Search tips
Search criteria 


Logo of jbacterPermissionsJournals.ASM.orgJournalJB ArticleJournal InfoAuthorsReviewers
J Bacteriol. 2013 February; 195(3): 436–443.
PMCID: PMC3554009

Individual and Combined Roles of the Master Regulators AphA and LuxR in Control of the Vibrio harveyi Quorum-Sensing Regulon


Bacteria use a chemical communication process called quorum sensing to control transitions between individual and group behaviors. In the Vibrio harveyi quorum-sensing circuit, two master transcription factors, AphA and LuxR, coordinate the quorum-sensing response. Here we show that AphA regulates 167 genes, LuxR regulates 625 genes, and they coregulate 77 genes. LuxR strongly controls genes at both low cell density and high cell density, suggesting that it is the major quorum-sensing regulator. In contrast, AphA is absent at high cell density and acts to fine-tune quorum-sensing gene expression at low cell density. We examined two loci as case studies of coregulation by AphA and LuxR. First, AphA and LuxR directly regulate expression of the genes encoding the quorum-regulatory small RNAs Qrr2, Qrr3, and Qrr4, the consequence of which is a specifically timed transition between the individual and the group life-styles. Second, AphA and LuxR repress type III secretion system genes but at different times and to different extents. The consequence of this regulation is that type III secretion is restricted to a peak at mid-cell density. Thus, the asymmetric production of AphA and LuxR coupled with differences in their strengths and timing of target gene regulation generate a precise temporal pattern of gene expression.


Bacteria use quorum-sensing-mediated communication to monitor population density and to alternate between individual and group behaviors. Quorum sensing relies on the production of and response to extracellular signaling molecules called autoinducers (AIs) that encode information about the cell density and the species composition of the bacterial community. Vibrio harveyi is a focus of quorum-sensing studies because it has provided the parts list and the regulatory design principles for bacterial communication. V. harveyi produces and detects three AIs, AI-1, CAI-1, and AI-2, that specify intraspecies, intragenus, and interspecies communication, respectively (1). The AIs are detected by three cognate membrane-bound two-component sensor kinase receptors, LuxN, CqsS, and LuxQ (1, 2). LuxQ works in conjunction with LuxP, a periplasmic binding protein (3).

At low cell density (LCD), when AI concentrations are low, the receptors act as kinases, shuttling phosphate through the quorum-sensing cascade to the response regulator LuxO. Phosphorylated LuxO (LuxO~P) activates the transcription of genes encoding five regulatory small RNAs (sRNAs), called Qrr1 to Qrr5 (49). The Qrr sRNAs control the production of the two quorum-sensing master transcription factors, AphA and LuxR (Fig. 1). The base pairing of the Qrr sRNAs to aphA mRNA induces its translation (10, 11), whereas the base pairing of the Qrr sRNAs to luxR mRNA causes its degradation (7, 9). Thus, at LCD, AphA is maximally produced, and LuxR is minimally produced (10). This pattern is reinforced by the AphA repression of luxR transcription at LCD. Under this condition, V. harveyi cells act as individuals.

Fig 1
Model for the alternating pattern of LuxR and AphA control of the quorum-sensing regulon. (Left) At LCD, a low AI concentration results in the production of LuxO~P, which activates qrr gene expression. The Qrr sRNAs repress the translation of ...

At high cell density (HCD), when AIs have accumulated, the AIs bind to their cognate receptors, causing them to switch from kinases to phosphatases, which results in the dephosphorylation of LuxO. In the absence of LuxO~P, the transcription level of the qrr genes is reduced, and this relieves the repression of luxR and decreases the activation of aphA (Fig. 1). Consequently, maximal LuxR production and minimal AphA production occur, a pattern that is reinforced by LuxR repressing the transcription of aphA (12, 13).

LuxR and AphA can both activate and repress gene expression (10, 13). LuxR and its homologs, for example, HapR in Vibrio cholerae and SmcR in Vibrio vulnificus, are members of the TetR family of transcriptional regulators (12). At HCD, LuxR controls genes including luxCDABE (luciferase), the type III secretion system (TTSS) genes, qrr2, qrr3, qrr4, and aphA (10, 1217). A previous reporter screen revealed that LuxR regulates over 50 promoters at HCD in V. harveyi (13). This screen was not saturated because known targets, such as luxCDABE, were not identified. AphA is a winged-helix transcription factor that controls virulence factor production in V. cholerae (18, 19). In V. harveyi, AphA was recently shown to regulate the expression of 296 genes at LCD, including luxR, qrr2, qrr3, and qrr4 (10).

Here we determine the individual and combined contributions of AphA and LuxR to quorum-sensing target gene expression in V. harveyi. Our biochemical analysis shows that, consistent with previous genetic predictions, the AphA and LuxR proteins exhibit reciprocal production patterns in response to changes in AI levels. These production profiles are, however, asymmetric: AphA is produced at LCD, but no AphA protein can be detected at HCD. LuxR is, in contrast, present throughout the growth curve but at higher concentrations at HCD than at LCD. Thus, AphA functions exclusively at LCD, while LuxR functions to different extents throughout growth. Microarrays and quantitative real-time PCR (qRT-PCR) demonstrate that AphA and LuxR control genes in distinct regulons, and they also coregulate 77 genes. To understand coregulation by AphA and LuxR, we examined two sets of these shared targets: the qrr sRNA genes and the TTSS genes. We find that LuxR and AphA both bind to and control the expression of the qrr promoters. The activation of the qrr genes by LuxR and the repression of the qrr genes by AphA precisely control Qrr sRNA levels during quorum-sensing transitions. Second, LuxR and AphA both bind to and repress the expression of TTSS genes, resulting in minimal TTSS gene expression at both LCD and HCD and a spike of TTSS gene expression at mid-cell density. Thus, the asymmetric production profiles of AphA and LuxR coupled with their individual and combined control of downstream regulatory targets establish a finely choreographed pattern of quorum-sensing gene expression.


