Characterization of the PAS domain in the sensor-kinase BvgS: mechanical role in signal transmission
© Dupré et al.; licensee BioMed Central Ltd. 2013
Received: 17 April 2013
Accepted: 19 July 2013
Published: 24 July 2013
In bacteria, signal-transduction two-component systems are major players for adaptation to environmental stimuli. The perception of a chemical or physical signal by a sensor-kinase triggers its autophosphorylation. The phosphoryl group is then transferred to the cognate response regulator, which mediates the appropriate adaptive response. Virulence of the whooping cough agent Bordetella pertussis is controlled by the two-component system BvgAS. Atypically, the sensor-kinase BvgS is active without specific stimuli at 37°C in laboratory conditions and is inactivated by the addition of negative chemical modulators. The structure of BvgS is complex, with two tandem periplasmic Venus flytrap domains and a cytoplasmic PAS domain that precedes the kinase domain, which is followed by additional phosphotransfer domains. PAS domains are small, ubiquitous sensing or regulatory domains. The function of the PAS domain in BvgS remains unknown.
We showed that recombinant BvgS PAS proteins form dimers that are stabilized by α helical regions flanking the PAS core. A structural model of the PAS domain dimer was built and probed by site-directed mutagenesis and by biochemical and functional analyses. Although we found no ligands for the PAS domain cavity, its integrity is required for signaling. We also showed that the structural stability of the PAS core and its proper coupling to its flanking N- and C-terminal α helices are crucial for BvgS activity.
We propose that a major function of the BvgS PAS domain is to maintain conformational signals arising from mechanical strain generated by the periplasmic domain. The tight structure of the PAS core and its connections with the upstream and downstream helices ensure signaling to the kinase domain, which determines BvgS activity. Many mild substitutions that map to the PAS domain keep BvgS active but make it unresponsive to negative modulators, supporting that modulation increases conformational strain in the protein.
KeywordsTwo-component system Bordetella Virulence regulation PAS domain Signaling
Two-component systems (TCS) are one of the predominant signal transduction systems in bacteria, which are often essential to enable microorganisms to adapt to changes of their environment . They regulate important developmental programs as well as bacterial virulence in response to environmental stimuli. Typically, they are composed of a transmembrane sensor-kinase protein and a cytoplasmic response regulator. Perception of a chemical or physical signal by the sensor leads to autophosphorylation, and then transfer of the phosphoryl group to the response regulator . Thus activated, the latter mediates a specific, frequently transcriptional, cellular response.
The whooping cough agent Bordetella pertussis colonizes the upper respiratory tract of humans. Its virulence regulon is controlled by the TCS BvgAS. At 37°C and in laboratory growth conditions, the BvgAS system is activated, leading to the transcription of a number of genes coding for virulence factors, necessary for infection . In contrast to most two-component sensor-kinases, BvgS appears to be active in its basal state. Switching to the avirulent Bvg- phase can be triggered by the addition of chemical modulators, such as nicotinate or sulfate ions. However, the authentic negative modulators that might act at specific stage(s) of the bacterium’s life cycle remain to be identified. BvgS is a hybrid sensor-kinase harboring several cytoplasmic domains that mediate a complex phospho-transfer cascade . It also contains three potential perception domains, two periplasmic Venus flytrap (VFT) domains in tandem and a cytoplasmic Per/ArnT/Sim (PAS) domain followed by the kinase domain . We have established that the second VFT domain, VFT2, binds nicotinate and related negative modulator molecules . BvgS is the prototype for VFT-containing sensor-kinases mostly found in Proteobacteria whose molecular mechanisms are poorly understood.
In this work, we characterized the PAS domain of BvgS (PASBvg). PAS domains are structurally conserved, 100- to 120-residue-long signaling modules with sensory and regulatory functions, present in kinases, chemoreceptors and other types of proteins in all branches of the phylogenetic tree [7, 8]. They are composed of a central, five-stranded anti-parallel β sheet flanked by α helices. Many PAS domains appear to form dimers in vitro and in vivo. A subset of PAS domains harbors heme, flavine nucleotide or other cofactors for perception of physical parameters such as light or O2. Some cytoplasmic PAS domains appear to modulate signal transmission rather than to directly perceive a signal [8, 10, 11]. Finally, some PAS domains, including the periplasmic ‘PDC’ (PhoP/DcuS/CitA) domains found in many bacterial TCS sensor-kinases bind small chemical ligands, which triggers signal transduction [12–15]. Although the presence of a PAS domain in BvgS has been recognized for over 20 years [16, 17], its role is still unknown. Here, we show that this domain is required for transmission of signals from the periplasm.
