riboswitch, broadly present in bacterial genomes, have been identified [14–17]. The presence of numerous c-di-GMP metabolic enzymes and an array of intracellular c-di-GMP receptors points to complex c-di-GMP signaling networks that modulates a wide array of cellular functions.
In the human diarrheal pathogen Vibrio cholerae, c-di-GMP promotes biofilm formation and inhibits flagellar motility [18–20]; in addition, c-di-GMP inhibits the expression of virulence genes including those encoding the major virulence factor, cholera toxin . To date, three transcription factors that directly sense c-di-GMP have been identified in V. cholerae: VpsT, VpsR and FlrA [22–24]. Each of these was previously characterized as a regulator of biofilm formation and/or motility [20, 25–28]. Five proteins containing a PilZ domain have been described in V. cholerae, some of which have roles in biofilm, motility and/or virulence . The V. cholerae genome also encodes two c-di-GMP riboswitches, Vc1 and Vc2, which lie upstream of gbpA and VC1722, respectively .
cAMP signaling is widespread in bacteria, and intracellular cAMP levels are heavily influenced by the availability of extracellular nutrient sources . In Gram-negative bacteria, uptake of a preferred sugar by the phosphoenolpyruvate-carbohydrate phosphotransferase transport system (PTS) relies on a sugar-specific transporter, EIIA. Following uptake of a PTS sugar, EIIA and other PTS components participate in a phosphorylation cascade that culminates phospho-transfer from EIIA to the incoming sugar. The phosphorylation state of EIIA serves as a measure of PTS sugar availability. Under conditions of PTS sugar limitation (and absence of a PTS sugar substrate), EIIA remains phosphorylated and stimulates the adenylate cyclase (AC), triggering cAMP biosynthesis. To date, the only known sensor of cAMP in bacteria is the cAMP receptor protein (CRP) . Together, the cAMP-CRP complex promotes the expression of genes involved in the uptake and utilization of non-PTS nutrient sources.
V. cholerae uses the cAMP-CRP system to respond to the absence of PTS-dependent sugars such as N-acetylglucosamine, sucrose, mannitol and fructose . Unlike E. coli, in which glucose utilization is PTS-dependent, glucose can be utilized via PTS and non-PTS mechanisms in V. cholerae . V. cholerae has also adapted the cAMP-CRP pathway to promote motility and inhibit biofilm formation [32, 33]. Transcriptome analyses have shown that cya and crp deletion mutants (which lack cAMP biosynthesis and sensing, respectively) have increased expression of genes involved in extracellular matrix production, reduced expression of genes involved in flagellum biosynthesis and chemotaxis [32, 33]. In addition, a crp deletion mutant has reduced expression of genes important for colonization and is attenuated in a mouse model of infection . Interestingly, the cAMP-CRP signaling pathway impinges upon the c-di-GMP signaling network; a crp mutant has altered expression of numerous genes involved in c-di-GMP metabolism .
V. cholerae naturally inhabits aquatic reservoirs, where it associates with chitinous surfaces such the exoskeletons of zooplankton and crustaceans . V. cholerae can be ingested through consumption of contaminated food or water and subsequently colonize the small intestine and cause diarrheal disease in humans. The colonization factor GbpA aids in the attachment of V. cholerae to surfaces in its native aquatic environment and in the host intestine [35, 36]. GbpA recognizes N-acetylglucosamine (GlcNAc), a component of mucin and a modification of glycoprotein and lipids found on the surface of the intestinal epithelium, thus mediating interactions with the host intestinal epithelium [35, 36]. GlcNAc also comprises the polymer chitin, a major component of the exoskeletons of crustaceans and zooplankton, thus serving as a substratum for V. cholerae colonization in aquatic reservoirs . In addition to serving as a ligand for GbpA, GlcNAc also regulates gbpA expression via the transcriptional regulator NagC [37, 38]. In V. cholerae and some other bacterial species, the transcription factor NagC regulates gene expression in response to GlcNAc and typically controls genes involved in GlcNAc uptake and metabolism [38–42]. Transcriptional profiling of a V. cholerae nagC mutant indicated that NagC represses gbpA transcription , suggesting that gbpA expression is down-regulated in the presence of mucin- and chitin-derived GlcNAc in the small intestine and in the aquatic environment, respectively [36–38].
In this study, we investigated the combined roles of the second messengers cAMP and c-di-GMP in regulating gbpA transcription. We report that c-di-GMP inhibits gbpA transcription independently of the previously described c-di-GMP riboswitch. Expression of gbpA is also influenced by the availability of PTS-dependent carbohydrates, and is accordingly regulated by cAMP-CRP through direct binding of this complex to the gbpA promoter. Together, our results indicate that gbpA transcription is regulated by both c-di-GMP and cAMP, in opposing fashion. The c-di-GMP and cAMP second messenger signaling pathways may thus function together to modulate the production of GbpA in response to discrete extracellular stimuli, likely impacting the ability of V. cholerae to colonize GlcNAc-containing surfaces in the aquatic and host environments.
Growth conditions and media
Escherichia coli, V. cholerae C6706 and mutant derivatives were cultured at 37 °C with aeration in Luria-Bertani (LB) broth containing 100 μg/ml streptomycin (Sm), 10 μg/ml chloramphenicol (Cm), and/or 50 μg/ml ampicillin (Amp), as appropriate. Where specified, V. cholerae was grown in M9 minimal medium (Fisher Scientific) supplemented with trace metals (1 ml l−1 of 5 % MgSO4, 0.5 % MnCl24H2O, 0.5 % FeCl3, 0.4 % nitrilotriacetic acid)  and 0.5 % (w/v) of the indicated carbon source.
Strains and plasmids included in this study are listed in Additional file 1: Table S1. Primer information is contained in Additional file 1: Table S2. The gbpA, nagC, crp, cpdA, cya, vpsT, vpsR and flrA genes were mutated by standard allelic exchange methods. A deletion in the Vc1 sequence upstream of gbpA was deleted in a similar manner. Using genomic DNA from V. cholerae C6706 as template, ~800 bp fragments upstream and downstream of the sequences to be deleted were amplified by PCR using primers named according to the pattern geneF1 + geneR1 for the upstream region of homology and geneF2 + geneR2 for the downstream region of homology. The primers introduced restriction sites (underlined sequences in Table S2) allowing ligation of the resulting fragments to each other and into the pCVD442 suicide vector. The exception is the vpsR mutation, for which the two fragments were joined by splicing by overlap extension, and then ligated into pCVD442. The ligations were transformed into DH5αλpir by electroporation and transformed colonies were identified on LB-Amp agar. The desired clones containing the upstream and downstream fragments were identified by PCR using primers geneF1 + geneR2 and/or pCVDseqF + pCVDseqR, which flank the multiple cloning site of pCVD442. The allelic exchange steps were done as described previously . Colonies were screened for the desired deletion by PCR using the corresponding geneF0 + geneR2 primers.
VC1592, which encodes an EAL domain c-di-GMP phosphodiesterase [45, 46], was amplified from C6706 genomic DNA using primers VC1592eF + VC1592eH6R. The product was digested with SacI and PstI, ligated into similarly digested pBAD33, and transformed into DH5α. Cm-resistant transformants were screened for the desired insert by PCR, and isolates were confirmed by sequencing.
The pPgbpA-Vc1-lacZ and pPgbpA-∆Vc1-lacZ plasmids were constructed by amplifying the gbpA promoter and 5′ UTR from V. cholerae C6706 and ΔVc1 genomic DNA, respectively, by PCR using gbpAP2F + gbpAR2. The PCR products were digested with EcoRI and SalI and ligated into pPlacthiM#2-lacZ  digested with the same enzymes. The ligation reaction was transformed into DH5α cells by electroporation, and Amp-resistant colonies obtained were screened with primers pLacSeq + gbpAR2. The resulting plasmids have PgbpA-UTR (wild type or ∆Vc1) as a translational fusion to lacZ, with the lac promoter driving transcription. The plasmids were introduced by electroporation into V. cholerae C6706 in which the endogenous lacZ gene was inactivated .