Bacterial strains and media.

Escherichia coli strains S17-1λpir, BL21(DE3) (Invitrogen), and derivatives (see Table S1 in the supplemental material) were grown with shaking at 37°C in Luria-Bertani (LB) medium unless otherwise stated. V. harveyi strain BB120 (BAA-1116) and derivatives (see Table S1 in the supplemental material) were grown with shaking at 30°C in Luria-Marine (LM) (20) medium. Antibiotics (Sigma) were used at concentrations described previously (10). Conjugation was used to transfer plasmids from E. coli into V. harveyi (10). Protein production from plasmids containing the Ptac promoter and the theophylline riboswitch was induced with 1 mM isopropyl-β-d-thiogalactopyranoside (IPTG) and 1 mM theophylline, respectively.

Molecular methods.

E. coli strain S17-1λpir was used for cloning procedures. Restriction enzymes, T4 polynucleotide kinase, T4 DNA ligase, and calf intestinal phosphatase were purchased from New England BioLabs (NEB). PCR mixtures contained iProof DNA polymerase (Bio-Rad). Plasmids containing the Ptac promoter, lacI, and the theophylline riboswitch were constructed by using pSAL12.1, a kind gift of the Gallivan laboratory (21), as described in Table S2 in the supplemental material. Oligonucleotides (Integrated DNA Technologies) are listed in Table S3 in the supplemental material. Plasmid constructs were introduced into electrocompetent E. coli S17-1λpir cells by using 0.2-cm Bio-Rad cuvettes. Sequences were confirmed by Genewiz, Inc., with plasmid-specific primers. The construction of mutations in V. harveyi was performed as previously described (10).

RNA was isolated from bacterial cultures by using the TRIzol (Invitrogen) method, as described previously (10). cDNA synthesis and qRT-PCR were performed as described previously (10), using primers listed in Table S3 in the supplemental material. Reactions were normalized to an internal standard (hfq) and analyzed by using the standard curve or ΔΔCT method. Western blot experiments were conducted as previously described (11, 17). Methods describing AphA and LuxR protein purification and DNA binding assays are included in the supplemental material.

Electrophoretic mobility shift assays (EMSAs).

Oligonucleotides (see Table S3 in the supplemental material) were purchased from Integrated DNA Technologies (PAGE purified). Complementary substrates were annealed in annealing buffer (50 mM Tris-HCl [pH 7.5], 100 mM NaCl) at 95°C for 1 min, followed by cooling 1°C per min for 70 min. Substrates generated by PCR were purified by gel extraction followed by QIAquick columns (Qiagen). Substrates were labeled with [γ-32P]ATP in 30-μl reaction mixtures containing T4 polynucleotide kinase (NEB) for 30 min at 37°C and cleaned on ProbeQuant G-50 microcolumns (GE Healthcare). Labeled DNA was incubated for 30 min in a 15-μl reaction mixture containing binding buffer (10 mM HEPES [pH 7.5], 100 mM KCl, 2 mM dithiothreitol [DTT], 200 μM EDTA), 10 ng/μl poly(dI-dC), 100 μg/ml bovine serum albumin (BSA), and the desired protein (AphA or LuxR) diluted in dilution buffer (10 mM Tris-HCl [pH 7.5], 10 mM NaCl, 1 mM EDTA, 0.1 mM DTT, and 20% glycerol). The reaction mixtures were separated on 6% TGE (25 mM Tris, 0.25 M glycine, 1 mM EDTA)-polyacrylamide native gels, and the gels were dried at 80°C for 45 min and exposed overnight on a storage phosphor screen. The screen was scanned by using a Typhoon scanner and analyzed both qualitatively and quantitatively by using ImageQuant software (GE Healthcare).

Time course analyses of gene expression.

Cultures of V. harveyi strains grown overnight were diluted ~1:1,000 in LM medium, and aliquots were collected at the time points noted. Samples were also collected from the cultures grown overnight to determine RNA levels at the initial time points. Transcript levels were analyzed by Quanti-gene Plex technology, as described previously (22), or RNA was collected and analyzed by qRT-PCR or microarrays.

AI-1 titration experiments.

Cultures of strains TL25 (ΔluxM ΔluxPQ ΔcqsS), YS10 (ΔluxM ΔluxPQ ΔcqsS ΔluxR), YS50 (ΔluxM ΔluxPQ ΔcqsS ΔaphA), or YS51 (ΔluxM ΔluxPQ ΔcqsS ΔaphA ΔluxR) grown overnight were diluted to an optical density at 600 nm (OD600) of 0.001 with various concentrations of AI-1 added. Cells were collected at an OD600 of 1.0 for RNA extraction and protein sample preparation.