Strains and plasmids
The sequence coding for the PAS core domain was amplified by PCR using the PAScore UP and PAScore LO oligonucleotides as primers (see Additional file 1: Table S1). The amplicon was inserted in pCRII-TOPO (Invitrogen) and sequenced. It was then introduced as a BamHI-HindIII fragment into the corresponding sites of pQE-30 (Qiagen). The resulting plasmid encodes the PASBvg core with an N-terminal His tag. Next, two longer constructs were prepared using the primers PAS His UP and PAS His LO and PAS GB1 UP and PAS GB1 LO. The first amplicon was introduced into pQE30 as a BglII-HindIII fragment, and the other was introduced into pGEV2  as a BamHI-XhoI fragment. The first plasmid codes for PASBvg flanked by its N- and C-terminal helices and with an N-terminal 6-His tag. The second codes for a fusion between the GB1 domain and the same BvgS fragment. Finally, sequences coding for PASBvg recombinant proteins of various lengths were amplified by PCR using a combination of the following primers: PAS N1UP, PAS N2UP or PAS N3UP and PAS C1LO, PAS C2LO or PAS C3LO (Additional file 1: Table S1). The amplicons were restricted as Bsa I fragments, introduced into the corresponding sites of the pASK-IBA35+ vector (IBA) and sequenced. The resulting plasmids encode recombinant PASBvg proteins with an N-terminal His tag in all cases.
Selected residues were replaced by site-directed mutagenesis as described in . Briefly, the Bvg-BglII and Bvg-Xba primers were used with the ‘LO’ and ‘UP’ primers of each pair of mutagenic oligonucleotides to perform overlapping PCRs (Additional file 1: Table S1; the names of the mutagenic oligonucleotides relate to the corresponding substitutions). After verification of the sequences, the mutated fragments were exchanged for their wild type (wt) counterparts in a plasmid that contains most of the bvgAS operon in tandem restriction cassettes . The bvgS sequence coded by that plasmid corresponds to that of Tohama I BP1877, except that a Glu codon is found at position 705, as found in most other B. pertussis strains . The mutations were then introduced into the chromosome of BPSM ∆bvgAS , a Tohama I derivative harboring a large deletion in the bvgAS operon, by using allelic exchange as described . Finally, a ptx-lacZ transcriptional fusion was generated in each of the recombinant strains using pFUS2 .
The virulent BPSME705 strain (wt control) and the avirulent B. pertussis BPSMΔbvgS were described in . BPSMΔbvgA harbour a chromosomal deletion of bvgA. It was constructed by allelic replacement using homologous recombination as follows. DNA fragments flanking the bvgA gene were amplified from the BPSM chromosome using the pairs of oligonucleotides BvgA-UP1 and BvgA-LO1, and BvgA-UP2 and BvgA-LO2, respectively. The amplicons were used as templates for an overlapping PCR, and the resulting amplicon was introduced as an XbaI-HindIII restriction fragment into pSS1129 restricted with the same enzymes . The resulting suicide plasmid was used for allelic replacement as described .
To introduce the substitutions of interest into the recombinant protein, the N2C3 UP and N2C3 LO primers were used to amplify the relevant gene portion from the mutagenized plasmids described above. The amplicons were then introduced into pASK-IBA35+ in the same manner as for the wt gene fragment.
Protein production and purification
Productions of the PASBvgS core from the pQE and pGEV derivatives were performed in Escherichia coli SG13009(pREP4) (Qiagen) and BL21(DE3), respectively. pREP4 harbors a lacI Q gene for repression of the lac promoter prior to induction with IPTG.
