Vancomycin does not affect the enzymatic activities of purified VanSA

Abstract

VanS is a membrane-bound sensor histidine kinase responsible for sensing vancomycin and activating transcription of vancomycin-resistance genes. In the presence of vancomycin, VanS phosphorylates the transcription factor VanR, converting it to its transcriptionally active form. In the absence of vancomycin, VanS dephosphorylates VanR, thereby maintaining it in a transcriptionally inactive state. To date, the mechanistic details of how vancomycin modulates VanS activity have remained elusive. We have therefore studied these details in an in vitro system, using the full-length VanS and VanR proteins responsible for type-A vancomycin resistance in enterococci. Both detergent- and amphipol-solubilized VanSA display all the enzymatic activities expected for a sensor histidine kinase, with amphipol reconstitution providing a marked boost in overall activity relative to detergent solubilization. A putative constitutively activated VanSA mutant (T168K) was constructed and purified, and was found to exhibit the expected reduction in phosphatase activity, providing confidence that detergent-solubilized VanSA behaves in a physiologically relevant manner. In both detergent and amphipol solutions, VanSA’s enzymatic activities were found to be insensitive to vancomycin, even at levels many times higher than the antibiotic’s minimum inhibitory concentration. This result argues against direct activation of VanSA via formation of a binary antibiotic-kinase complex, suggesting instead that either additional factors are required to form a functional signaling complex, or that activation does not require direct interaction with the antibiotic.

About the Authors:

Elizabeth C. Upton

Roles Conceptualization, Formal analysis, Investigation, Methodology, Writing – original draft, Writing – review & editing

¶‡ These authors are co-first authors on this work.

Affiliation: Department of Biochemistry and Molecular Biology, Drexel University College of Medicine, Philadelphia, Pennsylvania, United States of America

Lina J. Maciunas

Roles Conceptualization, Formal analysis, Investigation, Validation, Writing – review & editing

¶‡ These authors are co-first authors on this work.

Affiliation: Department of Biochemistry and Molecular Biology, Drexel University College of Medicine, Philadelphia, Pennsylvania, United States of America

Patrick J. Loll

Roles Conceptualization, Formal analysis, Funding acquisition, Investigation, Methodology, Supervision, Writing – review & editing

* E-mail: [email protected]

Affiliation: Department of Biochemistry and Molecular Biology, Drexel University College of Medicine, Philadelphia, Pennsylvania, United States of America

ORCID logo http://orcid.org/0000-0001-5416-4500

Introduction

Enterococci are commensal bacteria normally found in the human gastrointestinal system; however, they can also cause serious and potentially fatal systemic infections such as endocarditis and bacteremia [1]. Enterococcal infections have long been treated with vancomycin, but now the rise of vancomycin-resistant enterococci (VRE) threatens the utility of the antibiotic and presents a significant public health threat [2]. VRE have acquired vancomycin-resistance genes carried on transmissible DNA elements [3]. Different phenotypic variants of VRE are known, which differ in the level of resistance conferred; of these, A-type resistance is responsible for the majority of VRE encountered in humans [4]. However, all the known resistance phenotypes share certain common properties. All produce enzymes that remodel the cell wall in order to alter vancomycin’s target; in the case of VanA, this remodeling reduces vancomycin’s affinity for its target ~1,000-fold [5–7]. All resistance operons also encode VanS and VanR, two proteins that function together to control the expression of the other resistance genes, ensuring that the remodeling enzymes are expressed only in the presence of vancomycin.

This report focuses on the VanS and VanR proteins associated with A-type resistance (herein denoted VanSA and VanRA). VanSA and VanRA form a two-component system that modulates the expression of vancomycin resistance genes in response to antibiotic challenge. Two-component systems are ubiquitous in bacteria and plants [8–10] and help shape an organism’s response to signals in its environment. Two-component systems comprise a sensor and a response regulator; the former recognizes and transduces the signal, while the latter translates this signal into some cellular response. In the VanA two-component system, VanSA is a histidine kinase that serves as the sensor, and VanRA is a transcription factor that serves as the response regulator [11]. In the presence of vancomycin, VanSA autophosphorylates on a conserved histidine residue, and then transfers this phosphoryl group to an aspartate on VanRA [12, 13]. The phosphorylated VanRA is the active form of the transcription factor, which binds to the van promoters to activate transcription of the vancomycin-resistance genes [14]. In the absence of vancomycin, VanSA dephosphorylates VanRA, thereby maintaining it in its inactive state [11, 15]. Hence, three distinct catalytic activities are associated with VanSA: autophosphorylation, phosphotransfer, and dephosphorylation.

Although the broad outline of VanR-VanS functioning is known, many details remain elusive, including the mechanism by which VanS senses vancomycin. Two main models have been advanced to explain this process. The first posits a direct molecular interaction between vancomycin and the periplasmic domain of VanS, inducing a conformational change in the protein that leads to stimulation of autophosphorylation [16, 17]. The second model suggests that, rather than detecting the antibiotic directly, VanS instead senses some downstream consequence of vancomycin action, for example accumulation of a biosynthetic precursor, or a change in membrane fluidity caused by disruption of the cell wall [18–21]. Evidence is available to support both models, and there is currently not a consensus as to which (if either) is correct, or indeed if all VanS proteins even function by the same mechanism. Given the clinical importance of VRE, developing a better understanding of how VanSA senses vancomycin is of paramount importance.

A purified, reconstituted VanRA-VanSA signaling system will be of great benefit in addressing questions related to vancomycin sensing. In pioneering work from the Walsh laboratory, the cytosolic domain of VanSA was previously purified [15]; however, studies of how the vancomycin signal is sensed and transduced must necessarily include the transmembrane and periplasmic domains. This imperative has prompted more recent efforts in which full-length VanSA has been purified [22–25]. These studies of the full-length protein focused largely on its antibiotic binding and hydrodynamic characteristics. Now, we provide a complementary analysis of VanSA’s enzymatic functions. Herein we describe the purification of full-length VanSA, evaluate all three of its baseline enzymatic activities, assess the effect of vancomycin on these activities, and characterize its interaction with its cognate response regulator, VanRA. We also show that VanSA activity depends strongly on the mechanism of solubilization used, consistent with models in which small rearrangements of histidine kinase transmembrane domains give rise to activation or suppression of signaling activity [26].

Materials and methods

Protein expression

A gene encoding full-length VanSA (Uniprot Q06240) was synthesized using codon optimization for E. coli expression (Genscript) and cloned into the in-house vector pETCH [27], yielding a construct in which the sequence PGHHHHHH is appended to the C-terminus of the VanSA protein. The T168K mutant of VanSA was produced by a one-step PCR-based site-directed mutagenesis protocol [28]. Primers used are shown in S1 Table. To prepare an expression construct for the cytosolic domain of VanSA (cVanSA), we used the TMHMM server [29, 30] to predict the locations of the two transmembrane helices. This analysis suggested that the cytoplasmic domain begins at residue K98. We therefore cloned the sequence corresponding to residues 98–384 into pETCH, giving a construct having the sequences MV added at the N-terminus and PGHHHHHH at the C-terminus. The codon-optimized gene for full-length VanRA (Uniprot Q06239) was synthesized and subcloned into pETHSUL, [27] yielding a construct with a cleavable N-terminal 6xHis-SUMO tag. Removal of the SUMO tag with SUMO hydrolase produces a full-length VanRA molecule with a single glycine residue appended to its N-terminus. The full-length VanSA and VanRA proteins were expressed in BL21(DE3) cells, growing cells in LB broth at 37°C to an OD600 of ~0.4, at which point the temperature was reduced to 18°C and IPTG was added to a final concentration of 300 μM. Cells were harvested after ~20 hours of shaking at 175 RPM. Cytosolic VanSA was expressed in auto-inducing media [31] at 30°C and 225 RPM and harvested 20 hours after inoculation.