The pBAD33, pPDE (pBAD33::vieA), pPDEmut (pBAD33::vieA-E170A), and pVC1592 (pBAD33::VC1592) plasmids were introduced into the indicated strains by electroporation. Cm-resistant isolates were confirmed to have the desired plasmid by PCR.
Manipulation of the intracellular c-di-GMP level in V. cholerae
The intracellular c-di-GMP level was depleted through the ectopic expression of a V. cholerae c-di-GMP phosphodiesterase gene, vieA, as described previously [49, 50]. Briefly, V. cholerae bearing pBAD33 (“vector”) or pBAD33::vieA (“pPDE”) were grown in 2 ml LB-Sm-Cm broth at 37 °C with aeration. Ampicillin was included at 50 μg/ml if the strains also contained a lacZ reporter plasmid. For the indicated experiments, V. cholerae with pPDEmut (encoding enzymatically inactive VieA PDE) or pVC1592 (encoding an alternative c-di-GMP PDE) were included . At early exponential phase (OD600 ~ 0.2), 0.2 % L-arabinose was added to the cultures to induce vieA transcription from the P BAD promoter, and incubations were continued at 37 °C with aeration. Samples were collected at mid-exponential phase (optical density at 600 nm (OD600) ~ 0.5-0.7) for western blotting or qRT-PCR analysis as described below.
Reporter activity assays
The β-galactosidase activity was measured for V. cholerae strains containing the P gbpA -Vc1-lacZ fusion, with vector (pBAD33) or pPDE. Strains were grown in 2 ml M9 minimal medium with 0.5 % (w/v) glucose, maltose, sucrose, fructose or casamino acids. Ampicillin (50 μg/ml) and/or chloramphenicol (10 μg/ml) were included in the media as appropriate to maintain plasmids. Cultures were incubated at 37 °C with aeration. Expression of the vieA PDE gene was induced using 0.2 % L-arabinose as described above. Samples were grown to mid-exponential phase (OD600 0.45-0.6), and 100 μl were assayed for hydrolysis of ortho-nitrophenyl-β-D-galactoside using a Miller assay . At least three independent experiments were done, and the data were combined. Statistical analyses were done using unpaired t-tests.
GbpA antibody production
Anti-GbpA antiserum was produced by Yenzym 192 Antibodies, LLC, South San Francisco, CA. Antiserum was raised in rabbits to a synthetic peptide (CSNATQYQPGTGSHWEMAWDKR) that corresponds to GbpA from V. cholerae. The animal facilities were NIH/OLAW/PHS assured, USDA certified, and IACUC regulated.
GbpA and CRP detection by western blot
Equal-volume samples of mid-exponential phase cultures, normalized to OD600 (0.45-0.6), were collected. For detection of GbpA, the samples were centrifuged to remove the bacteria. Supernatant proteins were TCA precipitated, separated by electrophoresis, and subjected to western blotting with rabbit anti-GbpA antibodies. For detection of CRP, cells grown as above were collected by centrifugation. Whole lysates were electrophoresed and transferred to nitrocellulose membranes. CRP (~23.6 kDa) was detected using anti-CRP monoclonal antibodies (Neoclone). For cell lysates, RNA Polymerase β subunit (~150 kDa) served as a loading control and was detected with monoclonal antibodies (AbCam). In all western blots, goat α-rabbit IgG conjugated with IR800 dye (Thermo Scientific) was used as the secondary antibody. The blots were imaged using an Odyssey imaging system (LI-COR). At least three independent experiments were done, and a representative image is shown. Densitometry analyses were done using the Odyssey software. The intensities of the bands corresponding to GbpA in supernatants were normalized to those of a cross reactive band (indicated by asterisks in relevant images). For CRP quantification, the intensities of the bands of CRP in lysates were normalized to those of RNAP.
RNA purification and analysis using quantitative real-time PCR
Transcriptional analyses using quantitative reverse-transcriptase PCR (qRT-PCR) were done as previously described . Briefly, RNA was purified from mid-exponential phase (OD600 ~ 0.5-0.7) cultures. Genomic DNA was removed using the TURBO DNA-free kit (Ambion). For cDNA synthesis, RNA (200 ng) was reverse transcribed using the Tetro cDNA Synthesis Kit (Bioline). We included control reactions without reverse transcriptase for every cDNA sample. For the real time PCR reaction, cDNA and control samples were combined with 2× SYBR/fluorescein mix (SensiMix; Bioline) and 7.5 μM of each primer (named according to the scheme gene-qF and gene-qR for forward and reverse primers, respectively, Additional file 1: Table S2). We used the following program to amplify target cDNA: 95 °C for 10 min, followed by 40 cycles of 95 °C for 30 s, 55 °C for 1 min, and 72 °C for 30 s. Melt curves were included to verify amplification of single products. The data were analyzed using the ΔΔCt method, with Ct values normalized to the specified reference strain/condition, and to the Ct values of the reference gene rpoB and/or gyrA in each sample [52–54]. For each strain/condition, a minimum of three independent samples was tested. Statistical significance was determined by unpaired t-test.
Cloning and expression of crp and purification of the recombinant protein
The CRP gene was amplified from V. cholerae C6706 genomic DNA using primers CRPeF + CRPeH6R, which incorporate EcoRI and SalI restriction sites into the product, respectively. The CRPeH6R primer introduces 6 histidine codons at the 3′ end of the gene. The PCR product was digested with EcoRI and SalI and ligated into similarly digested pMMB67EH, a low-copy vector allowing IPTG-inducible gene expression . Ligations were transformed into E. coli DH5α cells. Ampicillin-resistant colonies containing pMMB67EH with crp-his6 insert were identified by PCR, yielding pMMB::crp-his6.
E. coli DH5α containing pMMB::crp-his6 was grown in LB broth at 37 °C with aeration to early exponential phase (OD600 ~ 0.2), at which point IPTG was added for a 0.5 mM final concentration. The culture was grown at 37 °C with aeration to mid- exponential phase (OD 600 nm ~ 0.7), then cells were collected by centrifugation. Cells were suspended in His6 lysis buffer consisting of 10 mm Tris, pH 8, 300 mm NaCl, 50 mm NaH2PO4, 10 % glycerol, 1 mm phenylmethylsulfonyl fluoride, and 5 mM imidazole . The cells were lysed by sonication, and CRP was purified by affinity chromatography with Ni-NTA resin (ThermoFisher) using the general methods described previously [10, 50]. The eluates were analyzed by SDS-PAGE and coomassie staining. CRP-containing fractions were dialyzed against 5 mM Tris 8.0, 10 mM MgCl2, 5 mM KCl, 5 mM CaCl2, 10 % glycerol using 10,000 MWCO Slide-A-Lyzer Dialysis Cassettes (Thermo Scientific). The CRP preparations were estimated to be > 95 % pure. Glycerol was added to a final concentration of 20 %, and the protein concentration was determined using the BCA Protein Assay Kit (Pierce). Aliquots of the protein were stored at −20 °C.
Electrophoretic mobility shift assays (EMSAs)
A 293 base pair gbpA promoter fragment was amplified from V. cholerae C6706 genomic DNA using primers gbpAP2F + Vc1R2. A 133 base pair non-specific control DNA fragment internal to the gbpA ORF was amplified with gbpAqF2 + gbpAqR2. EMSAs were done as previously described . Binding reactions were done in 10 mM Tris pH 7.5, 1 mM EDTA, 100 mM KCl, 0.1 mM DTT, 5 % glycerol (v/v) and 0.01 mg/ml BSA (final concentrations). The gbpA promoter fragment, CRP, and cAMP (Sigma-Aldrich) were used at final concentrations of 2.5 ng/μl, 11 ng/μl, and 33 μM, respectively. C-di-GMP (Biolog) was used at 33 μM, or 333 μM when in competition with cAMP. The non-specific DNA fragment (75 ng) was added to every mixture. After 1 h incubation at room temperature (~25 °C), the samples were electrophoresed on a 6 % TAE polyacrylamide gel. The gel was stained with GelRed (Biotium, Inc.) in TAE for 10 min, and then visualized under UV light.