Inducible expression of luxR and aphA.

The inducible expression of luxR and aphA was accomplished by constructing a plasmid (pJV025) that contained regulatory elements to control transcription and translation. The plasmid harbors lacIq and contains the Ptac promoter with a LacIq operator site that is sensitive to IPTG. The theophylline riboswitch aptamer (21) from pSAL12.1 was inserted into the 5′ untranslated region (5′-UTR), which results in the repression of translation in the absence of theophylline. FLAG-luxR and FLAG-aphA were cloned under the control of this “Ptactheo” promoter to yield pJV057 and pSTR738, respectively. To induce aphA and luxR expression, V. harveyi strains were diluted 1:1,000, grown to an OD600 of ~0.2, and induced with 1 mM IPTG and 1 mM theophylline, and samples were collected after 3 h. To monitor gene expression at LCD, cultures grown overnight in the presence of 1 mM IPTG were diluted 1:1,000 and grown to an OD600 of ~0.02 in 1 mM IPTG and 1 mM theophylline.

Microarray analyses.

RNA from V. harveyi strains was collected from cells grown in LM medium to an OD600 of ~1.2 in triplicate. The synthesis of cDNA and the microarray protocol were described previously (10). V. harveyi BB120 microarrays (Agilent) were designed as custom gene expression arrays (Amadid design ID 037644), using the melting temperature (Tm) method and the best-probe method. The arrays contained two 60-mer probes per open reading frame. Gene expression data were averaged from probes that were above background levels, as determined by Feature Extractor (Agilent); had P values of <0.0001; and differed by more than 2-fold in three out of four of the arrays. Data analysis was performed with the Princeton University Microarray Database (PUMAdb) ( These data are publically available at PUMAdb.


LuxR and AphA have asymmetric production profiles.

AphA and LuxR are the two master transcriptional regulators of quorum sensing. Thus, the precise patterns of AphA and LuxR production should govern the downstream pattern of quorum-sensing gene expression. To investigate AphA and LuxR production throughout quorum sensing, we measured the relative aphA and luxR transcript and AphA and LuxR protein production profiles at different AI concentrations. In this experiment, we used a V. harveyi strain (TL25 [ΔluxM ΔluxPQ ΔcqsS]) that does not produce AI-1 but responds to it when it is supplied exogenously. We applied different AI-1 concentrations to V. harveyi TL25 cells to mimic specific quorum-sensing states. The reason why we used strain TL25 rather than the wild type is because it is not possible to collect enough protein under LCD conditions to reliably perform Western blot analyses. We found that aphA levels decreased and luxR levels increased with increasing AI-1 concentrations (Fig. 2). Protein levels tracked with their corresponding mRNA levels (Fig. 2). LuxR could be detected even in the absence of AI-1, whereas AphA decreased to undetectable levels at AI-1 concentrations above 333 nM. These experiments demonstrate that AphA and LuxR exhibit opposite, but nonequivalent, alterations in production during V. harveyi quorum sensing, and this asymmetry is controlled by AIs. Importantly, and we return to this point below, AphA and LuxR are both present at LCD.

Fig 2
AphA and LuxR production profiles during quorum sensing. Shown are data for qRT-PCR of aphA and luxR and Western blot analyses of AphA and LuxR in V. harveyi TL25 (ΔluxM ΔluxPQ ΔcqsS) cells grown in the presence of various concentrations ...

LuxR and AphA are master regulators of quorum sensing.

To define the individual and combined contributions of AphA and LuxR to quorum-sensing target gene expression, we used microarray analyses. We compared profiles from V. harveyi mutant strains that constitutively mimic the LCD and HCD states. The LCD V. harveyi strain harbors a LuxO~P mimic, LuxO D47E (6, 9). The HCD V. harveyi strain is a ΔluxO strain (9). Microarray analyses revealed that levels of 365 transcripts differed by 2-fold or more in these two strains, and we refer to this set of genes as the “quorum-sensing regulon” (see Table S4 and Fig. S1 in the supplemental material). To identify the LCD genes controlled by AphA, we compared the expression profile of a luxO-D47E ΔluxR strain to that of a luxO-D47E ΔluxR ΔaphA strain. This “AphA LCD regulon” contains 167 genes (Fig. 1, left circle; see also Table S4 and Fig. S1 in the supplemental material). To identify the HCD genes controlled by LuxR, we compared the profile of a ΔluxO ΔaphA strain to that of a ΔluxO ΔaphA ΔluxR strain and discovered 625 genes. We call this set the “LuxR HCD regulon” (Fig. 1, right circle; see also Table S4 and Fig. S1 in the supplemental material). Interestingly, the AphA LCD regulon and the LuxR HCD regulon each include genes that are not members of the quorum-sensing regulon. Likewise, not all of the quorum-sensing regulon genes are contained in the AphA or LuxR regulons. Possible explanations for these results are provided in the Discussion.