All purification steps took place at 4°C. For all constructs used (S1 Fig), purification began with cell lysis in an Emulsiflex C5 cell homogenizer at 10,000–15,000 psi in lysis buffer (50 mM Tris pH 7.7, 500 mM NaCl, 5 mM MgCl2). Cell lysate was clarified by centrifugation at 5,000xg for 15 minutes, then spun at ~117,000xg for 1 hour to separate the membrane fraction (high-speed pellet) from the soluble fraction (high speed supernatant). At this point, the protocols used for the different constructs diverged; specifics are given below.

Full-length VanSA: The membrane pellet corresponding to 6 liters’ worth of cells was homogenized in 45 mL of lysis buffer, and then 5 mL of 10% (w/v) DDM were added. The suspension was rocked at 4°C for 1 hour and then centrifuged at 117,000xg for 1 hour to remove unsolubilized material. The supernatant was filtered through a 0.45 micron filter and loaded onto a 1-mL HiTrap IMAC HP column (GE Life Sciences) equilibrated in IMAC A buffer (50 mM Tris pH 7.8, 500 mM NaCl, 5 mM MgCl2, 40 mM imidazole) plus 0.1% DDM. To exchange the protein into LDAO the column was washed with IMAC A buffer containing 10 mM LDAO. VanSA was then eluted with a gradient (10 column volumes) to 100% IMAC B buffer (IMAC A+ 500 mM imidazole) + 10 mM LDAO. Fractions containing VanSA were pooled and concentrated to ~500 μL and loaded onto a 1.1 cm x 50 cm Sephacryl S-300 column equilibrated with 50 mM Tris pH 7.8, 500 mM NaCl, 5 mM MgCl2, 10 mM LDAO. Protein fractions were pooled and concentrated to ~500 μL and dialyzed vs. 50 mM Tris pH 7.8, 150 mM NaCl, 5 mM MgCl2, 5% glycerol, 10 mM LDAO. Final detergent concentrations in the purified samples were measured using TLC [32].

cVanSA: The high speed supernatant from 2 liters’ worth of cells was filtered and purified by immobilized metal chromatography, as described for full-length VanSA except using a 5-mL HiTrap IMAC HP column, and omitting detergents from the buffers. Fractions containing cVanSA were pooled and dialyzed against IEX start buffer (50 mM Tris pH 8.0, 50 mM NaCl.) The protein was then loaded on a 5-mL HiTrap Q HP column (GE Life Sciences) and eluted with a gradient (10 column volumes) from 50 to 500 mM NaCl. Fractions containing protein were pooled, concentrated, and loaded onto an S-300 column equilibrated in SEC buffer without detergent. Finally, the protein eluting from the size exclusion column was concentrated to >10 mg/mL and dialyzed into 50 mM Tris pH 7.8, 100 mM NaCl, 5 mM MgCl2, 5% glycerol.

VanRA: The high-speed supernatant was filtered and loaded onto a 5-mL HiTrap IMAC HP column equilibrated in IMAC A buffer. Fractions containing SUMO-VanRA were pooled, concentrated, and dialyzed overnight against IMAC A buffer. 200 μg of the SUMO hydrolase dtUD1 [27] was added to the dialysis bag to cleave the 6xHis-SUMO tag. The dialyzed material was passed over the same HiTrap IMAC HP column, which had been re-equilibrated in IMAC A buffer. The flow-through fractions containing VanRA were pooled, concentrated, and dialyzed against 2 L IEX start buffer. The VanRA was then purified by ion-exchange chromatography, using a 5-mL HiTrap Q HP column as described above. The purified VanRA peak was finally dialyzed against 50 mM Tris pH 7.8, 50 mM NaCl, 5 mM MgCl2, and 5% glycerol.

PhoR: The gene encoding the cytosolic portion of PhoR (residues N166-D431) was amplified from E. coli strain BL21(DE3) and subcloned into the in-house vector pETHM3c. The resulting construct encodes an N-terminally His6-tagged MBP protein connected at its C-terminus to PhoR, via a linker containing the recognition site for the rhinovirus 3c protease. The expression vector was introduced into BL21(DE3) cells. 2-mL overnight cultures were inoculated into 1 L LB medium and grown at 37° to OD600 ~0.4–0.6. Expression was induced with 300 μM IPTG for 2.5 hours. The supernatant from the high-speed centrifugation was filtered and purified by immobilized-metal affinity chromatography as described for other constructs, using a 5-mL HiTrap IMAC HP column. Fractions containing the MBP-PhoR fusion protein were concentrated and dialyzed overnight vs. IEX start buffer and then purified using a 5-mL HiTrap Q HP column, as described for cVanSA. Fractions from this step were directly loaded on a 1.0 cm x 5.0 cm amylose column (NEB Amylose Resin E8021L) equilibrated in 50 mM Tris pH 8.0, 500 mM NaCl. After washing, the bound protein was eluted with 10 mM maltose in the same buffer. The protein was finally dialyzed into 50 mM Tris pH 8.0, 50 mM NaCl, and 10% glycerol.

Differential filtration

The differential filtration assay was performed as described by Vergis et al. [33], using the Analytic Selector kit (Anatrace). Briefy, 500 μg of full-length VanSA was captured using a 20% slurry of His-bind resin (Millipore) in wash buffer (50 mM Tris, 500 mM NaCl, 40 mM imidazole pH 7.7) + 0.1% DDM. The slurry was dispensed into each well of a 0.2 μm filter plate, after which the beads were washed with wash buffer + 0.1% DDM, and then detergent-exchanged into the new detergents from the Analytic Selector kit. The protein was eluted from the His-bind beads and then applied directly to either a small (100 kDa) or large (300 kDa) MWCO filter plate. The eluates from these filtrations were analyzed by dot blot using an anti-6xHis antibody (Proteintech # HRP 66005); blots were scanned using a LI-COR Odyssey-FC imaging system.

Amphipol reconstitution

Purified, concentrated VanSA protein (approx. 150 uM) containing approximately 120 mM LDAO was diluted to 22 uM (1 mg/mL) with 50 mM Tris pH 7.4, 50 mM KCl. An aliquot of a 10% w/v solution of amphipol A8-35 (Anatrace) was added to give a 1:1 mass ratio of protein to amphipol [34], and the solution was incubated on ice for 30 minutes. A quantity of washed BioBeads (BioRad) was added equivalent to 20x the estimated mass of LDAO present, and the solution was mixed at 4° for 2 hours. Pilot ultracentrifugation experiments were used to determine that this treatment gave 100% recovery of the VanSA protein in the supernatant. Once this was confirmed, subsequent experiments omitted the ultracentrifugation step. After detergent removal with the BioBeads, the material was injected onto a Superdex 200 Increase 10/300 GL column (GE Healthcare) equilibrated with 20 mM Tris-Cl pH 7.4, 150 mM NaCl, and the peak corresponding to active VanSA was collected and used for enzymatic assays. A second, later-eluting peak was also observed, but showed substantially lower activity. The nature of this second species was not investigated further, but we did note that the second peak showed almost no dimer band on SDS-PAGE gels, suggesting it might containing VanSA monomers. Addition of 1% C12E8 to the protein solution prior to amphipol reconstitution decreased the relative size of the second peak.

