Original Research ARTICLE
Structural and Functional Characterization of the FadR Regulatory Protein from Vibrio alginolyticus
- 1Department of Medical Microbiology and Parasitology, Zhejiang University School of Medicine, Hangzhou, China
- 2Institute of Biophysics, Chinese Academy of Sciences, Beijing, China
- 3School of Life Sciences, Fujian Agriculture and Forestry University, Fuzhou, China
- 4Department of Microbiology, Nanjing Agricultural University, Nanjing, China
- 5Department of Microbiology, Perelman School of Medicine, University of Pennsylvania, Philadelphia, PA, United States
- 6Department of Biochemistry and Biophysics, University of North Carolina at Chapel Hill, Chapel Hill, NC, United States
The structure of Vibrio cholerae FadR (VcFadR) complexed with the ligand oleoyl-CoA suggests an additional ligand-binding site. However, the fatty acid metabolism and its regulation is poorly addressed in Vibrio alginolyticus, a species closely-related to V. cholerae. Here, we show crystal structures of V. alginolyticus FadR (ValFadR) alone and its complex with the palmitoyl-CoA, a long-chain fatty acyl ligand different from the oleoyl-CoA occupied by VcFadR. Structural comparison indicates that both VcFadR and ValFadR consistently have an additional ligand-binding site (called site 2), which leads to more dramatic conformational-change of DNA-binding domain than that of the E. coli FadR (EcFadR). Isothermal titration calorimetry (ITC) analyses defines that the ligand-binding pattern of ValFadR (2:1) is distinct from that of EcFadR (1:1). Together with surface plasmon resonance (SPR), electrophoresis mobility shift assay (EMSA) demonstrates that ValFadR binds fabA, an important gene of unsaturated fatty acid (UFA) synthesis. The removal of fadR from V. cholerae attenuates fabA transcription and results in the unbalance of UFA/SFA incorporated into membrane phospholipids. Genetic complementation of the mutant version of fadR (Δ42, 136-177) lacking site 2 cannot restore the defective phenotypes of ΔfadR while the wild-type fadR gene and addition of exogenous oleate can restore them. Mice experiments reveals that VcFadR and its site 2 have roles in bacterial colonizing. Together, the results might represent an additional example that illustrates the Vibrio FadR-mediated lipid regulation and its role in pathogenesis.
The Vibrionaceae is a family of Gram-negative bacteria inhabiting fresh/salt water environments that comprised a collection of pathogenic species (Thompson et al., 2005). V. cholerae is the notorious cause of cholera transmitted by contaminated water. V. parahaemolyticus is a zoonotic pathogen that cause serious food-borne infections from poorly-cooked sea-food (e.g., gastroenteritis and septicemia). Both V. vulnificus and V. alginolyticus are opportunistic bacterial pathogens since they cause severe wound infection and even fatal septicemia. The two major virulence determinants of Vibrio cholerae referred to toxin-coregulated pilus (TCP) (Taylor et al., 1987) and cholera toxin (CT) (Matson et al., 2007), which are coordinated by two independent activators ToxR, a transmembrane regulatory protein (Miller et al., 1987), and ToxT, a member of AraC family transcription factors (Champion et al., 1997). It seems true that the regulated expression of fatty acid metabolism is implicated into Vibrio pathogenicity in that (i) inactivation of fadR impairs virulence of V. vulnificus in mice (Brown and Gulig, 2008); (ii) the disruption of fadD gene encoding a long-chain fatty acyl coenzyme A ligase affected production of virulence factors, CtxAB and TcpA (Ray et al., 2011); and (iii) unsaturated fatty acids from bile interfered with bacterial mobility via remodeling bacterial membrane structure (Giles et al., 2011) and inhibited the expression of virulence factors (CtxAB and TcpA) by decreased DNA-binding activity of ToxT in V. cholerae (Brown and Gulig, 2008; Giles et al., 2011; Yang et al., 2013; Kovacikova et al., 2017). More recently, Kovacikova et al. (2017) proposed that the V. cholerae FadR controls the expression of the virulence cascade by indirect-regulation of ToxT via two different mechanisms (Kovacikova et al., 2017). In contrast to the E. coli FadR paradigm, its Vibrio homologs with an insert of 40 aa exhibit stronger ability of binding LC acyl-CoA thioesters (Heidelberg et al., 2000; Iram and Cronan, 2005). The structural mechanism of V. cholerae FadR relies on an additional acyl-CoA ligand binding site formed mainly by the 40-residue insert (Shi et al., 2015).
The paradigm E. coli FadR regulator, belonging to a GntR-type transcription factor, is a dimeric protein that is composed of an N-terminal DNA-binding motif and a C-terminal ligand-interaction domain (van Aalten et al., 2000, 2001; Xu et al., 2001). The E. coli FadR acts as a moderate global regulator in that it negatively regulates more than 12 fad genes [such as fadBA (Iram and Cronan, 2006), fadM (Feng and Cronan, 2009a), fadH (Feng and Cronan, 2010), etc.] and it positively regulates, the two key genes (fabA and fabB) of UFA synthesis (Henry and Cronan, 1992; Campbell and Cronan, 2001). In addition, FadR also activates the fabHDG operon required for SFA synthesis in E. coli (My et al., 2013). The physiological ligand of FadR is LC fatty acyl-CoA thioesters. Upon FadR binding of these ligands, FadR is released from all its DNA-binding sites (Henry and Cronan, 1992; Cronan, 1997). This mechanism explains the fatty acid-inducible expression of fad regulon (Overath et al., 1969; Klein et al., 1971) plus the fatty acids-mediated repression of fabA/fabB expression (Henry and Cronan, 1991; Campbell and Cronan, 2001). Although the structural basis for E. coli FadR regulation is well understood from the x-ray crystal structures of E. coli FadR alone (van Aalten et al., 2000), bound DNA (van Aalten et al., 2001; Xu et al., 2001) and in a complex with its ligand myristoyl-CoA (van Aalten et al., 2001), further investigations unexpectedly suggested that FadR orthologs display appreciable functional diversity (Iram and Cronan, 2005) in that FadR proteins from diverse Y-proteobacteria showed large differences in the ability to regulate E. coli fad regulon.
In views of genomic context of lipid metabolism (Figure 1), the Vibrio species, like V. cholerae, seem quite different from E. coli (and S. enterica) because they have two chromosomes that together encode all the enzymes of fatty acid metabolism. Unlike the paradigm “FadL-FadD” fatty acid transport system in E. coli, Vibrio encodes three fadL orthologs only one of which has the FadR-binding site recognized by Vibrio (Figure 1A) (Heidelberg et al., 2000). This might facilitate more efficient scavenging low level of fatty acids from the dilute marine environment (van den Berg et al., 2004). Relative to E. coli which has 12 FadR-regulated genes (Figures 1B–E), the predicted FadR-binding palindrome is detected in only 7 Vibrio genes including 5 known fad/fab genes, suggesting contraction of fad regulon (Figures 1F,G) (Zhang et al., 2015; Gao et al., 2016). Of note, the Vibrio plsB gene is under FadR control (Figures 1F,G), whereas the E. coli counterpart has no effect on this gene (Feng and Cronan, 2011). In contrast to the FadR of E. coli and S. enterica, all the three Vibrio FadR proteins (ValFadR for V. alginolyticus, VcFadR for V. cholerae and VpFadR for V. parahaemolyticus) consistently have an unusual insert of 40 residues (Figure S1), one of which had already been demonstrated to constitute an additional ligand-binding site in the case of VcFadR (Shi et al., 2015). It explains at least (if not all) why V. cholerae has potent ability in fatty acid sensing.