A number of conditions were tested to optimize protein production, by varying the temperature of the cultures, the absorbance at 600 nm of the culture at the time of induction, the concentration of inducer and the duration of the induction. Production of the 9 recombinant proteins from the pIBA derivatives was performed in E. coli BL21 (DE3). A number of inductions conditions were also tested, and the following one was identified as the most suitable. A 50-ml overnight culture in LB medium supplemented with 150 μg/ml ampicillin (LB-Amp100) was used to inoculate 1 liter of LB-Amp150 to an OD600 of 0.05. The culture was incubated at 37°C in a rotary shaker at 220 rpm. Expression of recombinant PASBvg was induced at an OD600 of 0.4 by the addition of 200 μg/L anhydrotetracycline (IBA). After 5 h of incubation under the same conditions, the cells were harvested by centrifugation at 8,000 × g for 20 min at 4°C. Hemin (Sigma) or 5-aminolevulinic acid (Sigma) were added at a concentration of 10 mM one hour before induction in the relevant cultures. For N2C3 production at 16°C, the cultures were grown at 37°C until they reached an OD600 of 0.4, then switched to 16°C 30 min before addition of the inducer. Induction was performed for 16 hours.
In all cases, the cell pellets were resuspended in 10 mM Tris–HCl (pH 7.5), 150 mM NaCl, 10 mM imidazole (binding buffer) with 5 μg/ml of DNase I (Sigma) and EDTA-free protease inhibitor cocktail (Roche). Cells were disrupted by three passages in a French pressure cell, and the bacterial debris was removed by centrifugation for 20 min at 10,000 × g. The supernatant was loaded onto a Ni2+-Sepharose affinity column (GE Life Sciences) pre-equilibrated with the binding buffer. Two washing steps were performed by using successively 10 mM and 50 mM of imidazole in the binding buffer, followed by an elution step with 200 mM imidazole. The protein was further purified by gel filtration in 10 mM Tris–HCl (pH 7.5), 150 mM NaCl through a HiLoad 16/60 Superdex 75 column (GE Healthcare). All purification steps were carried out at 4°C or 12°C.
Mass spectrometry analyses were performed on an ESI-Q-TOF spectrometer (Waters, Micromass) in positive ion mode by GIGA Proteomics at the University of Liège, Belgium. Purified N2C3 was used at a concentration of 10 μM in 27 mM ammonium acetate for native conditions, or in 31.25 mM ammonium acetate, 30% acetonitrile and 0.5% formic acid for denaturing conditions.
The delipidation treatment of the purified protein was performed as described in . The protein solution (4 mg/ml) was incubated with 1 ml of LIPIDEX 1000 matrix (Perkin Elmer) previously equilibrated in the gel filtration buffer, for 1 hour at 37°C under gentle agitation. The mixture was centrifuged, and the supernatant was collected and applied to the same amount of fresh LIPIDEX 1000 matrix. The incubation step was performed 6 times in total. Thermal denaturation was performed in 96-wells plate with 15 μl per well of a 30 μM protein solution and 4 × NanoOrange® (Invitrogen) diluted 125 folds from a 500 × stock solution . The plates were heated from 25°C to 85°C with a ramp rate of 0.07°C/s and read by a thermocycler (LightCycler 480 II, Roche) using excitation and emission wavelengths of 465 nm and 510 nm, respectively. The Tms were determined using the LightCycler480 Software. The experiments were performed two or three times at least in triplicate. The statistical analyses were performed using the unpaired t test of the Graphpad PRISM software.
For the crystallogenesis attempts, purified PASBvg proteins (N2C2, N2C3, N3C2 and N3C3) were concentrated using a centrifugal filter unit (Ultracel® 10 kDa membrane, Amicon® Ultra, Millipore, Billerica, MA). Crystallization screening was carried out using the sitting-drop, vapor-diffusion technique in 96-well microplates. Trays were set using a Phenix crystallization robot (Art Robbins instrument) and commercial crystallization kits (HR-Index, HR-AMSO4, HR-Cryst1&2, HR-Cryo from Hampton Research, Nextal-JCSG + from QIAGEN, Proplex and PACT from Molecular Dimensions). The drops were set up by mixing equal volumes (0.1 μl) of the protein and the precipitant solutions equilibrated against 75 μl of the precipitant solution. The protein concentrations ranged from 10 to 80 mg/ml for PASBvg N2C3 and N2C2 and from 10 to 30 mg/ml for PASBvg N3C2 and N3C3.