Autophosphorylation

Autophosphorylation was detected as described [35], using the bio-orthogonal ATP analog ATPγS to produce a thiophosphorylated protein. This protein was then treated with the alkylating agent p-nitrobenzyl mesolate (PNBM), and the resulting PNBM-derivatized thiophosphate epitope was identified immunochemically. Briefly, 1 mM ATPγS was added to 15 μM of the histidine kinase in a 15 μL volume using reaction buffer (50 mM Tris pH 7.4, 50 mM KCl, 10 mM MgCl2; for full-length VanSA 9 mM C12E8 was also included). After incubation at room temperature for the desired length of time, the reaction was quenched with 3 μL of 500 mM EDTA, pH 8.0. Then, 1 μL of 50 mM PNBM in 100% DMSO was added and incubated at room temperature for 1 hour, after which 4 μL of 6x sample buffer were added to each reaction before SDS-PAGE. After electrophoresis, the labeled proteins were transferred to a nitrocellulose membrane and blocked with 5% nonfat dry milk in 1x TBST (20 mM Tris, 500 mM NaCl pH 8.0) for 1 hour at room temperature. The membranes were then rocked overnight at 4°C with a 1:5000 dilution of anti-phosphothioester antibody (Abcam ab92570) in 1% milk. The membrane was washed 3x10 mins with TBST, and then incubated for 1 hour at room temperature with a 1:1000 dilution of goat anti-rabbit secondary antibody (Jackson ImmunoResearch HRP-GARIgG 111-035-003) in 1% milk. Finally, the membrane was washed 3x10 mins with TBST before reaction with peroxidase substrate solution for enhanced chemiluminescence (Pierce 32209) and visualized with film. ImageJ was used for quantification and background subtraction [36]. In the case of the full-length VanSA both the monomer and dimer bands were included in the quantification. Background-corrected intensities were normalized to the intensity of the 20-minute time point (corresponding to the maximum intensity observed in the course of the experiment).

Phosphotransfer

Phosphotransfer to VanRA was measured using a variation on the autophosphorylation protocol described above. Prior to the EDTA quenching step, 30 μM VanRA was added to 20 μM full-length VanSA (± 50 μM vancomycin) or 0.66 μM cVanSA. This VanRA was pre-treated with iodoacetamide to reduce alkylation of cysteine residues on the protein and avoid cross-reactivity with the anti-PNBM antibody. The phosphotransfer reactions were allowed to proceed for the desired lengths of time before being quenched with EDTA. Band intensities were background-corrected and normalized to the values obtained at the longest time point (30 minutes).

Dephosphorylation

For dephosphorylation experiments, phospho-VanRA was prepared by phosphorylation with PhoR. Briefly, a 150 μl reaction containing 28 μM MBP-PhoR fusion protein was allowed to autophosphorylate in the presence of 2 mM ATP for 1 hour at room temperature in reaction buffer. The reaction was then desalted twice using Zeba Spin desalting columns (Thermo 89882) to remove nucleotide. The desalted phospho-PhoR was then diluted in a 200 μl reaction to a final concentration of 20 μM, after which 20 μM VanRA was added and phosphotransfer was allowed to proceed for 2 hours at room temperature in reaction buffer. This reaction was then added to 500 μl amylose beads and incubated at room temperature for ~15 minutes to remove the MBP-PhoR. The beads were removed by filtration (0.2 micron centrifugal filter, Pall ODM02C34), and the phospho-VanRA was used to set up dephosphorylation experiments. Concentrations given are nominal; no effort was made to account for dilution occurring during the desalting step or during the amylose bead treatment. Phospho-VanRA was added to reaction buffer to a final concentration of ~7.5 μM, after which the histidine kinase was added to a final concentration of 7.5 μM (with or without 50 μM vancomycin). 15-μL aliquots were removed at various time points and quenched with 3 μL of 6x sample buffer. The samples were then run on a pre-cast Phos-tag gel (50 μM Phos-tag, 12.5% acrylamide; Wako) for 2–3 hours at 30 mA. Gels were stained with Coomassie Blue and photographed, after which band intensities were quantified with ImageJ.

Surface plasmon resonance

All SPR experiments were performed on a BioRad ProteOn XPR36 at 25°C, using immobilized VanRA as the ligand and full-length or cytosolic VanSA constructs as mobile phase analytes. VanRA was immobilized using the Rho1D4 epitope-antibody system [37]. Rho1D4 antibody was obtained from the University of British Columbia (Vancouver, Canada), and covalently attached to a GLC chip (BioRad) via amine coupling. Briefly, the chip surface was activated with a mixture of 20 mM EDC (1-ethyl-3-(3-dimethylaminopropyl)carbodiimide hydrochloride) and 5 mM sulfo-NHS (N-hydroxysulfosuccinimide) at 30 μL/min for 300 sec. 0.5 mg/mL Rho1D4 antibody was then injected on each lane at 30 μL/min for 420 seconds, yielding ~6000–7000 RU immobilized on the surface. The surface was then regenerated with 3 injections of 10 mM NaOH followed by 1% N-octyl-β-D-glucopyranoside (Anatrace, Maumee OH) at 100 μL/min for 18 seconds and equilibrated overnight in running buffer (50 mM BIS-TRIS pH 6.0, 150 mM NaCl, 10 mM MgCl2, and 0.005% Tween 20).

A VanRA construct was prepared with a C-terminal 1D4 epitope tag (amino acid sequence TETSQVAPA), connected to the C-terminus of VanRA by a GGGS linker. To confirm that the epitope tag does not affect protein function, phosphotransfer experiments were carried out, which showed that the 1D4-tagged VanRA is a competent substrate for phosphotransfer (S5 Fig). The tagged VanRA construct was diluted in running buffer to 1–25 μg/mL and passed over the chip at 50 μL/min for 30 seconds, followed by a 240-second dissociation time. This resulted in capture of 200–800 RU of the ligand. This was followed by five blank (buffer only) injections. Serial dilutions of the histidine kinases were prepared in running buffer (+ 9 mM C12E8 in the case of full-length VanSA), and were injected at 100 μL/min with an association time of 240 seconds and a dissociation time of 600 seconds (S4 Fig).

Equilibrium binding responses for the histidine kinases were normalized to the ligand response in each lane, using averaged response values at the end of the association phase, excluding any air bubbles (time points used to determine equilibration response values are shown as gray bars in S4 Fig). These normalized responses were then plotted as a fraction of the theoretical maximum response:

Running buffer without C12E8 was used for the dissociation phase, as inclusion of C12E8 led to bubble formation. However, full-length VanSA proved to be unstable in this buffer and appeared to precipitate on the chip during the dissociation phase. Hence, rather than use global fits of association and dissociation rates to derive KD values, binding affinities were obtained by fitting a one-site binding model to the equilibrium response data.

Fluorescence anisotropy

Cysteine modification was used to attach a fluorophore to VanRA for use in anisotropy experiments. Although VanRA contains multiple cysteine residues, they are not readily labeled by fluorescein maleimide (data not shown). Accordingly, site-directed mutagenesis was used to introduce an additional cysteine at the protein’s N-terminus, instead of the glycine used in the wild-type construct. A 67 μM solution of the cysteine-containing mutant in labeling buffer (50 mM Tris pH 7.8, 100 mM NaCl, 5 mM MgCl2, 0.05% Tween-20) was treated with 0.1 mM TCEP for 20 minutes on ice. A freshly prepared 7 mM solution of fluorescein maleimide (Thermo) in DMSO was then added to give a final fluorescein concentration of 250 μM (corresponding to a final DMSO concentration of 3.5%). The solution was incubated on ice, protected from light, for 1 hr, after which 1/10th volume of 50 mM cysteine in labeling buffer was added. After an additional 20 min incubation, the solution was filtered through a 0.45 micron filter (Pall NanoSep) and loaded onto a Sephacryl S-100 HR column (1 x 45 cm) equilibrated with labeling buffer. The column was eluted isocratically at 15 cm/hr, and fractions containing VanR were pooled, concentrated to approximately 8 μM, and used within several hours for anisotropy experiments. The fluorescently-labeled VanRA proved to be prone to aggregation, and so freshly prepared material was used for every experiment, and the fluorescently-tagged VanRA was not tested in phosphotransfer experiments. However, the structures of the receiver domains of response regulators are conserved [38, 39], making it clear that the N-terminal labeling site is on the opposite face of the receiver domain from the site of VanRA phosphorylation (Asp-53). Hence, modifications at the N-terminus are unlikely to interfere with the protein’s function.