A comparison of the AphA LCD regulon with the LuxR HCD regulon showed that 77 genes with a variety of predicted functions are controlled by both transcription factors (Table 1 and Fig. 1). Within this set of genes and the individual AphA and LuxR regulons, we identified all eight possible patterns of gene regulation by AphA and/or LuxR. There are genes activated exclusively by LuxR (306 genes, e.g., luxC), repressed exclusively by LuxR (242 genes, e.g., VIBHAR_05222, a putative thioesterase), activated exclusively by AphA (45 genes, e.g., VIBHAR_05936, a hypothetical protein), or repressed exclusively by AphA (45 genes, e.g., VIBHAR_02308, a hypothetical protein). There are also genes activated by LuxR and AphA (7 genes, e.g., VIBHAR_03648, pyrI, a putative aspartate carbamoyltransferase regulatory subunit), genes repressed by LuxR and AphA (52 genes, e.g., exsD, a TTSS transcription regulator), genes repressed by LuxR and activated by AphA (8 genes, e.g., VIBHAR_04884, a hypothetical protein), and genes activated by LuxR and repressed by AphA (10 genes, e.g., VIBHAR_02509, a homolog of V. cholerae hapA). A representative of each class of gene is shown in Fig. S1 in the supplemental material. To confirm these results, we performed complementation experiments by expressing either aphA or luxR from an inducible promoter in a V. harveyi ΔaphA ΔluxR mutant strain (STR417), followed by qRT-PCR of the target genes (see Fig. S2 in the supplemental material). In most cases, complementation occurred. However, in a few cases, regulatory patterns different than expected occurred, suggesting that factors in addition to AphA and LuxR must be involved in controlling these genes (for example, hapA [see Fig. S2 in the supplemental material]).

Table 1
Functional classes of genes coregulated by AphA and LuxRb

As noted above, asymmetry exists in the LuxR and AphA protein production profiles (Fig. 2). Specifically, although LuxR is maximally produced at HCD, it is also present at LCD, whereas little or no AphA is present at HCD. The microarrays showed that LuxR regulates the expression of 82 genes at LCD, while AphA has no influence on gene regulation at HCD (see Table S4 and Fig. S1 in the supplemental material). Collectively, our results favor a model in which LuxR controls genes at both HCD and LCD, while AphA regulates genes predominantly at LCD.

LuxR and AphA direct global gene expression patterns.

A curious finding was that over 50 genes are repressed by AphA at LCD and repressed by LuxR at HCD (see, for example, the TTSS genes, represented by exsD, in Fig. S1 in the supplemental material). Thus, we wondered, When are such genes expressed? To explore this and other possible interesting coregulation patterns, we used microarrays to monitor the expression levels of all 77 target genes that are controlled by both AphA and LuxR using V. harveyi strains possessing and lacking luxR and/or aphA (see Fig. S3 in the supplemental material). We found that genes repressed by both AphA and LuxR are maximally expressed in the window between LCD (OD600 of ~0.01) and HCD (OD600 of ~1.0). For example, consider the TTSS operons (see exsD in Fig. 3A). The full repression of exsD at LCD requires both AphA and LuxR at LCD, whereas only LuxR is necessary for repression at HCD. In other instances, the opposing effects of AphA and LuxR offset each other; for example, take the case of hapA (Fig. 3B). In this example, AphA repression is significantly stronger than is LuxR activation, leading to overall increasing hapA expression levels over growth. Because of this difference, the expression profile of hapA in the V. harveyi ΔaphA ΔluxR mutant strain is more similar to that in the ΔaphA single mutant than to that in the ΔluxR single mutant. For genes that are controlled roughly equally but in opposite directions by AphA and LuxR, the deletion of either aphA or luxR results in altered gene expression, but the deletion of both factors restores expression to nearly the wild-type pattern (VIBHAR_02311, a hypothetical protein, is AphA repressed and LuxR activated) (Fig. 3C). Thus, employing both AphA and LuxR in the quorum-sensing cascade enables patterns of gene expression that would not be possible if only a single transcription factor was involved.

Fig 3
AphA and LuxR coregulate genes during transitions between LCD and HCD. Expression profiles of representative genes at the indicated cell densities are shown. qRT-PCR was used to compare RNA samples collected from the wild-type (BB120), ΔaphA (JV48), ...

Direct coregulation of the qrr4 promoter by LuxR and AphA.

Because the Qrr sRNAs are central quorum-sensing regulators responsible for conveying the information encoded by AIs to the target gene output, we examined their control by AphA and LuxR in some detail. Using qrr4 as the representative, we investigated whether regulation requires both AphA and LuxR. We engineered a V. harveyi strain lacking both aphA and luxR, reintroduced inducible aphA and inducible luxR individually on plasmids, and measured qrr4 expression levels. LuxR activated qrr4 expression 2.4-fold independently of AphA, and AphA repressed qrr4 expression 2.9-fold independently of LuxR (Fig. 4A).

Fig 4
Regulation of qrr4 by AphA and LuxR. (A) qrr4 levels were measured by qRT-PCR. Samples were collected from strains expressing FLAG-luxR (pJV057) or FLAG-aphA (pSTR738) in a V. harveyi ΔluxR ΔaphA strain (STR417). RNA measurements were ...