Figure 1. Working model for Vibrio FadR-mediated fatty acid sensing and regulation. (A) Schematic representative for uptake and activation of long-chain fatty acids by FadL-FadD system of V. cholerae N16961. The long-chain fatty acids are transported by FadL membrane protein from the environment into periplasm and then activated by inner-membrane associated protein FadD to give LC acyl-CoA in cytosol. Among three putative FadR homologs encoded by V. cholerae N16961 genome, FadL2 (in red) is only one gene with a predicted FadR-binding site. LCFA is an abbreviation of long chain fatty acid. (B) Sequence logo for FadR-specific palindromes from E. coli MG1655. (C) Sequence logo for FadR-specific palindromes from Vibrio genus. The sequences of the known E. coli FadR sites were sampled from E. coli K-12 MG1655 (http://regprecise.lbl.gov/RegPrecise/regulon.jsp?regulon_id=10286), and the putative Vibrio FadR sites were collected from 9 Vibrio species (http://regprecise.lbl.gov/RegPrecise/sites.jsp?regulog_id=1762) (Novichkov et al., 2013). (D) E. coli FadR represses fad expression, but activates transcription of fabA/B and iclR on the condition without acyl-CoA thioesters. (E) Presence of long chain acyl-CoAs releases E. coli FadR protein from its cognate targets, resulting in an induction of fad expression and transcriptional inactivation of fabA/B and iclR. (F) Vibrio FadR represses the expression of limited fad members, whereas only activates fabA transcription on the condition with poor acyl-CoA species. (G) The generated long chain acyl-CoAs releases Vibrio FadR protein from its cognate targets, which consequently induces the expression of limited fad members, whereas only inactivates fabA transcription. The three representative genes (vc2105, fadBA, and fabA) are highlighted in bold and italic letters, whose ability of binding the Vibrio FadR regulator is demonstrated with EMSA (and/or SPR). The gray oval denotes E. coli FadR regulatory protein whereas the green oval denotes Vibrio FadR regulator. The small red circle represents the acyl-CoA pool. E. coli FadR has only one ligand-binding site in each monomer, whereas Vibrio FadR has two ligand-binding sites in each monomer.
Given that knowledge of fatty acid metabolism in V. alginolyticus is limited, here we report structural and functional characterization of V. alginolyticus FadR. The snapshot of the ValFadR-ligand complex structure also illustrates an additional ligand-binding site. Mice infection experiments suggest that both FadR and the second ligand-binding site might be required for bacterial successful colonization. Together, these results constitute an additional example facilitating us to further understand Vibrio fatty acid signaling by FadR and its relevance to bacterial virulence. It is rational that development of small molecule inhibitors targeting the FadR-mediated fatty acid sensing might be a promising strategy against Vibrio infections.
Characterization of the V. alginolyticus FadR
We are interested in probing if similar scenarios occur in V. alginolyticus. Thus, four types of FadR proteins (namely ValFadR, VcFadR, VpFadR, and EcFadR), were over-expressed and purified with nickel-affinity column, whose purity was judged by SDS-PAGE (Figure S2C). Size exclusion analyses confirmed that all the three Vibrio FadR proteins (ValFadR and VpFadR, in Figure S2A; VcFadR in Figure S2B) can form dimeric structure in solution, which is almost identical to that of EcFadR (Figure S2A). Together with surface plasmon resonance (SPR)-based detection, EMSA experiments were also applied to address binding abilities of the putative Vibrio FadR palindromes (Figures 1C,F,G). A 54 bp of DNA fragment covering the FadR palindrome in the upstream of the Vibrio fabA gene is designated herein as fabA probe. In general agreement with that of EcFadR (Figure 2A), gel shift assays also confirmed that the fabA probe interacts efficiently with ValFadR (Figure 2D). Similar scenarios were also seen with the other two Vibrio FadR regulatory proteins VcFadR (Figure 2B) and VpFadR (Figure 2C). Of note, super-shift bands appeared in the cases of VcFadR (Figure 2B) and ValFadR (Figure 2D). In addition, surface plasmon resonance (SPR) results showed clearly that the fabA probe binds to both EcFadR (Figure 3A) and ValFadR (Figure 3B) in the dose-dependent manner. The binding affinity of fabA to EcFadR and ValFadR is estimated to be 5.59 × 10−7 M (Figure 3A) and 2.58 × 10−7 M (Figure 3B), respectively. Indeed, we recently extended fad regulon to a newly-identified auxiliary fad member, vc2105 of V. cholerae (equivalent to vp0834 of V. parahaemolyticus) (Novichkov et al., 2013; Gao et al., 2016). Therefore, we believed that ValFadR is functional and its regulatory role is relatively-conserved (Figure 1).
Figure 2. Binding of fabA to four types of FadR regulatory proteins. (A) Gel filtration analyses for interaction of EcFadR with fabA. (B) Use of EMSA assays to detect interplay between fabA and VcFadR. (C) EMSA-based analyses for interaction of fabA with VpFadR. (D) Physical evidence for binding of ValFadR to fabA. The gel shift experiments were carried out using 9% native PAGE, and a representative result from no less than three independent experiments is given. In each assay (15 μl in total), the fabA probe (5 pmol) is supplemented, and varied level of FadR protein is indicated in the right hand five lanes of each panel (left to right) (2, 5, 10, 15, and 20 pmol). The four types of FadR proteins referred to EcFadR, VcFadR, VpFadR and ValFadR, respectively. The minus sign denotes the absence of FadR protein. FadR protein at high level precipitates easily in the wells of gel or triggers super-shift in the gel shift experiments.
Figure 3. SPR-based assays for binding of fabA to the FadR regulator. (A) SPR analysis of the E. coli FadR binding to the fabA promoter. (B) SPR assay for the V. alginolyticus FadR binding to the fabA promoter. SPR assays were conducted to study the affinity and kinetics of FadR proteins and a representative result is given regarding to EcFadR and ValFadR. FadR protein at various concentrations (typically 31.25–1,000 nM) were injected over the immobilized DNA probe covering the FadR palindrome of fabA gene. The immobilization level of fabA is 34 RU. KD, kd/ka, ka, association constant; kd, disassociation constant; RU, response units.
Distinct Ligand-Binding Manner of ValFadR and EcFadR
Consistent with earlier observations with EcFadR (Feng and Cronan, 2010, 2012) and VcFadR (Feng and Cronan, 2011), in vitro gel shift assays illustrated that only Long-chain fatty acyl-CoA species [e.g., palmitoyl-CoA (C16:0), palmitoleyl-CoA (C16:1), stearoyl-CoA (C18:0), and oleoyl-CoA (C18:1), in Figure S3] release the ValFadR protein from its cognate DNA, whereas the medium-chain fatty acyl-CoA thioesters [such as nonanoyl-CoA (C9:0) and decanoyl-CoA (C10:0)] cannot. However, it is not clear why the Vibrio FadR and EcFadR differ greatly in the amplitude of fatty acid sensing. Given that isothermal titration calorimetry (ITC) can give clues to different binding modes of small molecules to a certain protein and the equilibrium dissociation constants (Kds), we adopted the ITC method to monitor palmitoyl-CoA (C16:0) ligand binding to the three Vibrio FadR proteins (plus EcFadR) (Figure 4, Figure S4). Comparative analyses of the ITC profiles clearly showed that each EcFadR monomer binds palmitoyl-CoA ligand at the ratio of 1:1 (Figure 4A), which is consistent with the scenario seen with structure of E. coli FadR liganded with myristoyl-CoA (Figures 6A,B) (van Aalten et al., 2001). In contrast, each monomer of ValFadR bound 2 molecules of palmitoyl-CoA (Figure 4B). As anticipated, the similar ligand-binding pattern was also seen in VcFadR (Figure S4A) and VpFadR (Figure S4B). In addition, the ITC measurements showed that the binding of Vibrio FadRs (VcFadR, VpFadR, and ValFadR) palmitoyl-CoA (Figure 4B, Figure S4) are 4- to 10-fold higher than that of EcFadR (Figure 4A) [the value of Kd1 exhibited appreciably lower (3.17-fold for ValFadR (Figure 4B), 7.07-fold for VcFadR (Figure S4A), and 5.06-fold for VpFadR (Figure S4B)]. Obviously, it was consistent with the fact that Vibrio FadR is a much more efficient regulator than E. coli FadR (Iram and Cronan, 2005). Together, our ITC findings suggested that ligand-binding of Vibrio FadR is in a manner distinct from that of EcFadR (Figure 4, Figure S4), which is consistent with the scenario seen in structure of VcFadR reported by Shi et al. (Shi et al., 2015).
Figure 4. ITC-based evidence for distinct binding pattern of the palmitoyl-CoA ligand to FadR regulatory protein from E. coli and Vibrio alginolyticus. (A) ITC profile of the E. coli FadR binding its ligand palmitoyl-CoA. (B) The use of ITC to assay interplay between the V. alginolyticus FadR and its ligand palmitoyl-CoA. Ec, E. coli; Val, V. alginolyticus.