Titration series of cVanSA or MBP (negative control) were prepared in 150 μL binding reactions containing 40 nM fluorescently-labeled VanRA in labeling buffer. Anisotropy measurements were conducted at room temperature using a Tecan Spark microplate reader. Samples were excited at 490 nm and emission read at 525 nm, using a 10 nm bandpass for both emission and excitation. A 510 nm dichroic mirror was used to condition the emitted signal.

Results

Purification of full-length VanSA

Biophysical probes of molecular function require access to pure, active protein. While many in vitro studies of the VanSA protein have focused on its cytosolic fragment, the full-length protein is required to fully understand the details of signal detection and transduction (Fig 1). To complement recent studies that used purified full-length VanSA to examine the protein’s binding and hydrodynamic properties [22, 23], we sought to explore the catalytic activities of VanSA. Therefore, we expressed and purified a full-length construct with a C-terminal His6-tag, using E. coli as a heterologous expression host.

[Figure omitted. See PDF.]

Fig 1. Working model for VanRA-VanSA signaling.

A schematic view is shown for the VanSA protein. The protein comprises three domains: The sensor domain (gray), which includes two predicted transmembrane helices and is responsible for sensing the inducing signal; the dimerization & histidine-phosphotransfer (DHp) domain (green), which includes the conserved histidine that is the site of autophosphorylation; and the catalytic (CA) domain (magenta), which binds nucleotide triphosphate and is responsible for catalyzing histidine phosphorylation. In the absence of vancomycin, VanSA acts as a phosphatase, keeping VanRA in an inactive, dephosphorylated state. Vancomycin induces VanSA to autophosphorylate, after which phospho-VanSA transfers the phosphoryl group to VanRA. Finally, phospho-VanRA activates transcription of the van resistance genes.

https://doi.org/10.1371/journal.pone.0210627.g001

VanSA is a membrane protein, and therefore detergents are required to remove it from the membrane and maintain it in a soluble form. A wide variety of detergents is available, and the idiosyncratic nature of proteins makes it difficult to rationally predict which will be best for any particular protein [40]. For this reason, we empirically screened different detergents for their ability to support various steps in the VanSA purification. We first focused on the extraction step, in which VanSA is solubilized from the membrane fraction. After extracting with different detergents, we centrifuged at high speed, and used Western blotting to detect His-tagged protein in the high-speed supernatant. In this way, we settled upon n-dodecyl-β-D-maltopyranoside (dodecyl maltoside, DDM) for the extraction step. We used immobilized-metal affinity chromatography (IMAC) to purify the extracted VanSA, and then screened 19 different detergents to find ones that allowed VanSA to migrate as a monodisperse peak on a size-exclusion column. Lauryl dimethylamine oxide (LDAO) gave the best results, showing only a small aggregate peak at the void volume (Fig 2). However, we subsequently found that VanSA’s cognate response regulator, VanRA, would sometimes precipitate in the presence of LDAO, confounding efforts to study the interaction between the two proteins. At this point we revisited our choice of solubilizing agents, using a differential filtration assay to screen 96 detergents, while testing for the ability to maintain VanSA in a soluble, unaggregated form [33]. Detergents that satisfied this criterion were then tested to determine if VanRA remained soluble in their presence. Finally, the effect of the detergent on the autophosphorylation assay was assessed. From this effort we identified octaethylene glycol monododecyl ether (C12E8) as a detergent that maintains both proteins in a soluble form and allows for robust autophosphorylation activity. Thus, we use 1% DDM for extraction from the membrane fraction, 10 mM LDAO for IMAC, size-exclusion, and storage, and 9 mM C12E8 for activity assays.

[Figure omitted. See PDF.]

Fig 2. Purification of full-length VanSA.

At left is shown the size-exclusion chromatogram corresponding to the final step of the purification of the full-length VanSA protein. In LDAO, the protein elutes as a single monodisperse peak. At right is a Coomassie-stained SDS-PAGE gel showing the purified VanSA; the asterisk indicates the dimer band.

https://doi.org/10.1371/journal.pone.0210627.g002

Histidine kinases are widely considered to be obligate dimers [26]. In LDAO, VanSA gives a monodisperse peak on a size exclusion column, eluting slightly earlier than the 80 kDa apotransferrin standard (Fig 2). This is consistent with the 45 kDa VanSA protein behaving as an elongated dimer, as is seen for other sensor histidine kinases [23, 38, 41]; however, we note that the presence of bound detergent will increase the hydrodynamic radius of the protein and complicate estimates of size. On a denaturing SDS-PAGE gel, purified VanSA migrates primarily as a monomer, but small amounts of what is evidently an SDS-resistant dimer can also be seen (S2 Fig). By the method described above, we can regularly purify 2–3 mg of well-behaved full-length VanSA from 6 L of culture. In addition, we have prepared a C-terminally His-tagged construct of the cytosolic domain of VanSA (cVanSA); this protein also shows a mobility consistent with a dimer in size exclusion chromatography (data not shown) and yields ~10–12 mg per liter of culture.

Full-length VanSA is autokinase-active

Three activities are typically associated with a sensor histidine kinase: autophosphorylation, phosphotransfer to the cognate response regulator, and dephosphorylation of the response regulator. While all three of these activities have been demonstrated for an MBP-cytosolic VanSA fusion protein [15], little information is available in the literature about the activities of the full-length protein [22, 23, 25]. We began by probing the autokinase activities of our VanSA constructs. Using a non-radioactive autophosphorylation assay [35], we showed that both cVanSA and full-length VanSA are autokinase-active (Fig 3A and 3B). The total levels of phosphorylated protein observed were substantially lower for the full-length protein than for cVanSA (~7x); however, the kinetics of autophosphorylation were similar, with each construct approaching maximum autophosphorylation by 20 minutes (Fig 3B and 3C).

[Figure omitted. See PDF.]

Fig 3. Full-length VanSA displays three enzymatic activities.

(A) Autophosphorylation of VanSA. Equivalent concentrations of full-length and cytosolic VanSA were incubated with 1 mM ATPγS for 20 minutes. Both proteins autophosphorylate, with the cytosolic construct showing an approximately seven-fold higher level of autophosphorylation. Phosphorylation was detected by alkylation of the thiophosphoryl group with PNBM, followed by immunodetection as described in the Methods section. After quantification, blots were stripped and re-probed with an anti-6xHis antibody to verify consistent loading levels. (B) Time course of phosphorylation for the full-length and cytosolic VanSA constructs. The two time courses were run on the same gel, but are shown as separate panels with different exposures for optimal visualization. Representative gels are shown; the graph in panel (C) shows the quantification of three separate autophosphorylation experiments. Band intensities are normalized to the level of phospho-cVanSA at 20 minutes. (D) Phosphotransfer from VanSA to VanRA. Full-length phospho-VanSA (20 μM) or phospho-cVanSA (0.66 μM) were mixed with 30 μM VanRA, and the reaction was quenched at the times indicated. The graph in panel (E) shows the quantification of three separate phosphotransfer experiments; phospho-VanRA levels are normalized to the levels found at 30 minutes for each kinase. (F) Dephosphorylation of phospho-VanRA. VanSA (7.5 μM) was added to phospho-VanRA and aliquots were removed and quenched at the times indicated. Samples were run on Phos-tag gels to separate phosphorylated and unphosphorylated VanRA and stained with Coomassie Brilliant Blue. Experiments containing VanRA alone (i.e., no added VanSA) are used to determine the intrinsic decay rate of phospho-VanRA. Panel (G) shows the averages of at least three such experiments, with phospho-VanRA amounts being normalized to their starting levels. The asterisks indicate time points for which phospho-protein levels are significantly different (p < 0.01) between the VanRA-alone experiments (dashed lines) and those containing either full-length VanSA or cVanSA (solid lines). The lines shown represent fits of exponential decay curves to the data.

https://doi.org/10.1371/journal.pone.0210627.g003

Phosphotransfer from full-length VanSA to VanRA

After autophosphorylation, the next step in the signaling process is transfer of the phosphoryl group from the histidine kinase to the response regulator. In order to determine if our cVanSA and full-length VanSA proteins were able to participate in phosphotransfer to VanRA, we performed a variation on the autophosphorylation assay described above (Fig 3D and 3E). Both cVanSA and full-length VanSA were found to readily transfer phosphoryl groups to VanRA. For cVanSA the rate of phosphotransfer is very fast, with maximum transfer being achieved within a few seconds, while for full-length VanSA, phosphotransfer is slower, with maximum transfer being observed within 10 minutes.