To prepare the membrane fractions of the various B. pertussis strains, the bacteria were grown in modified Stainer-Scholte medium (SS)  containing 100 μg/ml streptomycin and 10 μg/ml gentamycin. After 24 h at 37°C under rotating agitation (220 rpm) cells were harvested by centrifugation, resuspended in phosphate-buffered saline (PBS) to an OD600 of 5 and broken using a Hybaid Ribolyser apparatus (30 s at speed 6 in tubes containing 0.1 mm silica spheres as the lysing matrix). The lysates were clarified by centrifugation (8000 × g, 10 minutes), and the membrane fractions were pelleted from 1 ml of supernatants by ultracentrifugation (90 000 × g, 1 hour). The pellets were resuspended in 100 μl PBS and used for denaturing electrophoresis in 4-8% gradient polyacrylamide gels (Novex, Life Technologies). The proteins were then transferred electrophoretically to nitrocellulose membranes for immunoblotting. Polyclonal antibodies against BvgS were raised in rats (Eurogentec, Belgium) and used at a 1:500 dilution in PBS + 0.1% Tween 20. The secondary antibody was an anti-rat immunoglobulin- alkaline phosphatase conjugate (Promega) at a 1:7,500 dilution in the same buffer. Revelation of the blots was performed using the BCIP/NBT Color Development Substrate (Promega).
A similarity search using PSI-BLAST  was performed to find suitable templates. Modeller 9v8  was used to build a model of the structure of the PAS domain of BvgS based on 3BWL. The protein side-chain conformations were predicted using SCWRL4 . The quality of the model was assessed using PROSA II . Molecular structure inspections and illustrations were made using PyMOL (PyMOL Molecular Graphics System, version 1.3, Schrödinger).
The various B. pertussis strains harboring specific mutations in bvgS and a ptx-lacZ fusion were grown in modified SS medium containing 100 μg/ml streptomycin and 10 μg/ml gentamycin. After 24 h at 37°C under rotating agitation as above, the bacterial suspension was used to initiate cultures in 10 ml of medium either not supplemented or containing the desired concentration of modulators. The inoculation volume was adapted to compensate for slower growth in the presence of high concentrations of nicotinate. The bacteria were grown until the cultures reached an OD600 of 1.5, harvested by centrifugation, resuspended in Z buffer (60 mM Na2HPO4, 40 mM NaH2PO4, 10 mM KCl, 1 mM MgSO4 and 2,7 ml of 2-mercaptoethanol per liter added immediately before use) to an OD600 of 5 and broken as described above. ß-galactosidase activities were determined as described . The experiments were performed in triplicate, and statistical analyses were conducted as above. The ptx operon codes for pertussis toxin, a virulence factor whose expression is positively regulated by BvgAS. The ptx-lacZ transcriptional fusion interrupts the first gene of the operon and places lacZ under the control of the Bvg-regulated ptx promoter. Thus, the levels of β galactosidase activity measured after growth in virulent, Bvg+ conditions reflect the activity of BvgS, while those under modulating conditions reflect the ability of BvgS to respond to the negative modulators.
Production of recombinant PAS proteins
Among the hundreds of predicted VFT sensor-kinases many, including BvgS, harbor in their cytoplasmic moiety PAS, GAF, receiver or Hpt domains in addition to the His-kinase module . When present, the PAS domain most frequently precedes the kinase domain.
Relevant features of the proteins produced in this work
Calculated MW (Da)#
69.7 ± 0.2
70.5 ± 0.3
63.1 ± 0.2
61.1 ± 0.5
Y596A + N631A
62.3 ± 0.2
60.3 ± 0.6
63.0 ± 0.4
66.8 ± 0.2
60.1 ± 0.1
Thus, recombinant PASBvg produced in E. coli is dimeric, and the flanking helices predicted to form coils that precede and follow the PAS core appear to stabilize it. Most kinases of two–component systems work as dimers, and therefore the finding that the domain immediately preceding the kinase in BvgS also dimerises is not unexpected. In addition, PAS domains of other proteins frequently form dimers. It is thus likely that PASBvg dimerises in the context of the full-length protein as well.