Low c-di-GMP induces gbpA transcription
A putative c-di-GMP riboswitch, named Vc1, was previously predicted upstream of the gbpA open reading frame . The Vc1 element shares 75 % identity with the well-characterized c-di-GMP riboswitch Vc2, which has been shown to bind c-di-GMP directly and positively regulate expression of a reporter gene in response to c-di-GMP in a heterologous bacterial host . The identification of the putative c-di-GMP riboswitch Vc1 upstream of gbpA suggests that gbpA expression is regulated by this signaling molecule. To test this, we used a previously described strategy for manipulating intracellular c-di-GMP levels in V. cholerae: the ectopic expression of a c-di-GMP metabolism gene. The expression of the vieA gene, which encodes a c-di-GMP phosphodiesterase, has been used to artificially manipulate intracellular c-di-GMP in V. cholerae, resulting in phenotypes consistent with reduced c-di-GMP: increased motility, reduced biofilm formation, and increased cholera toxin production [21, 50, 57]. To establish that vieA expression similarly results in altered intracellular c-di-GMP in V. cholerae C6706, the wild type strain used in this study, we evaluated the effect of vieA expression from plasmid “pPDE” on motility and biofilm formation, which are inhibited and promoted by c-di-GMP in V. cholerae, respectively. To assay swimming motility, colonies of V. cholerae C6706 with vector (pBAD33) or pPDE were inoculated into soft agar medium containing 0.2 % L-arabinose to induce gene expression, and expansion from the inoculation point was monitored. V. cholerae C6706 with pPDE showed significantly increased motility compared to the vector control (Additional file 2: Figure S1A). Importantly, V. cholerae C6706 with pPDEmut, which contains an E170A mutation that renders VieA enzymatically inactive , showed motility equal to the vector control. These results indicate that c-di-GMP hydrolysis by VieA augments V. cholerae motility, consistent with previous observations . In addition, expression of another EAL-domain c-di-GMP PDE gene, VC1592, enhanced motility comparably to vieA, indicating that the effect on motility is not specific to the VieA PDE [45, 46]. To assay biofilm formation, V. cholerae C6706 with vector or pPDE were grown statically for 24 h in LB broth containing 0.2 % L-arabinose for gene induction, and then the biofilm biomass was evaluated by crystal violet staining. Biofilm formation of V. cholerae C6706 with pPDE was reduced to 25 % of that generated by the vector control strain; expression of VC1592 similarly reduced biofilm production (Additional file 2: Figure S1B). Biofilm formation of V. cholerae C6706 with pPDEmut was intermediate between V. cholerae C6706 strains expressing functional PDE genes and the vector control strain. Combined with the motility assay results, these findings indicate that ectopic production of VieA effectively reduces intracellular c-di-GMP in V. cholerae C6706, reflected by increased swimming motility and reduced biofilm formation.
Using this expression strategy to manipulate intracellular c-di-GMP, we evaluated the effect of altering c-di-GMP on the abundance of the gbpA transcript and GbpA protein in V. cholerae with pPDE compared to V. cholerae with vector (grown in the presence of 0.2 % L-arabinose to drive vieA transcription as described in the Methods). Western blot analysis of GbpA production showed that GbpA was 2.8-fold more abundant in V. cholerae with reduced c-di-GMP (pPDE) (Fig. 1a). Regulation by c-di-GMP occurred at the level of transcription, as quantitative real time PCR analysis indicated that gbpA transcript levels were 11.1-fold higher in V. cholerae with pPDE (Fig. 1b). Importantly, gbpA transcript was similarly increased in V. cholerae with pVC1592, in which the alternative c-di-GMP PDE is produced, and is not altered in V. cholerae with pPDEmut, in which the enzymatically inactive VieA is produced (Fig. 1c). These results indicate the effect of VieA production on gbpA levels was due to depletion of c-di-GMP, and not a consequence of another regulatory function of VieA. Throughout the remainder of the study, we used V. cholerae C6706 with pPDE grown in the presence of arabinose to represent low c-di-GMP conditions, with V. cholerae C6706 with vector grown in the same conditions serving as the wild-type c-di-GMP control.
c-di-GMP inhibition of gbpA transcription is independent of the putative riboswitch Vc1
We next tested whether c-di-GMP induction of GbpA production is dependent on the putative riboswitch Vc1. To do this, we assessed the effect of depleting c-di-GMP in V. cholerae lacking the Vc1 sequence. This strain, ∆Vc1, lacks nucleotides 17–202 of the transcript, which encompass most of the 5′UTR including the c-di-GMP riboswitch, but retains the native gbpA promoter and the native ribosomal binding site. The pPDE and control plasmids were introduced into the ΔVc1 mutant, and the strains were assessed for changes in gbpA expression. In the ∆Vc1 strain with vector, gbpA transcript (Fig. 1b) and GbpA protein (Fig. 1a) were diminished by 75 and 83 %, respectively, compared to the wild type with vector, suggesting that removal of nucleotides 17–202 reduces expression. Yet depletion of c-di-GMP in the ΔVc1 strain (pPDE) increased GbpA production 3.4-fold (Fig. 1b) and gbpA transcription 15.4-fold (Fig. 1a), an effect equivalent to that seen in the wild type background.
In addition, we used lacZ fusions to either the wild type gbpA promoter and 5′UTR (P gbpA -Vc1-lacZ) or the promoter and 5′UTR lacking Vc1 (P gbpA -∆Vc1-lacZ) as reporters of gbpA expression. We measured β-galactosidase activity in V. cholerae with these plasmid-borne reporters, each with either vector or pPDE. In both the P gbpA -Vc1-lacZ and P gbpA -∆Vc1-lacZ reporter strains, reduction of c-di-GMP (pPDE) resulted in a statistically significant ~2-fold increase in β-galactosidase activity (Fig. 1d). Thus, c-di-GMP inhibition of gbpA expression is independent of Vc1, indicating that low intracellular c-di-GMP concentrations promote gbpA transcription initiation via the gbpA promoter.
The c-di-GMP responsive regulators VpsT, VpsR and FlrA are not involved in the regulation of gbpA transcription by c-di-GMP
We next aimed to determine the mechanism by which c-di-GMP inhibits gbpA transcription. We hypothesized that a c-di-GMP sensing transcription factor interacts with the gbpA promoter, either inhibiting expression in response to c-di-GMP, or alleviating activation in response to c-di-GMP. We first focused on three previously identified c-di-GMP binding transcription factors, VpsT, FlrA and VpsR, as potential mediators of c-di-GMP regulation of gbpA expression [22–24]. Transcriptional profiling studies analyzing V. cholerae vpsT, vpsR and flrA mutants have implicated each of the regulators in controlling gbpA expression [20, 58]. The FlrA protein was recently shown to directly sense c-di-GMP, and c-di-GMP binding inhibits the interaction of FlrA with a target flagellar gene promoter (flrBC) . Similarly, VpsT, a well-known activator of biofilm exopolysaccharide genes in V. cholerae , was recently shown to bind c-di-GMP, resulting in enhanced binding to the EPS gene promoters . Finally, VpsR, another positive regulator of V. cholerae exopolysaccharide gene expression and biofilm production , appears to interact directly with c-di-GMP; unlike VpsT and FlrA, c-di-GMP binding did not influence VpsR binding to target promoters (vpsT and aphA) .