Full-length VanSA dephosphorylates phospho-VanRA

Finally we assessed the ability of our VanSA constructs to dephosphorylate phospho-VanRA. These assays require preparation of phosphorylated VanRA, followed by initiation of dephosphorylation by addition of the histidine kinase; they are complicated by the intrinsic lability of the response regulator’s phospho-aspartate moiety [42]. We chose to use a non-radioactive Phos-tag assay to measure the half-life of phosphorylated VanRA in the presence and absence of VanSA [42–44]. Phospho-VanRA was generated using a non-cognate histidine kinase, E. coli PhoR. PhoR has previously been shown to promiscuously phosphorylate VanRA in an intracellular E. coli system [45], and the purified cytosolic domain of PhoR proved to efficiently transfer a phosphoryl group to the VanRA in vitro. After phosphorylating the response regulator, we removed the PhoR and monitored decay of phospho-VanRA over time. We found that the intrinsic half-life of phospho-VanRA (reflecting its decay rate in the absence of any added VanSA protein) was acutely sensitive to temperature; at the ambient temperature in our laboratory (which typically falls between 20 and 25° C), the measured half-life was approximately 3.5 hours (Fig 3), slightly less than half the value reported by Wright et al. under somewhat different conditions [15]. Addition of either cVanSA or full-length VanSA significantly hastened the breakdown of the phospho-VanRA, reflecting active dephosphorylation. Under these assay conditions, the full-length protein was less efficient than the cytosolic construct at catalyzing dephosphorylation.

VanSA has low micromolar affinity for VanRA

In some two-component systems, sensor histidine kinases have been reported to bind specifically to their cognate response regulators [46]. To assess the interaction between VanSA and VanRA, we used surface plasmon resonance. We immobilized VanRA via a C-terminal epitope tag and used the full-length and cytosolic histidine kinases as analytes in the mobile phase. Both constructs bound to VanRA with dissociation constants (KD) in the low micromolar range, consistent with the affinities found for other histidine kinase-response regulator pairs [46–53] (Table 1). Full-length VanSA was seen to bind VanRA ~3x more tightly than the isolated cytosolic domain. When the cytosolic VanSA was allowed to autophosphorylate immediately before the binding experiment, a modest increase in affinity was observed, suggesting that VanRA may bind the phospho-histidine form of VanSA more tightly; however, it must be noted that the cVanSA was not expected to be fully phosphorylated in this experiment, and the amount of phosphorylated material may also change over the course of the analysis, making interpretation of this result difficult.

[Figure omitted. See PDF.]

Table 1. Binding affinities for VanRA and VanSA constructs.

https://doi.org/10.1371/journal.pone.0210627.t001

To confirm the interaction between VanSA and VanRA, we employed fluorescence anisotropy as an orthogonal method. Only the cytosolic VanSA construct was used, to avoid non-specific interactions between hydrophobic fluorophore and detergent micelles. These experiments confirmed a specific binding interaction between cytosolic VanSA and VanRA (S4 Fig), giving a slightly lower KD value than that derived from the SPR experiments. The reason for the difference in KD estimates is not yet clear, but both methods consistently demonstrate specific binding between the purified sensor histidine kinase and its cognate partner.

Vancomycin does not alter the activity of full-length VanSA

If VanSA directly recognizes the vancomycin molecule, it makes sense that antibiotic binding should function as a trigger to alter the catalytic properties of the enzyme. To probe whether vancomycin influences any of the enzymatic activities of VanSA, we assayed for autophosphorylation, phosphotransfer, and dephosphorylation in the presence of 50 μM vancomycin, which is ~50x the typical minimum inhibitory concentration (MIC) seen for vancomycin-sensitive enterococcal strains [54, 55]. In none of these assays did vancomycin significantly alter the enzymatic activity of full-length VanSA (Fig 4); in fact, no effect was seen even when vancomycin concentration was increased to 200 μM (data not shown).

[Figure omitted. See PDF.]

Fig 4. Vancomycin does not affect activity of full-length VanSA.

(A) Autophosphorylation activity of VanSA ± 50 μM vancomycin. Protein (15 μM) was incubated with or without 1 mM ATPγS for the times indicated. Panel (B) shows the quantification, displaying phospho-VanSA band intensities normalized to the level attained at 20 minutes in the absence of vancomycin. (C) Phosphotransfer activity. 20 μM phospho-VanSA was mixed with 30 μM VanRA (± 50 μM vancomycin) and quenched at the times indicated. Panel (D) shows the quantification; phospho-VanRA band intensities are normalized to the level attained in the 30-min reaction in the absence of vancomycin. (E) Dephosphorylation activity. 7.5 μM VanSA (± 50 μM vancomycin) was added to ~7.5 μM phospho-VanRA, and aliquots were removed and quenched at the times indicated. Panel (F) shows the quantification with amounts of phospho-VanRA normalized to their starting values. Fitting decay curves to these data gives slightly different estimates for the phospho-VanRA half-life in the presence and absence of vancomycin; however, a t-test indicates that at each time point, the values with and without antibiotic are not significantly different. Error bars in the quantification plots represent standard deviations of at least three independent experiments.

https://doi.org/10.1371/journal.pone.0210627.g004

Consequences of a potential activating mutation

While detergent is necessary to extract the protein from the membrane and maintain it in soluble form, its use complicates the analysis of the protein’s activity, as noted above. In light of our observation that vancomycin fails to affect VanSA’s catalytic activities, we wished to be certain that the detergent was not altering the fundamental properties of the protein. To test for this, we probed whether detergent would alter the behavior of a VanSA mutant expected to be constitutively active, reasoning that if detergent is causing unphysiological behavior, it will likely perturb the constitutive behavior of the mutant.

We were unable to find documented examples of specific mutations in VanSA that confer a constitutive phenotype. However, mutations associated with such a phenotype have been found in related VanS proteins. For example, in B-type VRE strains the T237K and T237M mutations have both been found in constitutively active variants [56, 57]. In the VanSB protein, Thr-237 is four residues (one turn of a helix) downstream of the site of histidine phosphorylation. A similar mutation has been described in D-type strains, where a mutation in the corresponding residue (T170I) was found in a constitutive strain [58]. More generally, it appears that the presence of a threonine or asparagine four residues downstream of the phosphorylated histidine is an important determinant of phosphatase activity in histidine kinases [59, 60]. Accordingly, we chose to mutate the corresponding threonine residue in VanSA, Thr-168, to lysine, mimicking the T237K mutation in VanSB. When purified, the detergent-solubilized T168K VanSA mutant exhibited an autophosphorylation activity comparable to that of the wild-type protein, but its phosphatase activity was significantly impaired (Fig 5). Thus, it is clear that the T168K substitution perturbs the balance between autophosphorylation and phosphatase activities of the purified protein, consistent with the expected constitutive activity. Importantly, this observation increases confidence that detergent is not eliciting new or unphysiological behaviors in VanSA.