Overall Architecture of ValFadR
In our pilot trials of protein crystal screening, only the ValFadR amongst the three Vibrio FadR proteins (VcFadR, VpFadR, and ValFadR) is successful. The structure of apo-ValFadR was determined at 2.35 Å (Table 1). In an agreement with those of our gel filtration (Figure S2), ValFadR forms a dimer and belongs to space group of P43212, in which each asymmetric unit contains one FadR protomer (Table 1, Figures 7A,D). Solution structure of dimer is consistent with the previously-reported EcFadR (van Aalten et al., 2000) and VcFadR (Shi et al., 2015) (Figure 5, Figure S5). The analyses of structural superposition suggested that overall architecture of ValFadR (Figure 5B) can match well that of VcFadR (Figures 5A,C). The protomer is composed of two functional domains, the N-terminal DNA-binding domain, the C-terminal ligand-binding domain and one linker connecting these two domains (Figure S5). The N-terminal DNA-binding domain adopts a typical wHTH fold motif and includes three α helices (α1, α2, α3) and two β strands (β1 and β2) (Figures S1, S5). The C-terminal ligand binding domain forms an α-helix bundle and includes eight helices (Figures S1, S5). Sequence alignment revealed that ValFadR has more 40 residues (138–177 aa) insertion between helices α6 and α7 than EcFadR (Figure S1). The ValFadR structure shows that these 40 residues elongate helices α7, and form two helices, αA and αB, and some linking loops (Figures S1, S5B,E), which is generally similar to that of VcFadR alone (Figure 5) (Shi et al., 2015). Except the insert of 40 residues, the structure of apo-ValFadR (Figures S5B,E) is highly similar to that of apo-EcFadR (Figures S3A,D) with r.m.s.d over 223 Cα atoms (one protomer) of 1.5 Å (Figures S5C,F).
Figure 5. Structural comparison of the FadR proteins of V. cholerae and V. alginolyticus. (A) Ribbon structure of the dimeric FadR protein of V. cholerae. (B) X-ray structure of the V. alginolyticus FadR protein in dimer. (C) Structural superposition of the two FadR proteins from V. alginolyticus and V. cholerae. Vc, V. cholerae; Val, V. alginolyticus.
Structure of ValFadR Liganded with Palmitoyl-CoA
Unlike the fact that VcFadR was complexed with the ligand oleoyl-CoA (Shi et al., 2015), we obtained the crystal of ValFadR-liganded with palmitoyl-CoA that was diffracted by X-ray to 2.4 Å (Table 1). The asymmetric unit contains one ValFadR dimer and four palmitoyl-CoA molecules, in a 1:2 stoichiometry (Figures 6C, 7B,E) as reported for VcFadR (Shi et al., 2015), whereas EcFadR binds one molecule of ligand (myristoyl-CoA) per monomer (Figures 6A,D). It fully validated the general conclusion from the aforementioned ITC experiments (Figure 4, Figure S4). The two ligand-binding sites in ValFadR are similar to those observed with VcFadR (Figure S6) (Shi et al., 2015). One of the ligand molecules binds to ValFadR in the site that is equivalent to EcFadR ligand-binding site (designated site 1), and the second ligand binds to the pocket derived in part from the 40-residue insertion region. The site 1 is mainly formed by the C-terminal domain (Figures S6A,B), whereas the site 2 is formed by both the N- and C-domains (Figures S6C,D). The electron density of the acyl group in the ligand in site 1 is well defined whereas the phosphorylated adenosine head group is not clear (Figures S6A,B). The phosphorylated adenosine head of the palmitoyl-CoA ligand in one protomer interacts with several residues from the other protomer, including hydrogen bonds between Arg245 and the phosphate group. The pyrophosphate group interacts with residues of both Arg253 and Tyr115 via hydrogen bonds (Figures S6A,B). For the ligand in site 2, the phosphorylated adenosine head group is well defined in electron density while the acyl group lack this ability (Figures S6C,D). The phosphorylated adenosine head group inserts into the pocket derived from the part of the 40-residue insertion region. Among it, the adenosine group stacks with residues Tyr153 and Met187 and forms hydrogen bond with Asn130 and Tyr184. The phosphate group forms hydrogen bond with residue Lys156 and the pyrophosphate forms hydrogen bond with residues Arg126 and Arg191 (Figures S6C,D).
Figure 6. Chemical structures of the representative FadR ligands and structural comparison of the liganded-ValFadR with the EcFadR-ligand complex structure. (A) Chemical structures of LC fatty acyl-CoAs, the ligands for FadR regulatory proteins. The palmitoyl-CoA ligand that was successfully crystalized into the FadR protein is highlighted in orange, whereas the double bond is indicated in blue. (B) Complex structure of the monomeric form of EcFadR liganded with myristoyl-CoA ligand. The architecture of the EcFadR (PDB: 1H9G) is shown in blue cylinder, whereas the ligand of myristoyl-CoA is given in orange stick. (C) Complex structure of the monomeric form of ValFadR liganded with palmitoyl-CoA ligand (PDB: 5DV5). The protomer form of ValFadR is shown in cyan cylinder, and the extra-40aa insert is given in magenta. The ligands are shown in sticks, one of which is of light green in the binding site 1 and the other one present in site 2 is indicated in red. (D) Superposition of the monomeric structure of ValFadR-ligand and EcFadR-ligand structure via their C-terminal ligand-binding domains.
Figure 7. Structural comparison of the apo- and ligand bound-FadR protein from V. alginolyticus. Monomeric (A) and dimeric (D) structures of apo-ValFadR protein are shown in magenta cylinder (PDB: 5XGF). Protomer (B) and dimeric (E) structures of ligand-bound ValFadR protein are shown in cyan cylinder (PDB: 5DV5). The monomeric (C) and dimeric (F) structures of the apo- and ligand-bound ValFadR protein are superposed via their C-terminal ligand-binding domains. The ligand in binding site 1 is shown in gray spheres and the other one in binding site 2 is indicated with orange spheres. Val, V. alginolyticus; N, N-terminus of the FadR protein; C, C-terminus of the FadR protein.
Structural comparison revealed that the C-terminal domain of ValFadR is distinctly varied from that of EcFadR-ligand complex structure (Figure 6D), which is due to the different stoichiometry of ligand binding, with an r.m.s.d larger than 3 Å over 100 Cα atoms. In contrast, the N-terminal domain is similar to that of EcFadR with an r.m.s.d 1.0 Å over 70 Cα atoms (Figure 6D). The major difference between ValFadR and EcFadR lies in the N-domain orientations. The second ligand-binding site involves some residues of the N-terminal domain (Figures S6A,D) and the bound second ligand made the N-domain could not take the similar orientation observed in apo-ValFadR and EcFadR (Figures 6B–D). The large-scale movement of the N-domain leads to distance changes between the two DNA-binding domains of the protein dimer and places the domains in a conformation not suitable for DNA binding. It represents structural basis for ligand-triggered ValFadR-DNA dissociation.
Conformational Alteration of ValFadR by Ligand Binding
Structure superposition showed that the major difference between apo-ValFadR (Figures 7A,D) and liganded-ValFadR (Figures 7B,E) lies in the varied N-domain orientations (Figures 7C,F). Similar scenario also occurred between ligand-bound ValFadR and ligand-bound EcFadR (Figures 6B–D). To illustrate the mechanism whereby ligand-binding leads to the conformational change, both domains of apo-ValFadR and ligand-bound ValFadR are superposed. The N-domains show similar conformations with r.m.s.d 0.9 Å over 65 Cα atoms, so do the C-domains with r.m.s.d 1.3 Å over 173 Cα atoms (Figures 7C,F). These results suggest that the ligand-binding does not alter the overall conformation of both domains but mainly changes the orientation of N-domain (Figures 7C,F). The ligand in the site 1 does not interact with the N-terminal domain and the linker helix, indicating that this ligand-binding does not contribute to the large-scale domain swing. Also, there is no significant domain movement observed in EcFadR upon the ligand-binding (equivalent to site 1 of ValFadR). The ligand in the site 2 interacts with helix α4 of the linker. Interestingly, this helix α4 exists as a standard helix without a B factor significantly higher than the other local residues and did undergo a conformational change from helix to loop upon ligand binding (Figures S6C,D), which is quite different from that of VcFadR (Shi et al., 2015). The second ligand wedged into the interface of N- and C- domain via its acyl chain tail and alters the orientation of helix α4 as well as the N-domain, which is proposed to be a major reason for the large-scale domain swing upon binding the second ligand. Also, the additional ligand in one protomer interacts with many residues from the other protomer as described above, which definitely affects the dimeric interface and causes slightly relative movements between two protomers.