PASBvg structural model
We next attempted to obtain the X-ray structure of recombinant PASBvg. However, none of the four soluble recombinant proteins yielded diffracting crystals in spite of repeated attempts. We therefore searched for a homolog of known structure in the protein structure database, on the basis of which a 3-dimensional model of PASBvg could be built. The closest PAS domain of known structure, PASHm (pdb code: 3BWL), found in an Htr-like protein of Haloarcula marismortui has been crystallized in a structural genomic program. PASHm is dimeric and harbors a long α helix N terminal to the PAS core, like that predicted to link the transmembrane segment and PAS core domain in BvgS. Interestingly, the physico-chemical properties of these N-terminal flanking α helices are very similar between PASHm and PASBvg, with a number of charged residues in both cases. In the full-length protein of H. marismortui, the PASHm domain is followed by a predicted α helix and a histidine-kinase domain, like in BvgS. However, PASHm was crystallized without this C-terminal α helix. The features of PASHm – dimerisation and the presence of flanking helical extensions at both extremities are in agreement with the predictions and available data for PASBvg, indicating that the former represents a reasonable structural template for the latter.
Hypothesis of a heme co-factor
The His643Ala substitution was also introduced into the N2C3 recombinant protein, and the N2C3 variant was purified. Similar to all soluble proteins produced in this work, N2C3His643Ala was dimeric (not shown). Using the thermal shift assay its Tm was determined to be 7°C lower than its wt counterpart (Table 1). Altogether, our data do not support the notion that PASBvg has a heme cofactor. However, His643 appears to be required for BvgS response to negative signals, indicating its functional importance. It also contributes to the thermal stability of recombinant PASBvg.
Role of the PAS cavity
To probe for the presence of another potential co-factor or ligand in the PASBvg cavity, electron spray ionization mass spectrometry was performed in native conditions using the N2C3 variant. This analysis independently confirmed the dimeric nature of the recombinant protein, with a mass of 36,171 ± 3.6 Da, and ruled out the presence of a covalent ligand associated with recombinant PASBvg. A mass spectrometry analysis performed under denaturing conditions yielded a mass of 18,084 ± 1.8 Da, close to the calculated value (18.083 kDa excluding the initiation methionine).
We then targeted other residues of the PASBvg cavity between the inner surface of the β sheet and the helices of the PAS core. These residues were chosen on the basis of the structural model and of sequence alignments. PASBvg harbours a unique Cys residue (Cys607) in a short loop bordering the cavity. Cys residues have been implicated in co-factor binding in other types of PAS (e.g. LOV domains) . In addition, they may be involved in the perception of redox signals , a function that has been proposed for BvgS . The substitution of Cys607 by an Ala residue in full-length BvgS did not modify its basal activity in B. pertussis (Figure 4). Interestingly, BvgSCys607Ala was non-responsive to modulation by nicotinate, whereas it remained responsive to modulation by MgSO4. The responses to other modulators related to nicotinic acid were also tested (not shown). The activity of BvgSCys607Ala was modulated only at much higher modulator concentrations than those required for the wild type control, indicating that this variant has an intermediate rather than a non-responsive modulation phenotype.
The corresponding recombinant protein was produced, purified and analyzed by TSA. Its Tm was 8°C lower than that of wt N2C3 (Table 1). Altogether, these results identified a second residue of the PASBvg cavity whose replacement decreases both the denaturation temperature of the recombinant protein and the ability of BvgS to respond to nicotinic acid and related molecules that are perceived by the periplasmic domain.
The structure of the PAS domain of the Mycobacterium tuberculosis Rv1364c protein (pdb code 3K3C) shows an Arg residue in the cavity that is essential for the binding of a C16-fatty acid ligand . An Arg residue is found in PASBvg at a corresponding position (Arg670), and its side chain appears to be oriented in the same manner in the PASBvg model as that in PASRv1364c (Figure 3). In the latter protein, the ligand was identified only when the recombinant bacteria were grown at low temperatures (16°C) . We therefore purified N2C3 from E. coli grown at 16°C and subjected it to thermal shift analysis before and after delipidation, to test whether the loss of a putative ligand might destabilize the PASBvg domain. However, the Tm of N2C3 was not affected by this treatment, and it was similar to that measured for the protein grown at 37°C (not shown). Similarly, the Tm of the N2C3 protein harboring the Arg670Ala substitution was only moderately decreased compared to that of its wt counterpart (Table 1). We also introduced the Arg670Ala substitution in full-length BvgS, which did not affect its activity in B. pertussis or its ability to respond to negative signals (Figure 4). These observations thus rule out a major function for this residue in PASBvg.