[Figure omitted. See PDF.]

Fig 5. Autophosphorylation and phosphatase activities of the T168K mutant.

(A) Representative autophosphorylation assays for wild-type and mutant VanSA. No significant difference is seen in the autokinase activities of the two proteins. (B) Dephosphorylation activities of wild-type (black solid line) and mutant VanSA (red). Asterisks indicate time points for which levels of phospho-VanRA are significantly different (p < 0.05) for the two proteins. At all time points, the phospho-VanRA levels seen with the mutant protein are not significantly different from those seen with VanRA alone (black dotted line).

https://doi.org/10.1371/journal.pone.0210627.g005

Amphipol trapping of VanSA

Another way to approach the question of whether detergents are affecting VanSA activity is to transfer the protein to a different environment. One such environment is provided by amphipols, which are amphipathic polymers designed to wrap around a membrane protein’s hydrophobic surfaces and mask them from aqueous solvent [61]. Because each polymer makes multiple hydrophobic contacts with the protein, amphipols bind membrane proteins tightly, and exhibit a very slow rate of unbinding [34]. Accordingly, we transferred VanSA from detergent solution to the most commonly used amphipol, A8-35, and removed the detergent using BioBead treatment followed by gel filtration. The resulting VanSA-amphipol complex migrates as a single peak on a size-exclusion column (Fig 6A), demonstrating that the protein remains stable and homogeneous even after the removal of detergent. In contrast, the same detergent removal protocol, when performed in the absence of amphipol, results in the complete precipitation of the protein (data not shown). Interestingly, transferring the protein from detergent solution to an amphipol environment significantly enhances its autophosphorylation and phosphatase activities (Fig 6B and 6D). Critically, while the basal levels for these activities increase substantially, the activities themselves remain insensitive to vancomycin in the amphipol-solubilized protein (Fig 6C).

[Figure omitted. See PDF.]

Fig 6. Reconstitution of full-length VanSA with the amphipol A8-35.

(A) Size-exclusion chromatogram of amphipol-reconstituted VanSA, demonstrating the presence of a single soluble and homogeneous species. (B) Comparison of autophosphorylation activity for VanSA in detergent solution vs. amphipols. The amphipol-reconstituted species exhibits substantially higher enzymatic activity. This is demonstrated in the anti-6xHis loading control, which shows that small amounts of the protein-plus-amphipol solution give essentially equivalent activity to much larger amounts of the detergent-solubilized protein. (C) 50 μM vancomycin has no effect on the autophosphorylation activity of amphipol-reconstituted VanSA. (D) & (E) 50 μM vancomycin has no effect on the phosphatase activity of amphipol-reconstituted VanSA. Panel (D) shows a representative Phos-tag gel, with panel (E) showing the quantification of assays involving three independent sets of measurements.

https://doi.org/10.1371/journal.pone.0210627.g006

Discussion

Biochemical and biophysical studies benefit greatly from the ability to reconstitute functional complexes from purified components. For a signaling complex such as the VanR-VanS system, access to isolated proteins allows for the removal of complicating factors, such as the contributions of cross-talk from other cellular proteins and the effects of non-enzymatic phosphorylation by small-molecule phospho-donors. Additionally, obtaining purified full-length protein is particularly important in the case of VanS, in order to address the question of whether vancomycin binds directly to VanS to modulate its activity. We have purified the full-length VanSA protein associated with type-A enterococcal resistance, and demonstrate that the detergent-solubilized VanSA demonstrates all three enzymatic activities expected of a histidine kinase, namely autophosphorylation, phosphotransfer to its cognate response regulator, and dephosphorylation of the response regulator. We also describe a likely constitutively active mutant with impaired phosphatase activity, and describe a protocol for generating a detergent-free, amphipol-solubilized form of the protein, for which enzymatic activity levels are significantly enhanced to the detergent-solubilized form. It is instructive to compare the activities of these full-length VanSA protein preparations to those of the isolated cytoplasmic domain, which lacks the regulatory capabilities conferred by the transmembrane sensor domain.

In detergent solutions, the full-length VanSA protein exhibits lower autophosphorylation and phosphatase activities than the cytosolic domain (Fig 3A). The rate of phosphotransfer catalyzed by full-length VanSA also appears slightly slower than that seen with the cytoplasmic domain (Fig 3D and 3E), but this probably reflects different starting levels of phospho-histidine—because the phospho-histidine is a substrate in the bi-molecular phosphotransfer reaction, lower levels will translate into a lower apparent phosphotransfer rate. Indeed, one expects that phosphotransfer rates should be similar for both the cytosolic and full-length constructs, since in most two-component systems, the catalytic machinery for phosphotransfer resides primarily in the response regulator, rather than in the histidine kinase [8].

To determine whether the lower activity observed with full-length VanSA in detergent reflects a regulatory effect contributed by the protein’s transmembrane region, or a nonspecific detergent effect, we used amphipol A8-35 [62] as an alternative means of solubilizing the protein. In the amphipol-solubilized form, the protein regains high levels of activity, comparable to those observed for the cytosolic construct. Therefore, it does appear that detergent is suppressing the enzymatic activity of the protein. This is consistent with the published report that VanSA autokinase activity is exquisitely sensitive to DDM concentration [25]. To assess whether the detergent effect reflects direct inhibition of the protein’s catalytic machinery, one can examine the effects of detergent on the activity of the cytoplasmic construct; however, such experiments do not reveal any drastic changes in activity (S3 Fig). Hence, it seems likely that the detergent effects observed are a manifestation of structural and/or dynamic changes in the protein, such as perturbations in monomer-dimer equilibrium or subtle alterations in helix packing. The reduced activity therefore indicates that the micellar environment provided by the detergent does not mimic the native membrane environment with complete fidelity.

However, while detergents may reduce the activity of VanSA, there is reason to believe that they are not drastically altering the intrinsic properties of the enzyme. Specifically, we have created a constitutively activated form of VanSA, T168K, in which we removed a conserved threonine lying one turn of a helix downstream of the phosphorylated histidine. This mutation is predicted to reduce or completely remove phosphatase activity [59], and indeed in the mutant protein the phosphatase activity is reduced to unmeasurable levels, while the autokinase activity remains unchanged.

Perhaps the most interesting results to emerge from this work speak to the question of whether vancomycin and related antibiotics are sensed directly, via a molecular interaction with VanSA, or indirectly, via detection of a downstream consequence of antibiotic action. We show that high concentrations of vancomycin do not alter the enzymatic properties of VanSA, regardless of whether the protein is solubilized in detergent or with an amphipol. We studied vancomycin concentrations ranging from ca. 50-fold to 200-fold above the MIC levels for vancomycin-sensitive enterococci. Presumably, vancomycin-resistant enterococci must sense the antibiotic and mount a defensive response well before such a toxic threshold is reached; this implies that if the antibiotic is to exert a direct effect on VanSA’s enzymatic function, this effect should occur well below the concentrations we have tested.

We note that our results appear to conflict with a report that vancomycin modestly increases turnover in a general ATPase assay [22]. However, the relevance of such an ATPase assay is unclear, since the turnover numbers reported indicate many rounds of ATP hydrolysis per VanS molecule per minute. Such rapid ATP turnover is inconsistent with the stable VanS histidine phosphorylation observed by us (this work) and others [15], and would represent highly unusual behavior for a sensor histidine kinase. In contrast to the general ATPase assay, the activity measurements we report reflect physiologically relevant enzymatic activities directly related to the biological function of the VanSA protein. Vancomycin’s failure to alter these activities in our purified system argues against a direct sensing mechanism involving a binary antibiotic-VanSA complex. Of course, it is possible that direct sensing does occur, but requires additional partners that are not present in our minimal system; it is also possible that a natural inhibitor of VanSA is missing from our system, and its absence leads the enzyme to adopt a fully active form, incapable of further stimulation by antibiotic.