We tested the effect of vpsT, vpsR or flrA mutation on gbpA expression in response to c-di-GMP. The pPDE and control plasmids were introduced into the ΔvpsT, ΔvpsT and ΔflrA mutants, and gbpA expression was assessed by qRT-PCR and by western blot. Transcript analysis showed that the flrA mutant had somewhat (1.4-fold) higher gbpA transcript levels, and the vpsT and vpsR mutants had lower levels (55 and 46 % decreased, respectively), than the parental strain (Fig. 2b). These differences were not statistically significant, but the trends were supported by the results of the western blots comparing GbpA protein abundance in the mutants compared to the wild type with vector (Fig. 2a). Furthermore, depletion of c-di-GMP (pPDE) in the ΔflrA, ΔvpsT and ΔvpsR mutants resulted in 4.8-, 9.6- and 11.0-fold increased gbpA transcript, respectively, compared to the mutants with unmodified c-di-GMP (Fig. 2b). Inhibition of gbpA expression by c-di-GMP in the mutants and the wild type was apparent at the protein level as well (Fig. 2a). The observed changes were equivalent to the increase seen in the wild type background. Thus, none of the known c-di-GMP sensing transcription factors are required for positive regulation of gbpA expression by depletion this second messenger. It remains possible that c-di-GMP influences gbpA expression via these transcription factors in more subtle ways that are not apparent using the c-di-GMP depletion strategy.
c-di-GMP inhibits gbpA transcription in a nutrient dependent manner
GlcNAc and GlcNAc-containing mucin have been shown to regulate gbpA expression, and to date the only known transcriptional regulator of gbpA is NagC, a repressor of genes involved in GlcNAc utilization and of gbpA transcription [36–38]. We sought to determine how c-di-GMP impacts regulation of the gbpA promoter in the presence of N-acetylglucosamine (GlcNAc). We reasoned that GlcNAc, and perhaps other carbohydrates, may affect c-di-GMP inhibition of gbpA expression, and that NagC may participate in this process. Specifically, we postulated that c-di-GMP promotes NagC inhibition of gbpA expression, such that depletion of c-di-GMP results in NagC de-repression.
To test the effect of GlcNAc on regulation of gbpA expression by c-di-GMP, we generated V. cholerae strains with a translational fusion of lacZ to the gbpA promoter and 5′UTR, with either pPDE or the vector control. These strains were grown in a defined medium (M9 minimal medium, MM) supplemented with 0.5 % (w/v) GlcNAc, glucose, maltose, sucrose, fructose or casamino acids. The additional carbohydrates were included to address whether the potential effect of GlcNAc is specific to this sugar, and casamino acids were included as a non-carbohydrate carbon source control. The cultures were grown to mid-exponential phase (OD600 0.45-0.6), and expression of gbpA was measured by β-galactosidase assay, allowing normalization to the optical density of the culture to adjust for differences in growth due to the carbon source. Expression of gbpA was variable in the media tested (Fig. 3, black bars), possibly due to differences in growth rate with the different carbon sources (Additional file 2: Figure S2). Compared to V. cholerae with wild type c-di-GMP levels, reduction of c-di-GMP led to significantly increased reporter activity in V. cholerae grown in GlcNAc (1.35-fold), glucose (1.73-fold), maltose (1.59-fold) and casamino acids (1.67-fold), but not in bacteria grown in sucrose or fructose (Fig. 3, grey bars). The results could not be attributed to growth rate, as depleting c-di-GMP (pPDE) did not affect overall growth in these media (Additional file 2: Figure S2). These results indicate that growth on GlcNAc does not interfere with c-di-GMP regulation of gbpA expression.
To test whether NagC is required for c-di-GMP inhibition of gbpA expression, pPDE and the control vector were introduced into V. cholerae with an in-frame deletion of nagC (∆nagC). Consistent with previous reports [37, 38], deletion of nagC resulted in 2.2-fold higher GbpA protein (Fig. 4a) and 1.8-fold higher gbpA transcript abundance (Fig. 4b) than in the wild type. Upon lowering c-di-GMP levels through PDE gene expression, we observed 20-fold and 2.4-fold increases in gbpA transcript and GbpA protein, respectively, comparable to those seen in the wild type background (Fig. 4a and 4b, respectively). Thus, NagC is not required for gbpA inhibition by c-di-GMP, corroborating the lack of an effect of growth with GlcNAc as the sole carbon source.
Low c-di-GMP induces gbpA transcription in a cAMP-CRP-dependent manner
In V. cholerae, GlcNAc, sucrose and fructose are solely imported via a phosphoenolpyruvate-carbohydrate phosphotransferase system (PTS), and maltose is taken up via a PTS-independent mechanism . Glucose is a PTS-substrate that can also be imported via a PTS-independent pathway, and GlcNAc has been reported to be a PTS dependent carbohydrate in V. cholerae . However, a V. cholerae nagE mutant, which does not produce the GlcNAc PTS transporter component, is able to grow, albeit at a reduced rate, with GlcNAc as the sole carbon source, suggesting that an alternate GlcNAc uptake pathway(s) exists . We observed that c-di-GMP inhibition of gbpA expression did not occur during growth relying on the strictly PTS-dependent carbohydrates sucrose and fructose (Fig. 3), suggesting a dependence of c-di-GMP regulation on carbon source availability and the mechanism of uptake. Limitation of PTS-carbohydrates results in increased cAMP biosynthesis and CRP activation, allowing the bacterium to activate alternate metabolic pathways . Our results suggest that c-di-GMP inhibits gbpA transcription when cAMP-CRP levels are elevated. We thus considered the possibility that cAMP-CRP regulates gbpA transcription in a mechanism that is influenced by c-di-GMP levels.
To test the role of CRP in regulating gbpA in response to c-di-GMP, we generated a V. cholerae Δcrp mutant and examined it for gbpA production. By western blot, the Δcrp mutant reproducibly produced ~40 % less GbpA than the parent strain, supporting a role for CRP in upregulating GbpA production (Fig. 4a). The gbpA transcript was also reduced by 53 % in the Δcrp mutant (Fig. 4b). We next determined the role of CRP in mediating c-di-GMP regulation of gbpA by assessing expression in the Δcrp mutant bearing pPDE. Unlike in wild-type V. cholerae with the control plasmid, when intracellular c-di-GMP levels were lowered by PDE production in the ∆crp strain, there was no change in gbpA transcript or GbpA protein levels (Fig. 4a and 4b, respectively), indicating that CRP is required for activation of gbpA expression in response to decreased c-di-GMP concentrations.
We next evaluated the role of cAMP in the regulation of gbpA in V. cholerae. We generated a strain with an in-frame deletion of cya, which encodes the adenylate cyclase that synthesizes cAMP, yielding a strain that is incapable of CRP activation . The cya mutant, like the CRP mutant, produced less GbpA, with an 80 % decrease in protein compared to the wild type (Fig. 5a). A significant 80 % reduction in gbpA transcript abundance was also observed in the cya mutant using qRT-PCR (Fig. 5b). V. cholerae Δcya was then transformed with pPDE or the control vector, allowing us to determine the interplay between cAMP and c-di-GMP in controlling gbpA expression. When intracellular c-di-GMP was lowered by PDE production in the ∆cya background, there was no change in gbpA transcript or GbpA protein levels (Fig. 5a and 5b), mirroring the effect seen with the crp mutation.
Additionally, we tested the effect of CRP activation on GbpA production by mutating cpdA, which encodes the cAMP phosphodiesterase. In this mutant, cAMP cannot be degraded, and cAMP-CRP complex is constitutively active . In the cpdA mutant the levels of gbpA transcript and GbpA production were comparable the wild type parent (Fig. 5a and 5b). Reducing c-di-GMP (pPDE) in the cpdA mutant increased gbpA transcript and GbpA protein levels by 10.5-fold and 3.2-fold, respectively, compared to the same strain with unmodified c-di-GMP (Fig. 5a and 5b). These data further support that cAMP-CRP activates the expression of gbpA, and indicate that cAMP and CRP are required for c-di-GMP inhibition of gbpA expression.