We next determined the effect of the Tyr596Ala + Asn631Ala substitutions on the thermal stability of the recombinant protein. Surprisingly, although N2C3Tyr596Ala+Asn631Ala was purified in a soluble and dimeric form in good amounts, no cooperative denaturation profile was obtained by TSA, and thus no Tm could be calculated. This suggested a significantly looser structure of the PAS core even at lower temperatures. The observations that the joint replacements of Tyr596 and Asn631 in the PASBvg cavity both abolished BvgS activity and considerably destabilized PASBvg argue that the structural stability of the PAS core domain is important for BvgS function. Of note, mutations in the PAS core have been shown to affect the stability and function of other PAS domains as well [35, 36].
PAS coupling with flanking regions
To determine whether these substitutions affected the PASBvg structural integrity, they were introduced into the recombinant N2C3 protein, and the thermal stabilities of the three variants were determined (Table 1). The N2C3Asn608Ala protein was produced in very low amounts, suggesting that the substitution considerably affects its structural integrity. The soluble fraction of the protein was dimeric but had a tendency to precipitate, and therefore it could not be analyzed further. In contrast, the other two proteins were produced in reasonable amounts although lower than that of wt PASBvgS in soluble, dimeric forms, and they were relatively stable over time, suggesting that they were properly folded. Nevertheless, their Tms were more than 10°C lower than that of the corresponding wt protein (Table 1). Thus, disconnecting the PAS domain from the flanking helices both abolishes BvgS activity and significantly decreases the stability of recombinant PASBvg. The loss of BvgS activity seems to correlate with significantly looser PAS domain structures.
Over 20,000 PAS domains have been identified in different proteins. They are essentially involved in regulation or sensing. In the family of VFT-containing sensor-kinases of which BvgS is a prototype, PAS domains are frequently found between the transmembrane segment and the kinase domain. Sequences of the bvgAS locus from a number of B. pertussis, Bordetella bronchiseptica and Bordetella parapertussis isolates have shown the remarkable conservation of the PAS domain in BvgS, supporting the idea that it is functionally important . In this work, we identified specific amino acid residues in the PAS domain whose substitutions abolish BvgS activity. They map to three different locations: at the interfaces between the PAS core and its flanking N-terminal and C-terminal α helices, and in the PAS cavity. These results support a key transmission function for the PAS domain in BvgS, related to its critical position between the periplasmic and kinase domains. The PAS domain in BvgS needs to be tightly folded to fulfill this role, because significantly loosening the PAS core or its connections with upstream and downstream helices dramatically affects BvgS activity.
We found that the PASBvg domain dimerises in E. coli, and we propose that it does so in full-length BvgS as well. Dimer formation is consistent with earlier findings that the kinase domain of BvgS dimerises [39–41]. The increased solubility of recombinant PASBvg proteins containing large portions of the C- and N-terminal flanking α helices argues that the latter contribute to dimer formation, as described for some other PAS domains [42, 43]. The outer surfaces of the β sheet of PAS cores are generally hydrophobic, and in other PAS dimers they participate in the interface or are apposed to flanking helices [8, 13, 44]. This also appears to be the case for PASBvg. The structural model is also in good agreement with proposed mechanisms of signal transmission by other PAS domains, with the β sheet participating in signaling [43, 45, 46]. In the PASBvg model the β sheet is well positioned to relay information to the flanking C-terminal α helix and thus to the kinase domain.