We stress that our experiments measure activity, not binding, and therefore do not specifically address the question of whether vancomycin binds directly with VanSA. Recent reports have shown that vancomycin can elicit spectroscopic and hydrodynamic changes in purified full-length VanSA [22, 23], which are interpreted as evidence for direct binding of the antibiotic by the protein [63]. This argument suggests that vancomycin may indeed be binding VanSA in our assays, even though any such binding is not reflected by a change in enzymatic activity. However, an important caveat is that the Kd values inferred from the binding experiments are approximately 70 uM, and, as discussed above, it is difficult to reconcile such high dissociation constants with the much lower MIC values seen in vancomycin-sensitive organisms.

Conclusions

In summary, we have characterized the enzymatic properties of full-length VanSA, using both detergent and amphipols to solubilize this membrane-bound protein. Both forms of the protein exhibit all three of the activities expected from a sensor histidine kinase, with the amphipol-solubilized material showing significantly higher levels of activity overall. Vancomycin, the putative inducer of the VanR-VanS two-component system, does not alter the enzymatic activity of either form of the protein, suggesting that either the antibiotic does not interact directly with VanSA, or that additional factors are required to confer vancomycin sensing upon the protein.

Supporting information

[Figure omitted. See PDF.]

S1 Table. Primers used to prepare expression constructs.

https://doi.org/10.1371/journal.pone.0210627.s001

(DOCX)

S1 Fig. VanRA and VanSA proteins used in this study.

Our full-length VanSA construct contains 392 amino acids (including the C-terminal PG-6xHis tag). The cytosolic VanSA construct begins at Lys-98, immediately after the second predicted transmembrane domain; it contains two residues at the N-terminus (MV) that were contributed by the vector. The VanRA construct was expressed as a fusion protein with an N-terminal, 6xHis-SUMO tag. After removal of the SUMO partner, the protein contains the full VanRA sequence, along with a single additional glycine residue at the N-terminus (contributed by the vector).

https://doi.org/10.1371/journal.pone.0210627.s002

(TIF)

S2 Fig. Electrophoresis of full-length VanSA reveals a covalent, disulfide-linked dimer.

In denaturing SDS-PAGE, the main band for purified VanSA migrates at the expected monomer molecular weight, 45 kDa. However, a second band is consistently observed at ~90 kDa, corresponding to the molecular weight of a dimer (labeled with an asterisk in the gels shown). This upper band is labeled in both the anti-6xHis Western blot and in the anti-PNBM blot used for the autophosphorylation assay. Together, these facts point to this upper band being a VanSA dimer. SDS-resistant oligomers are commonly seen for membrane proteins, but we also considered the possibility that this band might represent a disulfide-linked dimer, since VanSA contains a single cysteine near the end of the second predicted transmembrane helix. The upper band withstands treatment with normal loading buffer, which contains a final concentration of 0.1 M DTT (panel A, left lane). However, we reasoned that the DTT may have become oxidized and lost efficacy after several freeze-thaw cycles, and therefore tested exposure to either 50 mM TCEP or fresh 5% β-mercaptoethanol for 10 minutes before adding loading buffer. Both of these treatments removed the upper band (panel B), indicating that it is indeed a disulfide-linked dimer.

https://doi.org/10.1371/journal.pone.0210627.s003

(TIF)

S3 Fig. Effect of C12E8 on enzymatic activities of cVanSA.

(A) C12E8 has at most a modest effect on autophosphorylation. Upper panel shows an anti-PNBM blot labeling phosphorylated cVanSA in the presence and absence of 9 mM C12E8. The anti-6xHis blot is used as a loading control. The quantitation of the autophosphorylation is shown in panel (B); band intensities are normalized to the intensity of the 20-minute time point for the detergent-free reaction. (C) Phosphotransfer is not significantly affected by the presence of C12E8. Upper panel shows an anti-PNBM blot in which both phosphorylated cVanSA and VanRA are labeled; lower panel shows an anti-6xHis blot serving as a loading control for His6-tagged cVanSA. (D) Quantitation plot for phosphotransfer reaction; band intensities for phospho-VanRA are normalized to the phospho-VanRA level at 30 minutes produced by cytosolic VanSA in the absence of C12E8. (E) Effect of C12E8 on the rate of cVanSA-catalyzed dephosphorylation of phospho-VanRA. Here we show the data from the average of 3 experiments and the fitted half-life curves for dephosphorylation with and without 9 mM C12E8. A modest reduction of activity is seen at the 2-hour time point (p < 0.05), but not at earlier time points.

https://doi.org/10.1371/journal.pone.0210627.s004

(TIF)

S4 Fig. VanRA binding by VanSA and PhoR probed by SPR.

Panels (A) through (C): At left are shown representative sensorgrams from SPR experiments using immobilized VanRA. The analytes used were as follows: (A) cVanSA, (B) full-length VanSA, and (C) autophosphorylated cVanSA. The corresponding normalized equilibrium response fits are shown at right. Concentrations shown are for dimers of the histidine kinases. Gray boxes in the sensograms represent the response range used to determine the equilibrium fit. (D) Verification of VanRA binding by cVanSA using fluorescence anisotropy. A representative binding curve is shown for cVanSA binding to fluorescently labeled VanRA. The overall change in anisotropy is small, as expected for the binding of a medium-sized protein such as VanRA to a medium-sized partner. However, the binding experiments yielded reproducible results with each fresh preparation of fluorescein-labeled VanRA. The curve shown represents a binding isotherm corresponding to a KD values of 0.2 μM. Experiments done on different days with different preparations of fluorescently labeled VanRA consistently gave KD values in the range of 0.1 to 1.0 μM.

https://doi.org/10.1371/journal.pone.0210627.s005

(TIF)

S5 Fig. 1D4-tagged VanRA is a competent substrate for phosphotransfer.

An anti-PNBM blot shows the time course of phosphotransfer from cytosolic VanSA to wild-type VanRA (left) and 1D4-tagged VanRA (right). For both VanRA constructs, rapid phosphotransfer is observed (within the mixing time of the experiment), followed by gradual loss of signal due to the phosphatase activity of VanSA. The 1D4-tagged construct migrates at a slightly larger molecular weight than the wild-type VanRA protein, owing to the additional 13 residues contributed by the linker and epitope tag.

https://doi.org/10.1371/journal.pone.0210627.s006

(TIF)

Acknowledgments

We gratefully acknowledge Simon Cocklin for assistance with the SPR experiments and Shae Padrick for consultation on the anisotropy experiments.

Citation: Upton EC, Maciunas LJ, Loll PJ (2019) Vancomycin does not affect the enzymatic activities of purified VanSA. PLoS ONE 14(1): e0210627. https://doi.org/10.1371/journal.pone.0210627

References

1. Arias CA, Murray BE. The rise of the Enterococcus: beyond vancomycin resistance. Nat Rev Microbiol. 2012;10(4):266–78. pmid:22421879; PubMed Central PMCID: PMCPMC3621121.

2. Reyes K, Bardossy AC, Zervos M. Vancomycin-Resistant Enterococci: Epidemiology, Infection Prevention, and Control. Infect Dis Clin North Am. 2016;30(4):953–65. pmid:27660091.

3. Arthur M, Courvalin P. Genetics and mechanisms of glycopeptide resistance in enterococci. Antimicrob Agents Chemother. 1993;37(8):1563–71. pmid:8215264; PubMed Central PMCID: PMCPMC188020.

4. O'Driscoll T, Crank CW. Vancomycin-resistant enterococcal infections: epidemiology, clinical manifestations, and optimal management. Infect Drug Resist. 2015;8:217–30. pmid:26244026; PubMed Central PMCID: PMCPMC4521680.