Physiological Roles of Vibrio FadR and the Additional Ligand-Binding Site 2
Genetic amenability in V. cholerae allowed us to create the ΔfadR deletion mutant, using the method of homologous recombination (Figure S7A). Following PCR-based identification, we harvested the interested ΔfadR mutant (Figure S7B). Given the fact that the ligand-binding site 2 of the Vibrio FadRs is mainly involved in the insertion of 40-residues (138-177aa, Figure S1, Figure 5), we therefore designed a site 2-deficient fadR mutant (Δ42 without 136-177aa) and engineered it into the ΔfadR mutant of V. cholerae. Functional complementation with the wild-type and/or Δ42 mutant of fadR gene into the ΔfadR to probe the in vivo role of fadR and the ligand-binding site 2 in the context of lipid metabolism in V. cholerae.
First, western blot analyses with anti-VcFadR rabbit sera as primary antibody showed that the wild-type of fadR gene and its derivative [i.e., the fadR (Δ42) mutant] can express well in V. cholerae, whereas not in the ΔfadR mutant strain of V. cholerae (Figure 8A). Subsequently, LacZ-based transcriptional assays revealed that fabA expression is decreased dramatically in the ΔfadR mutant of V. cholerae, and can be enhanced greatly upon over-expression of the wild-type V. cholerae fadR (Figure 8B). This result confirmed that FadR acts as an activator for the fabA gene of UFA synthesis in Vibrio. Of note, the fadR (Δ42, lacking the site 2) mutant gene failed to restore fabA transcription (Figure 8B), implying the site 2-containing region is critical for VcFadR function. Further analyses of fatty acids composition from Vibrio membrane phospholipids showed that (i) UFA/SFA ratio in the ΔfadR mutant (Figures 9B,E) is relatively lower than that of the wild-type strain (Figures 9A,E), (ii) this ratio can be restored in the complementary strain (CΔfadR+VcfadR) (Figures 9C,E); and (iii) the fadR (Δ42) mutant gene without the site 2 cannot (Figures 8D,E). Therefore, we believed that the Vibrio FadR does control/remodel membrane integrity determined by the ratio of UFA to SFA incorporated into bacterial membrane phospholipids (Figure 9) via its positive regulation of the fabA transcription (Figure 8).
Figure 8. FadR activates expression of fabA, an important gene for unsaturated fatty acid synthesis in V. cholerae. (A) Western blot analyses for fadR expression and its derivatives. The primary antibody used here is rabbit sera against V. cholerae FadR. (B) The beta-gal activity of fabA-lacZ transcription fusion is significantly decreased in the ΔfadR mutant, and can be restored by the functional complementation of the wild-type fadR [but not VcfadR(Δ42)]. The fadR deletion mutant strain referred to ΔfadR, and the two types of complemented strain of ΔfadR used corresponded to CΔfadR + VcfadR and CΔfadR + VcfadR(Δ42), respectively. The VcfadR(Δ42) denoted an engineered version of V. cholerae fadR with a 42-residue deletion covering the site 2 for ligand binding. Log-phase cultures were collected for assaying the LacZ activity. The β-gal activity is expressed as the mean ± standard deviation and is collected from no less than three independent experiments.
Figure 9. Systematic analyses of fatty acid profile suggests that functional alteration of the Vibrio FadR remodels structure of bacterial membrane phospholipids. (A) Analyses for the fatty acid composition isolated from the wild-type strain of V. cholerae. (B) Alteration in the fatty acid compositions in the ΔfadR mutant of V. cholerae. (C) The fatty acid profile in the complemented strain of ΔfadR mutant with plasmid-borne V. cholerae fadR. (D) Failure to recover the fatty acid composition of the V. cholerae ΔfadR strain using plasmid-driven expression of the V. cholerae fadR derivatives that lack the second ligand-binding site [designated as VcfadR(Δ42)]. (E) Effects on UFS/SFA ratio of membrane phospholipids by FadR regulatory protein in V. cholerae. *Student t-test p < 0.01.
Roles of Vibrio FadR and the Ligand-Binding Site 2 in Bacterial Virulence
Similar to the phenotype of the fadR insertional mutant strain of V. vulnificus (Brown and Gulig, 2008), the fadR deletion mutant strain of V. cholerae also displays slower growth in LB liquid media and colony of smaller size on LBA plates than the wild-type strain (Figure S8, Figure 9A). The growth/morphological defects were significantly restored by both plasmid-borne expression of the wild-type VcFadR (Figure S8) and the addition of exogeneous oleate (Figure 10A). However, the expression of fadR (Δ42) with ligand-binding site 2 deleted (Figure 8A) failed to complement the phenotype of defective growth (Figure S8). In light that fadR (Δ42) mutant neither augments the decreased expression of fabA, an important gene for UFA synthesis (Figure 8B), nor rescues the dysfunction in fatty acid composition of phospholipids in the ΔfadR mutant strain of V. cholerae (Figures 9D,E), we favored to hypothesize that the activation of fatty acids synthesis by FadR has significant impacts on bacterial growth and the ligand-binding site 2 is critical for FadR function in vivo.
Figure 10. Oleate can rescue the defection of bacterial growth and swarming caused by the inactivation of FadR. (A) The ΔfadR mutant exhibited the phenotype of small colony size, and growth defect was restored by an addition of oleate into LB media. The two V. cholerae strains used here included WT (C6706) and FYJ639 (ΔfadR). Bacterial cultures in serial 10-fold dilutions were spotted (from top to bottom) on plates of LBA solid medium, and kept at 37°C for 18 h. On the LBA plate without any addition of oleate (Left panel), the single colony size of ΔfadR is much smaller than that of the wild-type. However, the colonial size of the two strains is comparable upon the supplementation of oleate (Right panel) into the LBA plates. The typical colonies are indicated with red arrows. A representative result is given. (B) The ability of bacterial swarming, a virulence-associated trait, was impaired by the deletion of VcFadR, but rescued by the functional complementation of the wild-type fadR (but not fadR(Δ42)) and in vitro supplementation of oleate can rescue (C). For the swarming assays, the log-phase culture appropriately diluted (~10 ul) is spotted on semi-solid 0.3% agar LB plates and kept overnight at 37°C.
Given that the opportunistic pathogen V. vulnificus FadR is necessary for bacterial infection in mice (Brown and Gulig, 2008), it is of much interest to test if site 2 has a role in virulence-associated traits as well as infection competency in V. cholerae (Figures 10, 11). Thus, we examined the possible relevance of fadR (and/or the ligand-binding site 2) to bacterial swarming, a virulence-associated trait. As expected, the swarming ability was impaired greatly upon the removal of fadR from V. cholerae (Figure 10B) (Brown and Gulig, 2008). Functional complementation with VcFadR recovered it to that of the parental strain (Figure 10B). Although the expression of VcFadR (Δ42) (Figure 8A) failed to complement the loss of swarming ability, supplementation of exogenous oleate rendered them indistinguishable in the swarming assays (Figure 10C). We therefore anticipated that dysfunction of swarming/mobility is related to altered surface architecture of membrane phospholipids. Subsequently, we performed infant mouse colonization competition assays (Gardel and Mekalanos, 1996). To rule out the possible effects of delayed growth of ΔfadR mutant, we subjected them to the in vitro colonization trials on LBA plates supplemented with oleate prior to colonization experiments of mice in vivo. The result showed that the delayed growth phenotype of the ΔfadR mutant does not affect greatly the in vitro output [i.e., the ratio of colony numbers (WT/ΔfadR)] (Figure S10). Thus, we compared the colonization abilities of the wild-type strain with the ΔfadR mutant strain and the complementary strain of fadR mutant (with either wild-type fadR or fadR [Δ42, lacking site 2]). We found that the ΔfadR mutant is profoundly defective in colonization (the competitive index is around 0.004) (Figure 11), suggesting that FadR plays a critical role in V. cholerae virulence. Complementation with the wild-type fadR partially restored colonization of ΔfadR, whereas the plasmid containing fadR (Δ42) failed to recover the ΔfadR colonization (Figure 11). It seems possible that the site 2-containing region (42-residues long, 136-177aa) is critical for V. cholerae FadR as a functional virulence factor. In fact, we also noted expression of the two major virulence factors ctxA (Figure S9A) and ctpA (Figure S9B) are slightly inhibited by inactivation of fadR. This control of virulence factors was assigned by Kovacikova et al. (2017) to the indirect modulation of ToxT by FadR via two different mechanisms. Hence, our findings might be additional to the linker of bacterial fatty acid metabolism and Vibrio pathogenesis.