The finding that LuxR and AphA can individually regulate qrr4 expression does not exclude the possibility that they influence each other's function at the qrr4 promoter when both are present. Therefore, we examined whether both transcription factors could simultaneously bind to the qrr4 promoter. LuxR binds to the 21-bp palindrome TTCTGATAAATGTATTAGTAG located 166 bp upstream of the qrr4 transcription start site (Fig. 4B) (12). We found that AphA binds the 16-bp sequence TTGCATCATTTTGCAT located 125 bp upstream of the qrr4 transcription start site (Fig. 4B; see also Fig. S4 in the supplemental material). This AphA binding sequence shares a low level of identity (6 identical base pairs) with the AphA site characterized previously for V. cholerae (23, 24). We performed EMSAs with a probe harboring both the LuxR and AphA binding sites. LuxR and AphA each bound this DNA fragment (Fig. 4C), which is consistent with their ability to individually control qrr4 expression (Fig. 4A). In the presence of both LuxR and AphA, a DNA supershift occurred, indicating that both transcription factors can simultaneously bind the fragment (Fig. 4C).

To determine how LuxR and AphA together affect in vivo qrr4 expression, we monitored qrr4 expression as wild-type, ΔaphA, and ΔluxR V. harveyi cells transitioned from LCD to HCD. In the wild-type strain, following dilution into fresh medium, the qrr4 expression level increased ~5-fold at LCD (OD600 of ~0.01), and the expression level subsequently decreased 6-fold as cells transitioned to HCD (OD600 of ~1.0) (Fig. 4D). The deletion of aphA prolonged the maximal expression of qrr4 relative to that in wild-type V. harveyi. This result shows that AphA is responsible for setting the timing of the transition to HCD by repressing qrr expression. The deletion of luxR, in contrast, resulted in only modestly reduced levels of qrr4 compared to those of the wild-type strain at LCD (Fig. 4D). This result shows that in wild-type V. harveyi, sufficient LuxR is present at LCD to activate qrr4 expression immediately after the transition to LCD occurs, suggesting that LuxR is responsible for the rapid entrance into the LCD mode.

AphA and LuxR directly control regulation of the TTSS genes.

A second interesting case of coregulation by AphA and LuxR concerns the TTSS genes. We showed that TTSS genes are repressed by both AphA and LuxR, which confines their expression to a peak at mid-cell density (Fig. 3A; see also Table S4 and Fig. S5 in the supplemental material) (10, 13, 17). Here we investigate how this regulatory pattern is coordinated by AphA and LuxR. There are four TTSS structural operons in V. harveyi, TTSS.I to TTSS.IV (Fig. 5A), and these are activated by the regulators ExsA and ExsB (17). exsA and exsB lie upstream of the TTSS.IV operon (Fig. 5A) (13, 17). We first examined whether LuxR and AphA directly bind the promoters driving the expression of the TTSS genes using EMSAs with purified LuxR and AphA proteins. Using the LuxR position weight matrix reported previously (12), we predicted that two LuxR binding sites exist in PB (the exsB promoter) (positions −63 and +5 relative to the transcription start site) and that three exist in PA (the exsA promoter) (positions −115, +187, and +259 relative to the transcription start site) (Fig. 5A), and indeed, LuxR bound DNA fragments containing each of the predicted binding sites (Fig. 5B). A previous study did not find that LuxR bound at the site predicted at position −63 in PB (25). We assume that this discrepancy is due to different EMSA reaction conditions. LuxR did not bind to the TTSS.IV, TTSS.II/III, or TTSS.I promoter fragments (see Fig. S6 in the supplemental material). We do not yet have a position weight matrix to predict AphA binding sites. However, using fragments encompassing the entire promoter regions, we found that AphA also bound the PA and PB promoter fragments (Fig. 5C). Additionally, AphA bound the TTSS.IV and TTSS.I promoter fragments (Fig. 5C) but not the TTSS.II/III promoter fragment (see Fig. S6 in the supplemental material). Complementation experiments showed that the expression of either aphA or luxR causes the repression of both exsA and exsB (Fig. 5D) and all four TTSS structural operons in V. harveyi (see Fig. S5 in the supplemental material). Collectively, our data suggest that AphA (at LCD) and LuxR (at both LCD and HCD) directly repress exsA and exsB expression, and this leads to decreased expression levels of the four TTSS structural operons. In addition, AphA directly represses TTSS.I and TTSS.IV at LCD. The combined effect of this repression is a peak of TTSS expression levels between LCD and HCD.

Fig 5
AphA and LuxR directly repress TTSS genes and protein secretion. (A) Schematic of the TTSS operons in V. harveyi. Promoters (P) are indicated for the two regulators exsA (PA) and exsB (PB) and the four structural operons (PTTSS.1 to PTTSS.IV): TTSS.I ...

The ultimate output of the TTSS operons is a set of secreted proteins. To show that the transcriptional regulatory pattern generated by LuxR and AphA culminates in corresponding changes in protein levels, we monitored the production of the TTSS effector protein VopD using the AI-1-sensing strain (TL25) in the absence of AI-1 (LCD) or in the presence of saturating AI-1 concentrations (HCD). VopD is present at LCD, and it is undetectable at HCD (Fig. 5E). The deletion of aphA resulted in increased VopD levels only at LCD, whereas the deletion of luxR increased VopD levels at both LCD and HCD (Fig. 5E).