CRP production and activity are not directly affected by c-di-GMP
We next sought to understand how c-di-GMP influences CRP-dependent activation of gbpA expression; c-di-GMP could regulate crp transcription, CRP protein levels or CRP regulatory activity. To assess the effect of c-di-GMP on crp expression, crp transcript levels were measured in V. cholerae with wild type (vector) or reduced c-di-GMP levels (pPDE). Transcript levels of crp were not affected by altering c-di-GMP (Fig. 6a), suggesting that c-di-GMP directly or indirectly affects CRP protein levels or activity. The effect of c-di-GMP on CRP protein levels was determined by western blot. Lysates from wild type V. cholerae with vector or pPDE, as well as a crp-null control strain containing vector, were probed with anti-CRP antibodies. No differences in CRP abundance were apparent in V. cholerae with wild type or low c-di-GMP (Fig. 6b).
The identification of a consensus CRP binding site (GTGAGAGCTTGATTCCACATAT) upstream of gbpA (and upstream of the Vc1 sequence) using Virtual Footprint software  suggests that CRP interacts directly with the gbpA promoter. We postulated that c-di-GMP may interfere with the DNA-binding activity of CRP. To test this, we used electrophoretic mobility shift assays (EMSAs) to evaluate the interactions between CRP, c-di-GMP and the gbpA promoter. A 293 bp DNA fragment encompassing the gbpA promoter and C-terminally tagged CRP were used, and a non-specific 133 bp DNA fragment was included as a negative control in each sample. As observed previously for other promoters [61, 62], CRP alone was unable to bind the gbpA promoter fragment, but upon addition of the CRP ligand cAMP, CRP bound and shifted the gbpA promoter fragment (Fig. 6c). In contrast, the presence of c-di-GMP did not promote an interaction between CRP and the promoter fragment. Moreover, the addition of 10-fold excess c-d-GMP did not interfere with cAMP-CRP binding to the gbpA promoter. Therefore, in vitro, c-di-GMP does not influence the binding of cAMP–CRP to the gbpA promoter.
The c-di-GMP and cAMP-CRP signaling pathways act together on the gbpA promoter, but not other cAMP-CRP regulatory targets
To determine if c-di-GMP impacts the regulatory function of CRP, we assessed the regulation of additional CRP regulatory targets by c-di-GMP. We predicted that if c-di-GMP was having a global effect on CRP activity, additional CRP targets would be regulated in a fashion similar to gbpA. We tested three metabolic genes that are predicted targets of cAMP-CRP, VC1046, VC2013, and VC2544. All three genes were identified in a transcriptome analysis identifying CRP and cAMP regulated genes , and we additionally selected them because they each have a predicted CRP binding site in their promoter (Virtual Footprint) . Our results showed that relative to the wild type parent strain, transcript levels of VC1046, VC2013, and VC2544 were reduced by 65 % or more in the ∆crp background, suggesting that these genes are positively regulated by CRP (Fig. 7a). Next, we compared the abundance of these transcripts in wild type V. cholerae with vector or pPDE to determine whether manipulation of c-di-GMP affected expression of these genes. Whereas c-di-GMP depletion resulted in an 18.5-fold increase in gbpA transcript abundance, we observed no difference in the abundance of these transcripts in the strain with low c-di-GMP, as compared to wild type c-di-GMP levels (Fig. 7b). Together, these results suggest that the effect of low c-di-GMP on CRP activity at the gbpA promoter is not a global regulatory effect and that an additional factor mediates the impact of c-di-GMP on gbpA transcription initiation.
In response to extracellular stimuli, bacteria manipulate the levels of intracellular second messengers to drive behavioral changes that promote survival. Herein, we describe the combined effects of two nucleotide second messengers, c-di-GMP and cAMP, on transcriptional regulation of gbpA, a gene encoding a V. cholerae colonization factor produced in aquatic and host environmental conditions. Whereas cAMP promotes gbpA transcription via CRP binding to the gbpA promoter, c-di-GMP has a negative effect of gbpA promoter activity, and cAMP-CRP is epistatic to c-di-GMP regulation . As distinct extracellular cues trigger the c-di-GMP and cAMP signaling pathways, GbpA production may be modulated in response to multiple environmental parameters encountered by V. cholerae.
Having determined that c-di-GMP negatively affects gbpA promoter activity, we sought to identify the c-di-GMP effector that acts on the gbpA promoter. In the process, we determined that CRP activates gbpA transcription. The CRP protein binds the gbpA promoter in a cAMP-dependent manner in vitro, and a crp mutant has somewhat decreased production of GbpA. Moreover, in the crp mutant, depletion of c-di-GMP did not result in increased gbpA expression. The same effect was apparent in a cya mutant, which lacks the adenylate cyclase responsible for cAMP synthesis (eliminating the CRP activating signal). The observation that a cAMP phosphodiesterase (cpdA) mutant, with constitutively activated CRP, showed the same increase in GbpA upon c-di-GMP depletion as the parental strain indicates that cAMP-CRP promotes gbpA transcription, and only under CRP-activating conditions is the inhibitory effect of c-di-GMP on gbpA transcription apparent. Consistent with this, c-di-GMP inhibition of gbpA expression was observed during growth on carbon sources that do not rely on a PTS for uptake (glucose, maltose and casamino acids)—conditions in which cAMP is produced and CRP is active . In contrast, growth in media with the PTS-dependent sugars sucrose and fructose, whose uptake does not stimulate cAMP production and CRP activation , did not reveal an effect of c-di-GMP. Thus, c-di-GMP inhibition of gbpA transcription is observable when cAMP-CRP levels are high. That gbpA transcription was comparable in the presence of PTS-dependent and independent nutrient sources was a surprising result given that we anticipated that growth with PTS carbohydrates and the resulting low cAMP-CRP would decrease gbpA expression. However, it is possible that expression is affected by growth rate, which varies between growth media.
Given the role of CRP in c-di-GMP regulation of gbpA expression, we explored the possibility that c-di-GMP influences CRP at various levels. We excluded effects of c-di-GMP on CRP gene transcription and protein abundance. In other bacterial species, c-di-GMP has a direct role in controlling the activity of CRP-like proteins [63, 64]. For example, c-di-GMP has been shown to bind CAP (catabolite activation protein)-like protein CLP from Xanthomonas campestris, which inhibits its ability to bind DNA and thus to regulate virulence gene expression . Our data indicate that, while CRP does bind the gbpA promoter in a cAMP-dependent manner, c-di-GMP does not affect cAMP-CRP binding. Finally, c-di-GMP did not affect CRP regulatory function, because c-di-GMP did not broadly affect the expression of other CRP-regulated genes. Together these findings indicate that c-di-GMP does not regulate CRP, but regulates another effector that co-regulates gbpA expression.
Several other potential mediators of c-di-GMP inhibition of gbpA transcription were considered. First, we examined the role of NagC. Not only was NagC the only known regulator of gbpA expression , the NagC and CRP regulons were previously linked in E. coli, in which the NagC and CRP orthologues co-regulate the expression of genes in the chitobiose operon . While our results support previous reports indicating that NagC negatively regulates gbpA, this GlcNAc-responsive regulator had no impact on c-di-GMP regulation of gbpA expression. GlcNAc was previously suggested to be a PTS-dependent sugar in V. cholerae, in which case growth with GlcNAc as the sole carbon source would not be expected to activate the cAMP-CRP pathway . However, upregulation of gbpA was observed upon c-di-GMP depletion during growth with GlcNAc, mirroring the results obtained during growth with PTS-independent nutrients. One possible explanation for these results is that gbpA is regulated via multiple mechanisms during growth in GlcNAc (cAMP-CRP, NagC, c-di-GMP, possibly others), making the net gbpA transcription level difficult to predict. Alternatively, GlcNAc, like glucose, may not strictly rely on a PTS for uptake in V. cholerae. Indeed, although certain PTS components are essential for GlcNAc utilization in V. cholerae, a strain deficient in the EIIBGlcNAc transporter (NagE) retains the ability to grow with GlcNAc as the sole carbon source , suggesting that an additional GlcNAc transporter exists in this bacterium. Thus, an alternative pathway for GlcNAc transport would alleviate any impact on the cAMP-CRP pathway.