Figure 11. Roles of V. cholerae FadR and the new ligand-binding site 2 in bacterial virulence. Effects exerted by V. cholerae FadR on colonization in the infant mouse model. ΔfadR mutants containing vector control, VcfadR and VcfadR (Δ42) were co-inoculated into infant mice with wild-type at 1:1 ratio. After 18-h colonization, the colonized bacteria were enumerated on selective agar plates. Competitive index is calculated as output ratio of mutant to wild-type normalized against input ratio of mutant to wild-type. Horizontal line: mean of CI. **Student t-test p < 0.01; ns, no significance.
Different organisms have developed diversified mechanisms to tightly modulate fatty acid synthesis as fatty acids are energetically-expensive molecules to produce. To date, six bacterial transcription regulators have been identified. Three of them [FapR (Schujman et al., 2003), DesR (Aguilar et al., 2001; Zhu et al., 2006), and FabT (Lu and Rock, 2006)] are found in Gram-positive bacteria, while the other three members [FadR (Henry and Cronan, 1991; Cronan and Subrahmanyam, 1998; Campbell and Cronan, 2001), FabR (McCue et al., 2001; Zhang et al., 2002), and DesT (Zhang et al., 2007)] are derived from Gram-negative bacteria. Unlike the prototypical version of FadR regulatory protein, the E. coli fadR protein product (van Aalten et al., 2000, 2001; Xu et al., 2001), the description of three Vibrio FadR homologs (ValFadR, VpFadR, and VcFadR) from our groups and recent report by Shi and coworkers (Shi et al., 2015) defined a unique mechanism for bacterial fatty acid sensing in the genus of Vibrio (Figure 1). Although the Vibrio FadR proteins were derived from different species (V. alginolyticus from our group and V. cholerae for Kull's group), the structures we obtained are almost identical, both of which underlined that the insert of 40-residues constitute an extra-domain rich in α-helix (Figures S1, S5, Figure 5). Further dissection for two types of Vibrio FadR-ligand complexes [ValFadR/Palmitoyl-CoA (C16:0) from our group plus VcFadR/Oleoyl-CoA (C18:1) from F. Jon Kull's group] consistently reveal that the so-called “40-aa insert” of Vibrio FadR regulatory protein constitutes the second ligand-binding site in that it already retained the ligand-binding site 1 that is highly similar to that of E. coli FadR (Figure 6, Figure S6). This scenario seen with Vibrio FadR regulator sounds unusual, but not without precedent in that (i) the cAMP-receptor protein (CRP) requires binding of two cAMP molecules each monomer for its function (Passner and Steitz, 1997); (ii) BenM, a LysR-like regulator, has two ligand-binding sites for effector benzoate (Ezezika et al., 2007). Subsequently, the question raised is what could be a physiological explanation for this unique mechanism. We speculated that unlike the paradigm enteric bacterium E. coli colonizing the digestive tract rich in fatty acids, Vibrio species residing in aquatic environments with low level of fatty acids precipitated on the sediment (Giles et al., 2011) have to evolve a more efficient system for fatty acid uptake, rendering its fatty acid-responsive FadR regulator to select an additional ligand-binding site.
Indeed, complex structures of two types of the ligand/Vibrio FadR from our group (Figure 4, Figure S5) and report by Shi et al. (2015) allow us to better understand the structural/molecular basis for crosstalk/response of Vibrio FadR to effectors. As illustrated in Figure 6 and Figure S6, the head of CoA for the second ligand is well fixed and recognized, and the tail of fatty acid chain is inserted between N-terminus and C-terminus of ValFadR and a two-body interface. That is why we hypothesize that fatty acyl-CoA of different lengths might synergistically interfere with Vibrio FadR. In the dimeric form of Vibrio FadR protein, the ends of the four lines of fatty acyl chains converge at the same point, which determine the inability of the limited space to hold fatty acyl chains with much longer length. Probably, the acyl chain of both C16 in ValFadR (Figure 6, Figure S6), and C18 in VcFadR (Shi et al., 2015) seemed to be quite close to the its length limit. The fact that extensive ligand-triggered conformation changes seen with two FadR proteins (ValFadR and VcFadR, Shi et al., 2015) more completely impaired the DNA binding than that of E. coli FadR protein, provided structural explanation for our former observation that addition of oleate can result in almost full de-repression of Vibrio fad regulon, like fadBA (Iram and Cronan, 2005). Not only have we elucidated the contribution of the extra 40-aa insert to the function of Vibrio FadR protein in the context of lipid metabolism, but also discovered its relevance to bacterial infections (Figures 10, 11). Additionally, the uniqueness of this insert inVibrio might determine that the fatty acid sensing by FadR with double ligand-binding sites is exclusively distributed into the phylum of Vibrionaceae from ɤ-proteobacteria.
Together with the recent Kavocikova's discovery that virulence control by V. cholerae FadR is due to indirect cross-talking with ToxT, a master virulence regulator, via two independent mechanisms (Kovacikova et al., 2017), our results constituted additional input to better understanding of link between fatty acid metabolism and bacterial pathogenicity, i.e., membrane integrity of phospholipids is crucial for bacterial competitive colonization. The structural characterization of ValFadR regulator defines an additional example in the context of the diversified regulation of bacterial fatty acid metabolism (Marrakchi et al., 2002; Zhang and Rock, 2009). We hypothesized that the Vibrio FadR regulator has evolved this additional ligand-binding site to gain an advantage of infection competency in bacterial-host battle. Given the significant contribution of FadR regulatory protein to pathogenesis of certain Vibrio species, it is possible that development of small molecule drugs/inhibitors targeting the FadR-mediated mechanism for bacterial fatty acid sensing might be efficient therapeutics against severe infections by the zoonotic Vibrio pathogens.
Materials and Methods
Animal care and treatment were conducted in accordance with institutional guidelines and the protocols at Zhejiang University, China. Five-day-old CD1 mice were housed in a temperature-controlled room with proper darkness-light cycles, fed with a regular diet, and maintained under the Experimental Animal Center of Zhejiang University, China. The mouse experimental design and protocols used here were approved by the Ethics Committee of Zhejiang University, China (ZJU20170800).
Bacterial Strains and Growth Conditions
E. coli strains used here are derivatives of the wild-type K-12 strain (Table S1). Vibrio strains used here included V. cholerae EI Tor C6706 (Joelsson et al., 2006), V. parahaemolyticus ATCC 17802 and V. alginolyticus. E. coli SM10 (λ-pir) was used as the donor strain for conjugations with V. cholerae. These strains were routinely maintained in LB medium (Luria-Bertani medium containing 10 g of tryptone, 5 g of yeast extract and 10 g of NaCl per liter) or on LB agar plates (Feng and Cronan, 2011). LB without NaCl and containing 6% (wt/vol) sucrose was used for a selection of the strain with homologous recombination. The growth temperatures used are either 30° or 37°C. When necessary, antibiotics were added as follows (in μg/ml): tetracycline, 20 for E. coli and 2 for V. cholerae; ampicillin, 100; kanamycin, 50; and streptomycin, 100 (Feng and Cronan, 2009a).
Plasmids and DNA Manipulations
V. cholerae fadR gene was previously cloned pET16b vector (Iram and Cronan, 2005). The two fadR genes from V. parahaemolyticus and V. alginolyticus were separately amplified with PCR. They were directionally cloned into the pET28 expression vector. The resultant recombinant plasmids were introduced into E. coli BL21 (DE3) for large-scale production of the FadR protein. As we previously described in the synthesis of the Brucella bioR gene in vitro with little change (Feng et al., 2013), overlapping PCR was used to create a mutant fadR gene (fadR(Δ42)) with the deletion of 42 residues (136-177aa). The pWM91 vector is applied for construction of fadR knock-out plasmid (Metcalf et al., 1996). The expression plasmid pBBR1-MCS3 is used for functional assays of the fadR gene in different versions (VcfadR and the VcfadR mutant Δ42), Table S1) in V. cholerae (Kovach et al., 1995). All plasmid constructs were validated by PCR detection (Table S2) and direct DNA sequencing (Zhang et al., 2014).