V. harveyi uses two master transcription factors, AphA and LuxR, to regulate target genes underpinning individual and group behaviors. Here we demonstrate that AphA and LuxR individually and jointly regulate ~700 genes to specify these alternative life-styles. In response to AI, the first transcripts to change are those of aphA and luxR (data not shown). Specifically, the aphA expression level decreases and the luxR expression level increases within 15 min. This finding suggests that a priority in quorum sensing is to alter the levels of these two master transcription factors in order to promote the subsequent pattern of downstream gene expression. Several putative transcription factors exist among the AphA and LuxR target genes, and these secondary regulators could be responsible for linking the immediate AphA and LuxR responses to gene expression changes that occur later in the quorum-sensing cascade.

AphA acts at LCD, and LuxR acts at both LCD and HCD.

AphA is present at LCD and at the transition to HCD, during which time it controls the expression of 167 genes. Ninety of these genes are regulated exclusively by AphA (i.e., not by LuxR), indicating that these genes encode functions that must be activated or repressed when there are few cells in the population. LuxR is present at both LCD and HCD. Eighty-two genes are controlled by LuxR at LCD, and 75 of these are also controlled by LuxR at HCD. We predict that these 82 LuxR targets harbor the highest-affinity LuxR binding sites because they are controlled by LuxR when it exists at its lowest levels. These 82 genes and the additional 543 HCD LuxR targets likely encode functions that are important for carrying out group behaviors (activated) or that are detrimental to collective activities (repressed).

Quorum-sensing genes that are regulated independently of AphA and LuxR.

A comparison of the LCD-locked strain (luxO-D47E) to the HCD-locked strain (ΔluxO) shows that the entire quorum-sensing regulon consists of 365 genes. Regulation by AphA and/or LuxR accounts for 78% of the differences between these two strains. However, 79 genes in the quorum-sensing regulon are not controlled by LuxR or AphA (see Fig. S1 in the supplemental material). This result suggests that additional factors are involved in quorum-sensing gene regulation. The most obvious candidates for carrying out this regulation are the Qrr sRNAs. Currently, the expression levels of only four genes are known to be controlled by the Qrr sRNAs in V. harveyi (luxR, aphA, luxO, and luxM), and one additional target has been identified in V. cholerae (vca0939) (9, 10, 22, 26, 27). Some of the 79 genes that we identified could be under Qrr control, and we are currently investigating this possibility.

AphA- and LuxR-controlled targets that are not members of the quorum-sensing regulon.

We identified 429 genes that are under LuxR and/or AphA control that are not members of the quorum-sensing regulon (see Fig. S1 in the supplemental material). There are at least two possible explanations for these results. First, the regulation of some genes might be uncovered only in the complete absence of the transcription factor, i.e., in the ΔaphA or the ΔluxR deletion strain. If low levels of LuxR or low levels of AphA are sufficient to control gene expression, such genes will not be revealed in microarrays comparing the ΔluxO and luxO-D47E strains because residual LuxR and AphA exist. An example of this type of target is VIBHAR_06500 to VIBHAR_06505 (VIBHAR_06500-06505), which are activated 9-fold by LuxR at LCD and 6-fold by LuxR at HCD (see Table S4 in the supplemental material). A second explanation for our identification of AphA- and LuxR-controlled genes that are not members of the quorum-sensing regulon is that some genes are controlled by LuxR or AphA only during the quorum-sensing transition, so their steady-state LCD and HCD levels are roughly identical. Again, these genes would not be revealed in our microarray experiments. An example is VIBHAR_01372, which is repressed 4-fold by LuxR at HCD and 3-fold by AphA at LCD (see Table S4 in the supplemental material).

Two unequal master regulators.

We identified 77 genes that are regulated by both AphA and LuxR. Because each transcription factor can act as a repressor and as an activator, there are four possible combinations of coregulation, and we identified at least one example of each: both factors repress, both factors activate, AphA activates and LuxR represses, and AphA represses and LuxR activates. The largest class of genes controlled by both AphA and LuxR is the repressed/repressed class, which contains the TTSS operons.

Generally, LuxR regulation is stronger than that of AphA. For example, consider the TTSS.I operon, which is repressed 3-fold by AphA at LCD and repressed 21-fold by LuxR at HCD. If the role of LuxR overwhelms that of AphA, why employ AphA? We propose that AphA regulation ensures fine-tuned expression at LCD. Another interesting set of genes are VIBHAR_02040-02042, which are activated ~7.5-fold by LuxR at both LCD and HCD. If the expression of these genes must be modulated, another factor, such as AphA, must accomplish this task. Indeed, AphA represses VIBHAR_02040-02042 3-fold at LCD. Thus, AphA can serve to control genes at specific points in the V. harveyi life cycle when regulation by LuxR is insufficient.

Regulation of the TTSS genes by AphA and LuxR.

TTSSs encode important virulence factors in pathogens, including Vibrio parahaemolyticus, Salmonella enterica serovar Typhimurium, and Pseudomonas aeruginosa (17, 28, 29). We found that maximal TTSS gene expression in V. harveyi is confined to the window of growth between LCD and HCD (Fig. 3A). Our model is that at LCD, high levels of AphA combined with low LuxR levels are required for repression. Conversely, at HCD, a high LuxR concentration is sufficient for the repression of the TTSS operons. Precise temporal control of virulence gene expression may be critical to optimize infectivity, in this case by limiting expression to particular cell densities. We do not know why maximal TTSS gene expression at the LCD-to-HCD transition is optimal for V. harveyi pathogenesis. Interestingly, another virulence factor, HapA, is also regulated by both AphA and LuxR.