We directly evaluated three previously defined transcription factors known to bind c-di-GMP in V. cholerae, VpsT, VpsR and FlrA, as potential mediators of gbpA inhibition by c-di-GMP. These regulators were compelling candidates, because gbpA (VCA0811) appeared in transcriptional profiling studies of the respective mutants, with VpsT and VpsR suggested to act as activators and FlrA acting as a repressor [20, 58]. However, none of these transcription factors significantly altered gbpA expression or c-di-GMP regulation of gbpA. The effector that senses c-di-GMP and impinges on gbpA expression remains unidentified.
It is possible that carbon source influences c-di-GMP levels in V. cholerae. Earlier studies showed cross-talk between cAMP and c-di-GMP signaling pathways in V. cholerae. Fong et al. have demonstrated that cAMP-CRP signaling can impact c-di-GMP production by repressing the expression of the DGC cdgA, and accordingly, a crp mutant behaves like a strain with elevated c-di-GMP levels . To our knowledge, our findings are the first to link the regulatory effects of both cAMP and c-di-GMP at a single promoter. Increasing cAMP levels by inactivating the phosphodiesterase CpdA did not alter gbpA expression, suggesting that when CRP is maximally active, c-di-GMP can still inhibit CRP activation of gbpA. We speculate that direct interplay between cAMP-CRP and a c-di-GMP regulated factor may impact gbpA transcription such that maximal CRP-dependent activation of gbpA is apparent under conditions in which cAMP is abundant and c-di-GMP is low. Alternatively, the two regulatory events may be independent, and the effect of c-di-GMP is only observable when cAMP-CRP is present. Additional studies are needed to determine how nutrient availability, cAMP-CRP and c-di-GMP interact to control gbpA expression, and perhaps expression of other genes.
Previous studies have demonstrated a link between the available carbon source and surface colonization by V. cholerae. The ability to respond to PTS carbohydrates is important for binding to chitin, chitin degradation, and chitin-induced competence [54, 66]. The presence of PTS sugars, mutation of the adenylate cyclase gene cyaA, and mutation of crp, each of which reduce or eliminate cAMP-CRP, diminish the ability of V. cholerae to interact with chitin . As GbpA also plays a role in colonization of chitin and intestinal surfaces by V. cholerae [35, 36], it is tempting to speculate that cAMP-CRP links gbpA expression with expression of genes encoding chitin utilization and chitin-induced competence components. In addition, in a germ-free mouse model, V. cholerae requires a functional PTS system to persist in the intestine, indicating that this bacterium relies on PTS carbohydrates during infection . cAMP-CRP also influences expression of numerous other virulence factors of V. cholerae [32, 59, 67, 68]. Thus GbpA is part of the larger cAMP-CRP regulated program central to surface colonization by V. cholerae.
Genetic evidence suggests that V. cholerae modulates intracellular c-di-GMP levels during transitions between its native aquatic environment and the host intestine. Biofilm formation is positively regulated by c-di-GMP, which may enhance V. cholerae survival on chitin and other aquatic surfaces [18, 22, 50]. Indeed, c-di-GMP regulates the production of at least one other chitin binding protein, the hemagglutinin FrhA, and has been demonstrated to promote attachment of V. cholerae to chitin beads . Reduction of c-di-GMP is required to promote bacterial motility and increase expression of virulence factors [21, 49, 69–71], and there is evidence suggesting that V. cholerae may increase c-di-GMP at later stages of infection . Dysregulation of c-di-GMP signaling likely affects the ability of V. cholerae to persist in and transition between these environments.
The data presented here and in previous reports point to an exceedingly complex regulation of GbpA. In addition to derepression of gbpA by NagC in response to GlcNAc, we herein show that high c-di-GMP interferes with cAMP-CRP activation of gbpA transcription. Thus, the net production of GbpA would depend upon the levels of intracellular cAMP and the c-di-GMP. Another layer of GbpA regulation occurs through post-translational hydrolysis of GbpA by two quorum sensing regulated proteases, HapA and PrtV . Cell density-dependent hydrolysis of GbpA may also be linked to second messenger levels. The quorum sensing pathway of V. cholerae influences c-di-GMP levels at least in part through regulation of c-di-GMP metabolism genes [74, 75]. Quorum sensing is also linked to the cAMP-CRP signaling pathway in V. cholerae. CRP impacts the production of the quorum sensing regulator HapR, as well as synthesis of cholera autoinducer 1 [32, 62, 76]. Thus, the c-di-GMP, cAMP and quorum sensing signaling networks are intricately intertwined, leading to complex regulation of GbpA production.
In sum, the transcriptional, post-transcriptional and post-translational regulation of GbpA may allow V. cholerae to fine-tune GbpA production in response to changes in intracellular c-di-GMP concentrations. Importantly, numerous extracellular signals that impact intracellular c-di-GMP and cAMP levels could regulate GbpA production, influencing the ability of V. cholerae to colonize aquatic and host surfaces.
3′-5′ cyclic diguanylic acid, cyclic diguanylate
Cyclic adenosine monophosphate
Cyclic guanosine monophosphate
Guanosine pentaphosphate or tetraphosphate
M9 minimal medium
cAMP receptor protein
Phosphoenolpyruvate-carbohydrate phosphotransferase transport system
Quantitative real-time polymerase chain reaction
Tamayo R, Pratt JT, Camilli A. Roles of cyclic diguanylate in the regulation of bacterial pathogenesis. Annu Rev Microbiol. 2007;61:131–48.
Cotter PA, Stibitz S. c-di-GMP-mediated regulation of virulence and biofilm formation. Curr Opin Microbiol. 2007;10(1):17–23.
Hengge R. Principles of c-di-GMP signalling in bacteria. Nat Rev Microbiol. 2009;7(4):263–73.
Kalia D, Merey G, Nakayama S, Zheng Y, Zhou J, Luo Y, et al. Nucleotide, c-di-GMP, c-di-AMP, cGMP, cAMP, (p)ppGpp signaling in bacteria and implications in pathogenesis. Chem Soc Rev. 2013;42(1):305–41.
Romling U, Galperin MY, Gomelsky M. Cyclic di-GMP: the first 25 years of a universal bacterial second messenger. Microbiol Mol Biol Rev. 2013;77(1):1–52.
Ausmees N, Mayer R, Weinhouse H, Volman G, Amikam D, Benziman M, et al. Genetic data indicate that proteins containing the GGDEF domain possess diguanylate cyclase activity. FEMS Microbiol Lett. 2001;204(1):163–7.
Chang AL, Tuckerman JR, Gonzalez G, Mayer R, Weinhouse H, Volman G, et al. Phosphodiesterase A1, a regulator of cellulose synthesis in Acetobacter xylinum, is a heme-based sensor. Biochemistry. 2001;40(12):3420–6.
Christen M, Christen B, Folcher M, Schauerte A, Jenal U. Identification and characterization of a cyclic di-GMP-specific phosphodiesterase and its allosteric control by GTP. J Biol Chem. 2005;280(35):30829–37.
Ryjenkov DA, Tarutina M, Moskvin OV, Gomelsky M. Cyclic diguanylate is a ubiquitous signaling molecule in bacteria: insights into biochemistry of the GGDEF protein domain. J Bacteriol. 2005;187(5):1792–8.
Tamayo R, Tischler AD, Camilli A. The EAL domain protein VieA is a cyclic diguanylate phosphodiesterase. J Biol Chem. 2005;280(39):33324–30.
Schmidt AJ, Ryjenkov DA, Gomelsky M. The ubiquitous protein domain EAL is a cyclic diguanylate-specific phosphodiesterase: enzymatically active and inactive EAL domains. J Bacteriol. 2005;187(14):4774–81.