In-Frame Deletion of V. cholerae fadR and Genetic Complementation
V. cholerae El Tor C6706 (Joelsson et al., 2006) was used as the wild-type strain in this study unless otherwise noted. In-frame deletions were constructed by cloning of the upstream (and downstream) regions neighboring the target fadR gene (vc1900) into the suicide vector pWM91 containing a sacB counter-selectable maker (Metcalf et al., 1996). The upstream (and/or downstream) DNA fragments (of 700 bp long) flanking fadR were amplified by PCR using the two pairs of specific primers (L-flank fadR-5′/L-flank fadR-3′ and R-flank fadR-5′/R-flank fadR-3′) with the high-fidelity Prime STAR DNA Polymerase (Table S2). The flanking DNA sequences in the upstream (and downstream) of the fadR were overlapped and cloned into the two restriction sites of pWM91 (SacI and BamHI), giving knockout plasmid pWM91-fadRKO. Then the plasmid was introduced into the V. cholerae strain by conjugation from SM10 (λ-pir) and a single crossover event was selected by resistance to streptomycin and ampicillin. The selection growth in the absence of ampicillin and streptomycin assures that double crossover events occur. Finally, the ΔfadR mutant was given via sucrose-based screening. The proper genetic exchange event was confirmed by multiplex-PCR and direct DNA sequencing.
For functional complementation, the wild-type fadR gene of V. cholerae plus its VcfadR mutant (fadR(Δ42)) were directionally inserted into the pBBR1-MCS3 vector via the two sites (KpnI and XbaI), giving plasmids like pBBR1-MCS3-fadR (Table S1). The resultant plasmids were transformed into E. coli SM10 (λ-pir), and then conjugated into the V. cholerae ΔfadR mutant. Tran-conjugants were selected on LB plates containing streptomycin and tetracycline. All the constructs were verified by direct DNA sequencing of PCR products.
Anti-FadR Rabbit Sera and Western Blot
Anti-sera against VcFadR were prepared as previously described (Shao et al., 2011). Pre-immune sera were collected from New Zealand White rabbits (female, 1.5 kg) and then animals were injected subcutaneously at multiple sites with approximately 1 mg/kg of purified FadR recombinant protein emulsified with Freund's complete adjuvant (1:1). After 2 weeks, each rabbit received the first booster injection with the same antigen concentration emulsified with Freund's incomplete adjuvant (1:1). One week later, each rabbit received the second booster injection with the same antigen concentration emulsified with Freund's incomplete adjuvant (1:1). Then, anti-serum samples were collected when the booster injection was administered 7 days later. The sensitivity and specificity of antibody were evaluated routinely by ELISA and Western blot (Feng and Cronan, 2009b). Using the rabbit sera against VcFadR protein as primary antibody, Western blotting analyses were conducted to detect expression of fadR gene (and its derivatives) in the wild-type (or ΔfadR mutant) strain of V. cholerae.
Growth Phenotypes and Swarming Assays
Growth phenotypes of V. cholerae and its derivatives were examined using both LBA solid plates and measurement of growth curves. To determine effect of colony size by the deletion of fadR, bacterial cultures in series of 10-fold dilution were spotted on solid LBA plates and maintained overnight at 37°C. Similarly, the cultivation of V. cholerae species in liquid LB media at 37°C was monitored for plotting the growth curves. For swarming assays, log-phase cultures were diluted appropriately (10 μl each) is spotted on semi-solid 0.3% agar LBA plates and kept overnight at 37°C prior to visualization of mobility. Over three independent trials were conducted.
Assays for Competition Colonization in Infant Mice
Following the protocol established by Davies et al. (2011) with minor modifications, we evaluated the role of fadR in bacterial virulence through the competitive colonization experiments in the model of infant mouse. Briefly, the wild-type strain of V. cholerae (either C6706 or C6706 lac−) and its mutants were cultivated on LBA plates with streptomycin (100 μg/ml) overnight at 37°C. The wild-type and mutant strains were mixed together in LB medium. 100 μl of competition mixtures (about 1 X 105 CFU) were inoculated into a 5-day-old CD1 infant mouse. Serial dilutions of the competition mixture were plated on LBA plates with streptomycin (100 μg/ml) as the selective pressure and enumerated to determine the input ratio of wild-type to the mutant strain. After incubation at 30°C for 18 h, the infant mice were sacrificed, and small intestines were removed and homogenized in 5 ml of LB. Serial dilutions were plated on LBA plates containing streptomycin (100 μg/ml) and enumerated to determine the output ratio of wild-type to the appropriate mutant strain. The competitive index for each mutant is defined as the input ratio of mutant/wild-type strain divided by the output ratio of mutant/wild-type strain.
Protein Expression and Purification
Since all the other three FadR proteins of Vibrio origins were tagged with hexa-histidine on the N-terminus, similar to the paradigm E. coli FadR protein stocked in our lab. The recombinant proteins were routinely prepared as we described before (Zhang et al., 2014). Briefly, when the optical density at wavelength of 600 nm (OD600) reached 0.6, the bacterial culture was induced with 0.2 mM isopropyl-β-D-1-thiogalactopyranoside (IPTG) at 30°C overnight. Following lysis by sonication, the cell lysate was clarified by centrifugation and loaded onto a nickel-ion affinity column (Qiagen). After removal of contaminant proteins with washing buffer containing 50 mM imidazole, the 6xHis-tagged FadR protein was eluted in elution buffer containing 150 mM imidazole, concentrated by ultra-filtration (30-kDa cutoff) and exchanged into 20 mM Tris-HCl (pH 7.5) containing 100 mM NaCl. The soluble fractions were further purified by gel filtration with a Superdex 200 10/300 column (GL, GE Healthcare) and the resultant FadR proteins were judged with 12% SDS-PAGE. Protein concentrations were measured using the BCA method with BSA as internal reference (Thermo Scientific).
Electrophoretic Mobility Shift Assays
As we described earlier with minor modifications (Zhang et al., 2014), electrophoretic mobility shift assays (EMSA) were conducted to test the binding of FadR protein to the DNA targets. In this case, FadR protein of E. coli and Vibrio were studied. The FadR-specific DNA probes is fabA probe which is specific to the fatty acid biosynthesis fabA gene. The above double-stranded DNA probe was generated by annealing the two complementary primers in TEN buffer (10 mM Tris-HCl, 1 mM EDTA, 100 mM NaCl; pH 8.0). Generally, the DNA probe was mixed with/without FadR protein in binding buffer and incubated at room temperature. The DNA-protein complexes were separated with native PAGE gels (Feng and Cronan, 2011, 2012; Tang et al., 2014).
Surface Plasmon Resonance
To further address the interplay between FadR proteins and the DNA target (such as fabA), surface plasmon resonance (SPR) was employed using a Biacore3000 instruments (GE Healthcare) at 25°C. For immobilization on an SA sensor chip, the biotinylated DNA probe of fabA was specifically captured by streptavidin on the surface. All the SPR experiments were run in the running buffer (20 mM Tris-HCl, pH7.5, 200 mM NaCl and 0.005% Tween 20) at the flow rate of 30 μl/min. A series of dilutions of protein samples were injected and passed over the chip surface for 2 min. The dissociation phase was followed for 3 min in the same buffer, and the surface was then regenerated with 0.025% SDS for 24 s. Kinetic parameters were analyzed using a global data analysis program (BIA evaluation software), and final graphs were further processed with Origin software.
Isothermal Titration Calorimetry
To study the binding of FadR protein to its effector molecule like palmitoyl-CoA, isothermal titration calorimetry (ITC) was conducted using a MicroCal iTC200 (Malvern) with a cell volume of 200 μl. Both FadR samples and the ligand of palmitoyl-CoA were dialyzed against the same buffer (20 mM Tris-HCl pH7.5, 100 mM NaCl) to minimize artifacts due to minor differences of the buffer composition. Prior to titration, the sample of FadR protein was injected into the cell, and the syringe was filled with palmitoyl-CoA. All the ITC experiments were performed at 25°C with a reference power of 8 and a stirring speed of 1,000 rpm. The final heat was corrected by subtracting the dilution heat from palmitoyl-CoA titrated to buffer. The raw data was analyzed with the Origin software (note: one set of sites for EcFadR, two sets of sites for VpFadR and ValFadR, and sequential binding sites for VcFadR).