Generation of global patterns of gene expression.

Multiple feedback loops involving the Qrr sRNAs control the flow of information through the quorum-sensing circuit (9, 16, 22). AphA represses and LuxR activates qrr expression. Additionally, AphA and LuxR repress each other's expression (Fig. 1). These feedback loops are critical to maintain the appropriate levels of the Qrr sRNAs during the transitions from HCD to LCD and from LCD to HCD. We propose a model for how these feedback loops could affect the transitions. First, consider the HCD-to-LCD transition when there is an immediate need to terminate group behaviors. The activation of the qrr genes is a function of LuxO~P and LuxR. LuxO phosphorylation occurs on a time scale of seconds, so qrr activation by LuxO~P is immediate. Residual LuxR protein that accumulated at HCD (Fig. 2) further activates qrr gene expression. The surge in Qrr production represses luxR expression, thus ending the HCD program. The Qrr sRNAs activate aphA expression, which initiates the LCD program. AphA ensures that the LCD program is undertaken by transcriptionally repressing luxR.

During the opposite transition from LCD to HCD, AIs lead to decreased concentrations of LuxO~P and thus to decreased levels of Qrr sRNA production. Therefore, the level of LuxR production increases and the level of AphA production decreases. Residual AphA continues to repress qrr expression, causing a more rapid termination of the LCD program than if AphA was not a part of the program. The LuxR repression of aphA ensures a commitment to HCD. This model predicts that the deletion of aphA should extend Qrr sRNA production and slow the progression to HCD, which is indeed borne out by our results (Fig. 4D).

We suspect that the main advantage of having two rather than one master regulator concerns response kinetics. That said, once the system possesses both AphA and LuxR, adding additional binding sites for either or both of these transcription factors is an economical mechanism to achieve an even finer regulation of particular targets. Furthermore, employing two regulators could allow the integration of environmental cues, in addition to the quorum-sensing autoinducers, into the control of gene expression. Ultimately, because maximal productions of AphA and LuxR occur at distinct times (AphA at LCD and LuxR at HCD), individual regulation and coregulation by AphA and LuxR establish complex gene expression patterns that could not be achieved if only one of these regulators was a member of the quorum-sensing cascade.

Supplementary Material

Supplemental material:


We thank Justin Gallivan for generously providing the theophylline riboswitch plasmid (pSAL12.1). We thank Donna Storton, Jessica Buckles, and John Matese for assistance with microarray experiments and analyses. We also thank Ned Wingreen for helpful comments and suggestions.

PUMAdb is funded in part by NIH grant P50 GM071508 and is a project within the Lewis-Sigler Institute for Integrative Genomics at Princeton University. This work was supported by the Howard Hughes Medical Institute, National Institutes of Health (NIH) grant 5R01GM065859, NIH grant 5R01AI054442, National Science Foundation (NSF) grant MCB-0343821 to B.L.B., NIH fellowship F32AI085922 to S.T.R., and NIH fellowship F32GM089019 to J.C.V.K.