Ryan RP, Fouhy Y, Lucey JF, Crossman LC, Spiro S, He YW, et al. Cell-cell signaling in Xanthomonas campestris involves an HD-GYP domain protein that functions in cyclic di-GMP turnover. Proc Natl Acad Sci U S A. 2006;103(17):6712–7.
Boyd CD, O’Toole GA. Second messenger regulation of biofilm formation: breakthroughs in understanding c-di-GMP effector systems. Annu Rev Cell Dev Biol. 2012;28:439–62.
Sudarsan N, Lee ER, Weinberg Z, Moy RH, Kim JN, Link KH, et al. Riboswitches in eubacteria sense the second messenger cyclic di-GMP. Science. 2008;321(5887):411–3.
Kulshina N, Baird NJ, Ferre-D’Amare AR. Recognition of the bacterial second messenger cyclic diguanylate by its cognate riboswitch. Nat Struct Mol Biol. 2009;16(12):1212–7.
Smith KD, Lipchock SV, Ames TD, Wang J, Breaker RR, Strobel SA. Structural basis of ligand binding by a c-di-GMP riboswitch. Nat Struct Mol Biol. 2009;16(12):1218–23.
Lee ER, Baker JL, Weinberg Z, Sudarsan N, Breaker RR. An allosteric self-splicing ribozyme triggered by a bacterial second messenger. Science. 2010;329(5993):845–8.
Lim B, Beyhan S, Meir J, Yildiz FH. Cyclic-diGMP signal transduction systems in Vibrio cholerae: modulation of rugosity and biofilm formation. Mol Microbiol. 2006;60(2):331–48.
Lim B, Beyhan S, Yildiz FH. Regulation of Vibrio polysaccharide synthesis and virulence factor production by CdgC, a GGDEF-EAL domain protein, in Vibrio cholerae. J Bacteriol. 2007;189(3):717–29.
Syed KA, Beyhan S, Correa N, Queen J, Liu J, Peng F, et al. The Vibrio cholerae flagellar regulatory hierarchy controls expression of virulence factors. J Bacteriol. 2009;191(21):6555–70.
Tischler AD, Camilli A. Cyclic diguanylate regulates Vibrio cholerae virulence gene expression. Infect Immun. 2005;73(9):5873–82.
Krasteva PV, Fong JC, Shikuma NJ, Beyhan S, Navarro MV, Yildiz FH, et al. Vibrio cholerae VpsT regulates matrix production and motility by directly sensing cyclic di-GMP. Science. 2010;327(5967):866–8.
Srivastava D, Harris RC, Waters CM. Integration of cyclic di-GMP and quorum sensing in the control of vpsT and aphA in Vibrio cholerae. J Bacteriol. 2011;193(22):6331–41.
Srivastava D, Hsieh ML, Khataokar A, Neiditch MB, Waters CM. Cyclic di-GMP inhibits Vibrio cholerae motility by repressing induction of transcription and inducing extracellular polysaccharide production. Mol Microbiol. 2013;90(6):1262–76.
Klose KE, Novik V, Mekalanos JJ. Identification of multiple sigma54-dependent transcriptional activators in Vibrio cholerae. J Bacteriol. 1998;180(19):5256–9.
Yildiz FH, Dolganov NA, Schoolnik GK. VpsR, a member of the response regulators of the two-component regulatory systems, is required for expression of vps biosynthesis genes and EPS(ETr)-associated phenotypes in Vibrio cholerae O1 El Tor. J Bacteriol. 2001;183(5):1716–26.
Prouty MG, Correa NE, Klose KE. The novel sigma54- and sigma28-dependent flagellar gene transcription hierarchy of Vibrio cholerae. Mol Microbiol. 2001;39(6):1595–609.
Casper-Lindley C, Yildiz FH. VpsT is a transcriptional regulator required for expression of vps biosynthesis genes and the development of rugose colonial morphology in Vibrio cholerae O1 El Tor. J Bacteriol. 2004;186(5):1574–8.
Pratt JT, Tamayo R, Tischler AD, Camilli A. PilZ domain proteins bind cyclic diguanylate and regulate diverse processes in Vibrio cholerae. J Biol Chem. 2007;282(17):12860–70.
Gorke B, Stulke J. Carbon catabolite repression in bacteria: many ways to make the most out of nutrients. Nat Rev Microbiol. 2008;6(8):613–24.
Houot L, Chang S, Absalon C, Watnick PI. Vibrio cholerae phosphoenolpyruvate phosphotransferase system control of carbohydrate transport, biofilm formation, and colonization of the germfree mouse intestine. Infect Immun. 2010;78(4):1482–94.
Liang W, Pascual-Montano A, Silva AJ, Benitez JA. The cyclic AMP receptor protein modulates quorum sensing, motility and multiple genes that affect intestinal colonization in Vibrio cholerae. Microbiology. 2007;153(Pt 9):2964–75.
Fong JC, Yildiz FH. Interplay between cyclic AMP-cyclic AMP receptor protein and cyclic di-GMP signaling in Vibrio cholerae biofilm formation. J Bacteriol. 2008;190(20):6646–59.
Reidl J, Klose KE. Vibrio cholerae and cholera: out of the water and into the host. FEMS Microbiol Rev. 2002;26(2):125–39.
Kirn TJ, Jude BA, Taylor RK. A colonization factor links Vibrio cholerae environmental survival and human infection. Nature. 2005;438(7069):863–6.
Bhowmick R, Ghosal A, Das B, Koley H, Saha DR, Ganguly S, et al. Intestinal adherence of Vibrio cholerae involves a coordinated interaction between colonization factor GbpA and mucin. Infect Immun. 2008;76(11):4968–77.
Meibom KL, Li XB, Nielsen AT, Wu CY, Roseman S, Schoolnik GK. The Vibrio cholerae chitin utilization program. Proc Natl Acad Sci U S A. 2004;101(8):2524–9.
Ghosh S, Rao KH, Sengupta M, Bhattacharya SK, Datta A. Two gene clusters co-ordinate for a functional N-acetylglucosamine catabolic pathway in Vibrio cholerae. Mol Microbiol. 2011;80(6):1549–60.
Plumbridge J, Kolb A. CAP and Nag repressor binding to the regulatory regions of the nagE-B and manX genes of Escherichia coli. J Mol Biol. 1991;217(4):661–79.
Plumbridge J, Kolb A. DNA loop formation between Nag repressor molecules bound to its two operator sites is necessary for repression of the nag regulon of Escherichia coli in vivo. Mol Microbiol. 1993;10(5):973–81.
Yang C, Rodionov DA, Li X, Laikova ON, Gelfand MS, Zagnitko OP, et al. Comparative genomics and experimental characterization of N-acetylglucosamine utilization pathway of Shewanella oneidensis. J Biol Chem. 2006;281(40):29872–85.
Miyashiro T, Klein W, Oehlert D, Cao X, Schwartzman J, Ruby EG. The N-acetyl-D-glucosamine repressor NagC of Vibrio fischeri facilitates colonization of Euprymna scolopes. Mol Microbiol. 2011;82(4):894–903.
Callahan 3rd LT, Ryder RC, Richardson SH. Biochemistry of Vibrio cholerae virulence. II. Skin permeability factor-cholera enterotoxin production in a chemically defined medium. Infect Immun. 1971;4(5):611–8.
Donnenberg MS, Kaper JB. Construction of an eae deletion mutant of enteropathogenic Escherichia coli by using a positive-selection suicide vector. Infect Immun. 1991;59(12):4310–7.
Pratt JT, McDonough E, Camilli A. PhoB regulates motility, biofilms, and cyclic di-GMP in Vibrio cholerae. J Bacteriol. 2009;191(21):6632–42.