To measure bacterial β-gal activity, log-phase cultures of V. cholerae carrying the plasmid-borne pTL61T-PfabA-lacZ transcription fusion grown in LB media (Table S1) were collected by spinning and suspended in Z-buffer (Gao et al., 2016). The data was obtained from three independent assays.
Protein Crystallization and Data Collection
All the apo-FadR homologs of three Vibrio species (ValFadR, VpFadR, and VcFadR) were subjected to initial crystallization trials at protein level of 10 mg/ml, using hanging-drop vapor diffusion method at 16°C. 1μl of protein solution was mixed equally with the well solution. Consequently, crystals of apo-ValFadR were observed on the condition containing 200 mM Calcium Acetate, 100 mM Sodium Cacodylate pH 6.5 and 7% PEG8000. After 2–3 days, crystals grew to dimension of 0.1 mm by 0.15 mm by 0.1 mm. To obtain the crystal of ValFadR complex with ligand, a 2-fold molar excess of palmitoyl-CoA was added to 10 mg/ml ValFadR solution, and incubated for 2 h at 16°C before crystallization. The crystals were grown on the condition (4% Tacsimate, pH 5.0, 11% PEG3350) in 2 weeks. Crystal was transferred to cryo-protecting solution of mother liquor containing 15% glycerol for a few seconds and then quickly flash-cooled in liquid nitrogen and the dataset was collected on a Rigaku R-Axis IV++ image plate using Cu Kα radiation (λ = 1.5418 Å) at 100 K.
Structure Determination and Refinement
Diffraction data of protein crystals was integrated and processed using MOSFLM and SCALA from the CCP4 program suite (Collaborative Computational Project, 1994). The structure of ValFadR was determined by molecular replacement using EcFadR structure (PDB: 1E2X) as a search model. The model was first built automatically using PHENIX package (Adams et al., 2002) and then manually with COOT (Emsley and Cowtan, 2004) and structure refinement was performed with Phenix. For the structure of ValFadR and palmitoyl-CoA complex, the apo-ValFadR structure was used as a search model and then was built manually with Coot and refined with Phenix. The stereo-chemical quality of the refined structures was verified with PROCHECK (Morris et al., 1992). All structural representations were prepared with PyMol (DeLano Scientific). The two PDB accession numbers are listed as follows: 5XGF for ValFadR alone and 5DV5 for ligand-bound ValFadR protein.
YF designed this project; YF, YL, RG, XX, JL, and DL performed experiments and analyzed the data; LB, JZ, HW, BH, and SW contributed reagents and tools; YF, DL, YL, JZ, and SW wrote this manuscript.
Conflict of Interest Statement
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
This work was supported by National Key R&D Program of China [2017YFD0500202 (YF)], the National Natural Science Foundation of China under Grant No. 31570027 & 81772142 (YF), Zhejiang Provincial Natural Science Foundation of China under Grant No. LR15H190001 (YF) and National Key Basic Research Program of China [2013CB127802 (SW), 2016YFC1200100 (YF)]. YF is a recipient of the “Young 1000 Talents” Award. We would like to thank Prof. John E. Cronan and Mr. Saif Ullah for critical reading of this manuscript.
Adams, P. D., Grosse-Kunstleve, R. W., Hung, L. W., Ioerger, T. R., McCoy, A. J., Moriarty, N. W., et al. (2002). PHENIX: building new software for automated crystallographic structure determination. Acta Crystallogr. D Biol. Crystallogr. 58, 1948–1954. doi: 10.1107/S0907444902016657
Aguilar, P. S., Hernandez-Arriaga, A. M., Cybulski, L. E., Erazo, A. C., and de Mendoza, D. (2001). Molecular basis of thermosensing: a two-component signal transduction thermometer in Bacillus subtilis. EMBO J. 20, 1681–1691. doi: 10.1093/emboj/20.7.1681
Brown, R. N., and Gulig, P. A. (2008). Regulation of fatty acid metabolism by FadR is essential for Vibrio vulnificus to cause infection of mice. J. Bacteriol. 190, 7633–7644. doi: 10.1128/JB.01016-08
Campbell, J. W., and Cronan, J. E. Jr. (2001). Escherichia coli FadR positively regulates transcription of the fabB fatty acid biosynthetic gene. J. Bacteriol. 183, 5982–5990. doi: 10.1128/JB.183.20.5982-5990.2001
Champion, G. A., Neely, M. N., Brennan, M. A., and DiRita, V. J. (1997). A branch in the ToxR regulatory cascade of Vibrio cholerae revealed by characterization of toxT mutant strains. Mol. Microbiol. 23, 323–331. doi: 10.1046/j.1365-2958.1997.2191585.x
Cronan, J. E. Jr. (1997). In vivo evidence that acyl coenzyme A regulates DNA binding by the Escherichia coli FadR global transcription factor. J. Bacteriol. 179, 1819–1823. doi: 10.1128/jb.179.5.1819-1823.1997
Davies, B. W., Bogard, R. W., Dupes, N. M., Gerstenfeld, T. A., Simmons, L. A., and Mekalanos, J. J. (2011). DNA damage and reactive nitrogen species are barriers to Vibrio cholerae colonization of the infant mouse intestine. PLoS Pathog. 7:e1001295. doi: 10.1371/journal.ppat.1001295
Ezezika, O. C., Haddad, S., Clark, T. J., Neidle, E. L., and Momany, C. (2007). Distinct effector-binding sites enable synergistic transcriptional activation by BenM, a LysR-type regulator. J. Mol. Biol. 367, 616–629. doi: 10.1016/j.jmb.2006.09.090
Feng, Y., and Cronan, J. E. (2009b). Escherichia coli unsaturated fatty acid synthesis: complex transcription of the fabA gene and in vivo identification of the essential reaction catalyzed by FabB. J. Biol. Chem. 284, 29526–29535. doi: 10.1074/jbc.M109.023440
Feng, Y., and Cronan, J. E. (2011). The Vibrio cholerae fatty acid regulatory protein, FadR, represses transcription of plsB, the gene encoding the first enzyme of membrane phospholipid biosynthesis. Mol. Microbiol. 81, 1020–1033. doi: 10.1111/j.1365-2958.2011.07748.x
Feng, Y., Xu, J., Zhang, H., Chen, Z., and Srinivas, S. (2013). Brucella BioR regulator defines a complex regulatory mechanism for bacterial biotin metabolism. J. Bacteriol. 195, 3451–3467. doi: 10.1128/JB.00378-13
Gao, R., Lin, J., Zhang, H., and Feng, Y. (2016). Transcriptional repression of the VC2105 protein by Vibrio FadR suggests that it is a new auxiliary member of the fad regulon. Appl. Environ. Microbiol. 82, 2819–2832. doi: 10.1128/AEM.00293-16
Giles, D. K., Hankins, J. V., Guan, Z., and Trent, M. S. (2011). Remodelling of the Vibrio cholerae membrane by incorporation of exogenous fatty acids from host and aquatic environments. Mol. Microbiol. 79, 716–728. doi: 10.1111/j.1365-2958.2010.07476.x
Heidelberg, J. F., Eisen, J. A., Nelson, W. C., Clayton, R. A., Gwinn, M. L., Dodson, R. J., et al. (2000). DNA sequence of both chromosomes of the cholera pathogen Vibrio cholerae. Nature 406, 477–483. doi: 10.1038/35020000
Henry, M. F., and Cronan, J. E. Jr. (1991). Escherichia coli transcription factor that both activates fatty acid synthesis and represses fatty acid degradation. J. Mol. Biol. 222, 843–849. doi: 10.1016/0022-2836(91)90574-P
Henry, M. F., and Cronan, J. E. Jr. (1992). A new mechanism of transcriptional regulation: release of an activator triggered by small molecule binding. Cell 70, 671–679. doi: 10.1016/0092-8674(92)90435-F