Published ahead of print 30 November 2012

Supplemental material for this article may be found at


1. Ng WL, Bassler BL. 2009. Bacterial quorum-sensing network architectures. Annu. Rev. Genet. 43:197–222. [PubMed]
2. Henke JM, Bassler BL. 2004. Three parallel quorum-sensing systems regulate gene expression in Vibrio harveyi. J. Bacteriol. 186:6902–6914. [PMC free article] [PubMed]
3. Bassler BL, Wright M, Silverman MR. 1994. Multiple signalling systems controlling expression of luminescence in Vibrio harveyi: sequence and function of genes encoding a second sensory pathway. Mol. Microbiol. 13:273–286. [PubMed]
4. Bassler BL, Wright M, Showalter RE, Silverman MR. 1993. Intercellular signalling in Vibrio harveyi: sequence and function of genes regulating expression of luminescence. Mol. Microbiol. 9:773–786. [PubMed]
5. Bassler BL, Wright M, Silverman MR. 1994. Sequence and function of LuxO, a negative regulator of luminescence in Vibrio harveyi. Mol. Microbiol. 12:403–412. [PubMed]
6. Freeman JA, Bassler BL. 1999. A genetic analysis of the function of LuxO, a two-component response regulator involved in quorum sensing in Vibrio harveyi. Mol. Microbiol. 31:665–677. [PubMed]
7. Lenz DH, Mok KC, Lilley BN, Kulkarni RV, Wingreen NS, Bassler BL. 2004. The small RNA chaperone Hfq and multiple small RNAs control quorum sensing in Vibrio harveyi and Vibrio cholerae. Cell 118:69–82. [PubMed]
8. Lilley BN, Bassler BL. 2000. Regulation of quorum sensing in Vibrio harveyi by LuxO and sigma-54. Mol. Microbiol. 36:940–954. [PubMed]
9. Tu KC, Bassler BL. 2007. Multiple small RNAs act additively to integrate sensory information and control quorum sensing in Vibrio harveyi. Genes Dev. 21:221–233. [PubMed]
10. Rutherford ST, van Kessel JC, Shao Y, Bassler BL. 2011. AphA and LuxR/HapR reciprocally control quorum sensing in vibrios. Genes Dev. 25:397–408. [PubMed]
11. Shao Y, Bassler BL. 2012. Quorum-sensing non-coding small RNAs use unique pairing regions to differentially control mRNA targets. Mol. Microbiol. 83:599–611. [PMC free article] [PubMed]
12. Pompeani AJ, Irgon JJ, Berger MF, Bulyk ML, Wingreen NS, Bassler BL. 2008. The Vibrio harveyi master quorum-sensing regulator, LuxR, a TetR-type protein is both an activator and a repressor: DNA recognition and binding specificity at target promoters. Mol. Microbiol. 70:76–88. [PMC free article] [PubMed]
13. Waters CM, Bassler BL. 2006. The Vibrio harveyi quorum-sensing system uses shared regulatory components to discriminate between multiple autoinducers. Genes Dev. 20:2754–2767. [PubMed]
14. Swartzman E, Silverman M, Meighen EA. 1992. The luxR gene product of Vibrio harveyi is a transcriptional activator of the lux promoter. J. Bacteriol. 174:7490–7493. [PMC free article] [PubMed]
15. Miyamoto CM, Smith EE, Swartzman E, Cao JG, Graham AF, Meighen EA. 1994. Proximal and distal sites bind LuxR independently and activate expression of the Vibrio harveyi lux operon. Mol. Microbiol. 14:255–262. [PubMed]
16. Tu KC, Waters CM, Svenningsen SL, Bassler BL. 2008. A small-RNA-mediated negative feedback loop controls quorum-sensing dynamics in Vibrio harveyi. Mol. Microbiol. 70:896–907. [PMC free article] [PubMed]
17. Henke JM, Bassler BL. 2004. Quorum sensing regulates type III secretion in Vibrio harveyi and Vibrio parahaemolyticus. J. Bacteriol. 186:3794–3805. [PMC free article] [PubMed]
18. Skorupski K, Taylor RK. 1999. A new level in the Vibrio cholerae ToxR virulence cascade: AphA is required for transcriptional activation of the tcpPH operon. Mol. Microbiol. 31:763–771. [PubMed]
19. De Silva RS, Kovacikova G, Lin W, Taylor RK, Skorupski K, Kull FJ. 2005. Crystal structure of the virulence gene activator AphA from Vibrio cholerae reveals it is a novel member of the winged helix transcription factor superfamily. J. Biol. Chem. 280:13779–13783. [PMC free article] [PubMed]
20. Rickard AH, Palmer RJ, Jr, Blehert DS, Campagna SR, Semmelhack MF, Egland PG, Bassler BL, Kolenbrander PE. 2006. Autoinducer 2: a concentration-dependent signal for mutualistic bacterial biofilm growth. Mol. Microbiol. 60:1446–1456. [PubMed]
21. Lynch SA, Gallivan JP. 2009. A flow cytometry-based screen for synthetic riboswitches. Nucleic Acids Res. 37:184–192. [PMC free article] [PubMed]
22. Tu KC, Long T, Svenningsen SL, Wingreen NS, Bassler BL. 2010. Negative feedback loops involving small regulatory RNAs precisely control the Vibrio harveyi quorum-sensing response. Mol. Cell 37:567–579. [PMC free article] [PubMed]
23. Kovacikova G, Lin W, Skorupski K. 2003. The virulence activator AphA links quorum sensing to pathogenesis and physiology in Vibrio cholerae by repressing the expression of a penicillin amidase gene on the small chromosome. J. Bacteriol. 185:4825–4836. [PMC free article] [PubMed]
24. Kovacikova G, Lin W, Skorupski K. 2005. Dual regulation of genes involved in acetoin biosynthesis and motility/biofilm formation by the virulence activator AphA and the acetate-responsive LysR-type regulator AlsR in Vibrio cholerae. Mol. Microbiol. 57:420–433. [PubMed]
25. Waters CM, Wu JT, Ramsey ME, Harris RC, Bassler BL. 2010. Control of the type 3 secretion system in Vibrio harveyi by quorum sensing through repression of ExsA. Appl. Environ. Microbiol. 76:4996–5004. [PMC free article] [PubMed]
26. Teng SW, Schaffer JN, Tu KC, Mehta P, Lu W, Ong NP, Bassler BL, Wingreen NS. 2011. Active regulation of receptor ratios controls integration of quorum-sensing signals in Vibrio harveyi. Mol. Syst. Biol. 7:491 doi:10.1038/msb.2011.30. [PMC free article] [PubMed]
27. Hammer BK, Bassler BL. 2007. Regulatory small RNAs circumvent the conventional quorum sensing pathway in pandemic Vibrio cholerae. Proc. Natl. Acad. Sci. U. S. A. 104:11145–11149. [PubMed]
28. Yahr TL, Wolfgang MC. 2006. Transcriptional regulation of the Pseudomonas aeruginosa type III secretion system. Mol. Microbiol. 62:631–640. [PubMed]
29. Angot A, Vergunst A, Genin S, Peeters N. 2007. Exploitation of eukaryotic ubiquitin signaling pathways by effectors translocated by bacterial type III and type IV secretion systems. PLoS Pathog. 3:e3 doi:10.1371/journal.ppat.0030003. [PMC free article] [PubMed]

Articles from Journal of Bacteriology are provided here courtesy of American Society for Microbiology (ASM)