In the current mechanistic model, BvgS is active in its basal state, and this activity requires the integrity of the periplasmic domain, since specific substitutions or insertions in the periplasmic region of BvgS abolish activity [6, 47]. We thus propose that in its basal, non-liganded state the periplasmic domain adopts a conformation that provides a positive signal to the system. The binding of nicotinate to the VFT2 domain modifies this conformation and strongly decreases the positive-signaling capability of the protein . The distinct conformational states of the periplasmic domain most likely impose distinct conformations onto the membrane segment that are propagated via long α helices to the PASBvg domain and from there to the kinase domain underneath. In this work, we found that disruption of the coupling between PASBvg and its upstream or downstream α helices abolishes BvgS activity, as do some of the PAS cavity substitutions. We therefore propose that the conformation of the periplasmic domain generates mechanical strain in BvgS, and that a major function of the PAS domain in BvgS is to maintain, and possibly to amplify, this conformational signal. The complete loss of activity of some BvgS variants generated in this study correlates with strong decreases in thermal stability of the recombinant PAS domain. The corresponding substitutions thus cause considerably looser structures that most likely make the PASBvg domain unable to maintain and/or transmit the proper conformational strain to the kinase. The importance of the PAS core for stability and activity has also been shown for other PAS domains [35, 36].
Another observation from this and previous work is that a number of substitutions in the PAS domain do not inactivate BvgS but render it unresponsive to negative modulation by nicotinate and sulfate [16, 47, 48]. Previously reported substitutions that make BvgS unresponsive to modulation map essentially to a PAS core loop oriented towards the N-terminal flanking helix or to the N-terminal helix itself (Figure 2). It is thus likely that they affect the connection between the PAS core and the upstream region or the stability of the PAS dimer through its N-terminal helices. In the current work, new substitutions that impair or abolish responsiveness to modulation were also identified in the PAS cavity. The structural stabilities of the latter two PASBvg variant proteins appeared to be decreased to a lower extent than those of the inactive proteins. The observation that the unresponsive BvgS PAS variants remain competent to transmit positive but not negative signals suggests that transmission of modulating signals implies an increased conformational strain relative to the basal, positive-signaling state.
Our results do not support the hypothesis that PASBvgS has a heme co-factor. Thus, the His643Ala substitution does not abolish BvgS activity, as would be expected from the loss of an O2-sensing heme for a strictly aerobic and virulent bacterium. However, this substitution abolishes the response of BvgS to negative modulation, and another substitution in the PAS cavity (Cys607Ala) also decreases BvgS sensitivity to nicotinate. These effects might be explained either by a moderate loosening of the PAS core because the small Ala side chain replaces a larger one, which disrupts the transmission of negative signals, or by a defect in binding a potential intracellular ligand required for transmission of negative signals. The double Tyr596Ala + Asn631Ala substitutions in the PAS cavity that abolish BvgS activity and strongly decrease the PAS thermal stability might also disable ligand binding in vivo. Binding of a cytoplamic ligand by the PAS domain would be consistent with the established link between the nutritional state of B. pertussis and its virulence  and with the observations that BvgAS regulates cytochrome expression and might perceive redox signals [17, 50]. Thus, the PASBvg domain might sense intracellular molecule(s) whose abundance reflect(s) the metabolic state of the bacterium, and changes to the concentration of these components might affect signaling. Such a scenario would be compatible with the ‘rheostat’ behavior attributed to BvgS . In any case, the effects of cavity mutations on BvgS activity lend strong support to our model that the conformation of the PAS core –intrinsically or by virtue of ligand binding- is critical for signaling.
Although substantial information has been gathered about how the cytoplasmic domains of BvgS work, the function of its PAS domain has remained unknown. In this work, we performed its characterization, which represents new information that contributes to our understanding of VFT-containing sensor-kinases. We showed that the recombinant PAS domain of the sensor-kinase BvgS dimerises, and that the N- and C-terminal α-helical regions that flank the PAS core are critical for dimer stabilization. We identified specific amino acid residues in the PAS domain that are essential for BvgS activity, located in the PAS core and at the junctions between it and its flanking α helices. We thus propose a mechanical role for the PAS domain in BvgS, which is to maintain the conformational tension imposed by the periplasmic moiety of BvgS. The degree of tension in the protein determines the activity of the kinase, and modulation corresponds to an increased tension. Our model thus explains for the first time the phenotypes of a number of BvgS variants that harbor mild substitutions in the PAS domain and are unable to respond to negative modulation.
Venus flytrap domain
Thermal shift assay
Melting (denaturation) temperature
We thank Eve Willery for the construction of BPSMΔbvgA. E. D. was supported by a pre-doctoral grant from the French Ministry for Research and then by a grant from the Fonds de la Recherche Médicale (FRM). This work was supported by funds from INSERM, CNRS, and University Lille-Nord de France.
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