Iram, S. H., and Cronan, J. E. (2006). The beta-oxidation systems of Escherichia coli and Salmonella enterica are not functionally equivalent. J. Bacteriol. 188, 599–608. doi: 10.1128/JB.188.2.599-608.2006
Joelsson, A., Liu, Z., and Zhu, J. (2006). Genetic and phenotypic diversity of quorum-sensing systems in clinical and environmental isolates of Vibrio cholerae. Infect. Immun. 74, 1141–1147. doi: 10.1128/IAI.74.2.1141-1147.2006
Klein, K., Steinberg, R., Fiethen, B., and Overath, P. (1971). Fatty acid degradation in Escherichia coli. An inducible system for the uptake of fatty acids and further characterization of old mutants. Eur. J. Biochem. 19, 442–450. doi: 10.1111/j.1432-1033.1971.tb01334.x
Kovach, M. E., Elzer, P. H., Hill, D. S., Robertson, G. T., Farris, M. A., Roop, R. M., et al. (1995). Four new derivatives of the broad-host-range cloning vector pBBR1MCS, carrying different antibiotic-resistance cassettes. Gene 166, 175–176. doi: 10.1016/0378-1119(95)00584-1
Kovacikova, G., Lin, W., Taylor, R. K., and Skorupski, K. (2017). The fatty acid regulator FadR influences the expression of the virulence cascade in the El Tor biotype of Vibrio cholerae by modulating the levels of ToxT via two different mechanisms. J. Bacteriol. 199:e00762-16. doi: 10.1128/JB.00762-16
McCue, L., Thompson, W., Carmack, C., Ryan, M. P., Liu, J. S., Derbyshire, V., et al. (2001). Phylogenetic footprinting of transcription factor binding sites in proteobacterial genomes. Nucleic Acids Res. 29, 774–782. doi: 10.1093/nar/29.3.774
Metcalf, W. W., Jiang, W., Daniels, L. L., Kim, S. K., Haldimann, A., and Wanner, B. L. (1996). Conditionally replicative and conjugative plasmids carrying lacZ alpha for cloning, mutagenesis, and allele replacement in bacteria. Plasmid 35, 1–13. doi: 10.1006/plas.1996.0001
My, L., Rekoske, B., Lemke, J. J., Viala, J. P., Gourse, R. L., and Bouveret, E. (2013). Transcription of the Escherichia coli fatty acid synthesis operon fabHDG is directly activated by FadR and inhibited by ppGpp. J. Bacteriol. 195, 3784–3795. doi: 10.1128/JB.00384-13
Novichkov, P. S., Kazakov, A. E., Ravcheev, D. A., Leyn, S. A., Kovaleva, G. Y., Sutormin, R. A., et al. (2013). RegPrecise 3.0–a resource for genome-scale exploration of transcriptional regulation in bacteria. BMC Genomics 14:745. doi: 10.1186/1471-2164-14-745
Overath, P., Pauli, G., and Schairer, H. U. (1969). Fatty acid degradation in Escherichia coli. An inducible acyl-CoA synthetase, the mapping of old-mutations, and the isolation of regulatory mutants. Eur. J. Biochem. 7, 559–574. doi: 10.1111/j.1432-1033.1969.tb19644.x
Ray, S., Chatterjee, E., Chatterjee, A., Paul, K., and Chowdhury, R. (2011). A fadD mutant of Vibrio cholerae is impaired in the production of virulence factors and membrane localization of the virulence regulatory protein TcpP. Infect. Immun. 79, 258–266. doi: 10.1128/IAI.00663-10
Schujman, G. E., Paoletti, L., Grossman, A. D., and de Mendoza, D. (2003). FapR, a bacterial transcription factor involved in global regulation of membrane lipid biosynthesis. Dev. Cell 4, 663–672. doi: 10.1016/S1534-5807(03)00123-0
Shao, Z., Pan, X., Li, X., Liu, W., Han, M., Wang, C., et al. (2011). HtpS, a novel immunogenic cell surface-exposed protein of Streptococcus suis, confers protection in mice. FEMS Microbiol. Lett. 314, 174–182. doi: 10.1111/j.1574-6968.2010.02162.x
Shi, W., Kovacikova, G., Lin, W., Taylor, R. K., Skorupski, K., and Kull, F. J. (2015). The 40-residue insertion in Vibrio cholerae FadR facilitates binding of an additional fatty acyl-CoA ligand. Nat. Commun. 6:6032. doi: 10.1038/ncomms7032
Tang, Q., Li, X., Zou, T., Zhang, H., Wang, Y., Gao, R., et al. (2014). Mycobacterium smegmatis BioQ defines a new regulatory network for biotin metabolism. Mol. Microbiol. 94, 1006–1023. doi: 10.1111/mmi.12817
Taylor, R. K., Miller, V. L., Furlong, D. B., and Mekalanos, J. J. (1987). Use of phoA gene fusions to identify a pilus colonization factor coordinately regulated with cholera toxin. Proc. Natl. Acad. Sci. U.S.A. 84, 2833–2837. doi: 10.1073/pnas.84.9.2833
Thompson, F. L., Gevers, D., Thompson, C. C., Dawyndt, P., Naser, S., Hoste, B., et al. (2005). Phylogeny and molecular identification of Vibrios on the basis of multilocus sequence analysis. Appl. Environ. Microbiol. 71, 5107–5115. doi: 10.1128/AEM.71.9.5107-5115.2005
van Aalten, D. M., DiRusso, C. C., and Knudsen, J. (2001). The structural basis of acyl coenzyme A-dependent regulation of the transcription factor FadR. EMBO J. 20, 2041–2050. doi: 10.1093/emboj/20.8.2041
van Aalten, D. M., DiRusso, C. C., Knudsen, J., and Wierenga, R. K. (2000). Crystal structure of FadR, a fatty acid-responsive transcription factor with a novel acyl coenzyme A-binding fold. EMBO J. 19, 5167–5177. doi: 10.1093/emboj/19.19.5167
Xu, Y., Heath, R. J., Li, Z., Rock, C. O., and White, S. W. (2001). The FadR.DNA complex. Transcriptional control of fatty acid metabolism in Escherichia coli. J. Biol. Chem. 276, 17373–17379. doi: 10.1074/jbc.M100195200
Yang, M., Liu, Z., Hughes, C., Stern, A. M., Wang, H., Zhong, Z., et al. (2013). Bile salt-induced intermolecular disulfide bond formation activates Vibrio cholerae virulence. Proc. Natl. Acad. Sci. U.S.A. 110, 2348–2353. doi: 10.1073/pnas.1218039110
Zhang, H., Zheng, B., Gao, R., and Feng, Y. (2015). Binding of Shewanella FadR to the fabA fatty acid biosynthetic gene: implications for contraction of the fad regulon. Protein Cell 6, 667–679. doi: 10.1007/s13238-015-0172-2
Zhang, Y., Gao, R., Ye, H., Wang, Q., and Feng, Y. (2014). A new glimpse of FadR-DNA crosstalk revealed by deep dissection of the E. coli FadR regulatory protein. Protein Cell 5, 928–939. doi: 10.1007/s13238-014-0107-3
Zhang, Y. M., Marrakchi, H., and Rock, C. O. (2002). The FabR (YijC) transcription factor regulates unsaturated fatty acid biosynthesis in Escherichia coli. J. Biol. Chem. 277, 15558–15565. doi: 10.1074/jbc.M201399200
Zhang, Y. M., Zhu, K., Frank, M. W., and Rock, C. O. (2007). A Pseudomonas aeruginosa transcription factor that senses fatty acid structure. Mol. Microbiol. 66, 622–632. doi: 10.1111/j.1365-2958.2007.05934.x
Keywords: FadR, ligand, fatty acid sensing, virulence, Vibrio alginolyticus
Citation: Gao R, Li D, Lin Y, Lin J, Xia X, Wang H, Bi L, Zhu J, Hassan B, Wang S and Feng Y (2017) Structural and Functional Characterization of the FadR Regulatory Protein from Vibrio alginolyticus. Front. Cell. Infect. Microbiol. 7:513. doi: 10.3389/fcimb.2017.00513
Received: 11 October 2017; Accepted: 29 November 2017;
Published: 12 December 2017.
Edited by:Martin John McGavin, University of Western Ontario, Canada
Reviewed by:Hongxia Wang, University of Alabama at Birmingham, United States
Xiaohui Zhou, University of Connecticut, Storrs, United States
Copyright © 2017 Gao, Li, Lin, Lin, Xia, Wang, Bi, Zhu, Hassan, Wang and Feng. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) or licensor are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Youjun Feng, email@example.com
†These authors have contributed equally to this work.