McKee RW, Kariisa A, Mudrak B, Whitaker C, Tamayo R. A systematic analysis of the in vitro and in vivo functions of the HD-GYP domain proteins of Vibrio cholerae. BMC Microbiol. 2014;14:272-014-0272-9.
Nomura Y, Yokobayashi Y. Reengineering a natural riboswitch by dual genetic selection. J Am Chem Soc. 2007;129(45):13814–5.
Tamayo R, Patimalla B, Camilli A. Growth in a biofilm induces a hyperinfectious phenotype in Vibrio cholerae. Infect Immun. 2010;78(8):3560–9.
Tamayo R, Schild S, Pratt JT, Camilli A. Role of cyclic di-GMP during el tor biotype Vibrio cholerae infection: characterization of the in vivo-induced cyclic di-GMP phosphodiesterase CdpA. Infect Immun. 2008;76(4):1617–27.
Tischler AD, Camilli A. Cyclic diguanylate (c-di-GMP) regulates Vibrio cholerae biofilm formation. Mol Microbiol. 2004;53(3):857–69.
Miller JH. Experiments in Molecular Genetics. Cold Spring Harbor, NY: Cold Spring Harbor Laboratory Press; 1972.
Mudrak B, Tamayo R. The Vibrio cholerae Pst2 phosphate transport system is upregulated in biofilms and contributes to biofilm-induced hyperinfectivity. Infect Immun. 2012;80(5):1794–802.
Quinones M, Kimsey HH, Waldor MK. LexA cleavage is required for CTX prophage induction. Mol Cell. 2005;17(2):291–300.
Lo Scrudato M, Blokesch M. The regulatory network of natural competence and transformation of Vibrio cholerae. PLoS Genet. 2012;8(6):e1002778.
Morales VM, Backman A, Bagdasarian M. A series of wide-host-range low-copy-number vectors that allow direct screening for recombinants. Gene. 1991;97(1):39–47.
Hellman LM, Fried MG. Electrophoretic mobility shift assay (EMSA) for detecting protein-nucleic acid interactions. Nat Protoc. 2007;2(8):1849–61.
Beyhan S, Tischler AD, Camilli A, Yildiz FH. Transcriptome and phenotypic responses of Vibrio cholerae to increased cyclic di-GMP level. J Bacteriol. 2006;188(10):3600–13.
Beyhan S, Bilecen K, Salama SR, Casper-Lindley C, Yildiz FH. Regulation of rugosity and biofilm formation in Vibrio cholerae: Comparison of VpsT and VpsR regulons and epistasis analysis of vpsT, vpsR and hapR. J Bacteriol. 2006;189(2):388–402.
Skorupski K, Taylor RK. Cyclic AMP and its receptor protein negatively regulate the coordinate expression of cholera toxin and toxin-coregulated pilus in Vibrio cholerae. Proc Natl Acad Sci U S A. 1997;94(1):265–70.
Munch R, Hiller K, Grote A, Scheer M, Klein J, Schobert M, et al. Virtual Footprint and PRODORIC: an integrative framework for regulon prediction in prokaryotes. Bioinformatics. 2005;21(22):4187–9.
Chen B, Liang W, Wu R, Liang P, Kan B. Phenotype microarray screening of carbon sources used by Vibrio cholerae identifies genes regulated by the cAMP receptor protein. Can J Microbiol. 2013;59(7):472–8.
Silva AJ, Benitez JA. Transcriptional regulation of Vibrio cholerae hemagglutinin/protease by the cyclic AMP receptor protein and RpoS. J Bacteriol. 2004;186(19):6374–82.
Chin KH, Lee YC, Tu ZL, Chen CH, Tseng YH, Yang JM, et al. The cAMP receptor-like protein CLP is a novel c-di-GMP receptor linking cell-cell signaling to virulence gene expression in Xanthomonas campestris. J Mol Biol. 2010;396(3):646–62.
Fazli M, O’Connell A, Nilsson M, Niehaus K, Dow JM, Givskov M, et al. The CRP/FNR family protein Bcam1349 is a c-di-GMP effector that regulates biofilm formation in the respiratory pathogen Burkholderia cenocepacia. Mol Microbiol. 2011;82(2):327–41.
Plumbridge J, Pellegrini O. Expression of the chitobiose operon of Escherichia coli is regulated by three transcription factors: NagC, ChbR and CAP. Mol Microbiol. 2004;52(2):437–49.
Blokesch M. Chitin colonization, chitin degradation and chitin-induced natural competence of Vibrio cholerae are subject to catabolite repression. Environ Microbiol. 2012;14(8):1898–912.
Kovacikova G, Skorupski K. Overlapping binding sites for the virulence gene regulators AphA, AphB and cAMP-CRP at the Vibrio cholerae tcpPH promoter. Mol Microbiol. 2001;41(2):393–407.
Li CC, Merrell DS, Camilli A, Kaper JB. ToxR interferes with CRP-dependent transcriptional activation of ompT in Vibrio cholerae. Mol Microbiol. 2002;43(6):1577–89.
Camilli A, Mekalanos JJ. Use of recombinase gene fusions to identify Vibrio cholerae genes induced during infection. Mol Microbiol. 1995;18(4):671–83.
Lee SH, Angelichio MJ, Mekalanos JJ, Camilli A. Nucleotide sequence and spatiotemporal expression of the Vibrio cholerae vieSAB genes during infection. J Bacteriol. 1998;180(9):2298–305.
Tischler AD, Lee SH, Camilli A. The Vibrio cholerae vieSAB locus encodes a pathway contributing to cholera toxin production. J Bacteriol. 2002;184(15):4104–13.
Schild S, Tamayo R, Nelson EJ, Qadri F, Calderwood SB, Camilli A. Genes induced late in infection increase fitness of Vibrio cholerae after release into the environment. Cell Host Microbe. 2007;2(4):264–77.
Jude BA, Martinez RM, Skorupski K, Taylor RK. Levels of the secreted Vibrio cholerae attachment factor GbpA are modulated by quorum-sensing-induced proteolysis. J Bacteriol. 2009;191(22):6911–7.
Waters CM, Lu W, Rabinowitz JD, Bassler BL. Quorum sensing controls biofilm formation in Vibrio cholerae through modulation of cyclic di-GMP levels and repression of vpsT. J Bacteriol. 2008;190(7):2527–36.
Hammer BK, Bassler BL. Distinct sensory pathways in Vibrio cholerae El Tor and classical biotypes modulate cyclic dimeric GMP levels to control biofilm formation. J Bacteriol. 2009;191(1):169–77.
Liang W, Sultan SZ, Silva AJ, Benitez JA. Cyclic AMP post-transcriptionally regulates the biosynthesis of a major bacterial autoinducer to modulate the cell density required to activate quorum sensing. FEBS Lett. 2008;582(27):3744–50.
We would like to thank Kimberly Walker and members of the Tamayo lab for input on these studies. A.K. was supported by an ASM Robert D. Watkins Fellowship. A.G. was supported by NSF REU award DBI-1156840. The funding bodies had no role in the experimental design, in the collection, analysis or interpretation of the data, in the preparation of the manuscript, or in the decision to submit the manuscript for publication.
The authors declare that they have no competing interests.
AK generated strains and performed most experiments. AG performed some western blot analyses. AK and RT analyzed the data and prepared the manuscript. All authors read and approved the final manuscript.
Supplemental Tables S1-S3: (S1) Strains used in this study, (S2) Plasmids used in this study, and (S3) Primers used in this study. (PDF 306 kb)
Supplemental Figures S1 and S2: (S1) Manipulation of c-di-GMP in V. cholerae following ectopic expression of phosphodiesterase genes, and (S2) Growth of V. cholerae reporter strains on various carbon sources. (PDF 252 kb)
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Kariisa, A.T., Grube, A. & Tamayo, R. Two nucleotide second messengers regulate the production of the Vibrio cholerae colonization factor GbpA. BMC Microbiol 15, 166 (2015). https://doi.org/10.1186/s12866-015-0506-5