5. Bugg TD, Wright GD, Dutka-Malen S, Arthur M, Courvalin P, Walsh CT. Molecular basis for vancomycin resistance in Enterococcus faecium BM4147: biosynthesis of a depsipeptide peptidoglycan precursor by vancomycin resistance proteins VanH and VanA. Biochemistry. 1991;30(43):10408–15. pmid:1931965.

6. McComas CC, Crowley BM, Boger DL. Partitioning the loss in vancomycin binding affinity for D-Ala-D-Lac into lost H-bond and repulsive lone pair contributions. J Am Chem Soc. 2003;125(31):9314–5. pmid:12889959.

7. Walsh CT, Fisher SL, Park IS, Prahalad M, Wu Z. Bacterial resistance to vancomycin: five genes and one missing hydrogen bond tell the story. Chem Biol. 1996;3(1):21–8. pmid:8807824.

8. Zschiedrich CP, Keidel V, Szurmant H. Molecular Mechanisms of Two-Component Signal Transduction. J Mol Biol. 2016;428(19):3752–75. pmid:27519796; PubMed Central PMCID: PMCPMC5023499.

9. Ulrich LE, Zhulin IB. The MiST2 database: a comprehensive genomics resource on microbial signal transduction. Nucleic Acids Res. 2010;38(Database issue):D401–7. pmid:19900966; PubMed Central PMCID: PMCPMC2808908.

10. Ortet P, Whitworth DE, Santaella C, Achouak W, Barakat M. P2CS: updates of the prokaryotic two-component systems database. Nucleic Acids Res. 2015;43(Database issue):D536–41. pmid:25324303; PubMed Central PMCID: PMCPMC4384028.

11. Arthur M, Molinas C, Courvalin P. The VanS-VanR two-component regulatory system controls synthesis of depsipeptide peptidoglycan precursors in Enterococcus faecium BM4147. J Bacteriol. 1992;174(8):2582–91. Epub 1992/04/01. pmid:1556077; PubMed Central PMCID: PMC205897.

12. Arthur M, Depardieu F, Courvalin P. Regulated interactions between partner and non-partner sensors and response regulators that control glycopeptide resistance gene expression in enterococci. Microbiology. 1999;145 (Pt 8):1849–58. pmid:10463151.

13. Haldimann A, Fisher SL, Daniels LL, Walsh CT, Wanner BL. Transcriptional regulation of the Enterococcus faecium BM4147 vancomycin resistance gene cluster by the VanS-VanR two-component regulatory system in Escherichia coli K-12. J Bacteriol. 1997;179(18):5903–13. pmid:9294451; PubMed Central PMCID: PMCPMC179483.

14. Holman TR, Wu Z, Wanner BL, Walsh CT. Identification of the DNA-binding site for the phosphorylated VanR protein required for vancomycin resistance in Enterococcus faecium. Biochemistry. 1994;33(15):4625–31. Epub 1994/04/19. pmid:8161518.

15. Wright GD, Holman TR, Walsh CT. Purification and characterization of VanR and the cytosolic domain of VanS: a two-component regulatory system required for vancomycin resistance in Enterococcus faecium BM4147. Biochemistry. 1993;32(19):5057–63. Epub 1993/05/18. pmid:8494882.

16. Koteva K, Hong HJ, Wang XD, Nazi I, Hughes D, Naldrett MJ, et al. A vancomycin photoprobe identifies the histidine kinase VanSsc as a vancomycin receptor. Nat Chem Biol. 2010;6(5):327–9. Epub 2010/04/13. pmid:20383152.

17. Kwun MJ, Novotna G, Hesketh AR, Hill L, Hong HJ. In vivo studies suggest that induction of VanS-dependent vancomycin resistance requires binding of the drug to D-Ala-D-Ala termini in the peptidoglycan cell wall. Antimicrob Agents Chemother. 2013;57(9):4470–80. Epub 2013/07/10. pmid:23836175; PubMed Central PMCID: PMC3754309.

18. Baptista M, Depardieu F, Courvalin P, Arthur M. Specificity of induction of glycopeptide resistance genes in Enterococcus faecalis. Antimicrob Agents Chemother. 1996;40(10):2291–5. Epub 1996/10/01. pmid:8891132; PubMed Central PMCID: PMC163522.

19. Ulijasz AT, Grenader A, Weisblum B. A vancomycin-inducible lacZ reporter system in Bacillus subtilis: induction by antibiotics that inhibit cell wall synthesis and by lysozyme. J Bacteriol. 1996;178(21):6305–9. Epub 1996/11/01. pmid:8892834; PubMed Central PMCID: PMC178505.

20. Handwerger S, Kolokathis A. Induction of vancomycin resistance in Enterococcus faecium by inhibition of transglycosylation. FEMS Microbiol Lett. 1990;58(2):167–70. pmid:2227352.

21. Allen NE, Hobbs JN Jr. Induction of vancomycin resistance in Enterococcus faecium by non-glycopeptide antibiotics. FEMS Microbiol Lett. 1995;132(1–2):107–14. pmid:7590155.

22. Hughes CS, Longo E, Phillips-Jones MK, Hussain R. Characterisation of the selective binding of antibiotics vancomycin and teicoplanin by the VanS receptor regulating type A vancomycin resistance in the enterococci. Biochimica et biophysica acta. 2017;1861(8):1951–9. pmid:28511809; PubMed Central PMCID: PMCPMC5482315.

23. Phillips-Jones MK, Channell G, Kelsall CJ, Hughes CS, Ashcroft AE, Patching SG, et al. Hydrodynamics of the VanA-type VanS histidine kinase: an extended solution conformation and first evidence for interactions with vancomycin. Sci Rep. 2017;7:46180. pmid:28397853; PubMed Central PMCID: PMCPMC5387412.

24. Hughes CS, Longo E, Phillips-Jones MK, Hussain R. Quality control and biophysical characterisation data of VanSA. Data Brief. 2017;14:41–7. Epub 2017/08/03. pmid:28765830; PubMed Central PMCID: PMCPMC5526436.

25. Hussain R, Harding SE, Hughes CS, Ma P, Patching SG, Edara S, et al. Purification of bacterial membrane sensor kinases and biophysical methods for determination of their ligand and inhibitor interactions. Biochem Soc Trans. 2016;44(3):810–23. pmid:27284046; PubMed Central PMCID: PMCPMC4900758.

26. Jacob-Dubuisson F, Mechaly A, Betton JM, Antoine R. Structural insights into the signalling mechanisms of two-component systems. Nat Rev Microbiol. 2018;16(10):585–93. Epub 2018/07/17. pmid:30008469.

27. Weeks SD, Drinker M, Loll PJ. Ligation independent cloning vectors for expression of SUMO fusions. Protein Expr Purif. 2007;53(1):40–50. pmid:17251035; PubMed Central PMCID: PMCPMC1892228.

28. Zheng L, Baumann U, Reymond JL. An efficient one-step site-directed and site-saturation mutagenesis protocol. Nucleic Acids Res. 2004;32(14):e115. Epub 2004/08/12. pmid:15304544; PubMed Central PMCID: PMCPMC514394.

29. Sonnhammer EL, von Heijne G, Krogh A. A hidden Markov model for predicting transmembrane helices in protein sequences. Proc Int Conf Intell Syst Mol Biol. 1998;6:175–82. pmid:9783223.

30. Krogh A, Larsson B, von Heijne G, Sonnhammer EL. Predicting transmembrane protein topology with a hidden Markov model: application to complete genomes. J Mol Biol. 2001;305(3):567–80. pmid:11152613.

31. Studier FW. Protein production by auto-induction in high density shaking cultures. Protein Expr Purif. 2005;41(1):207–34. pmid:15915565.

32. Eriks LR, Mayor JA, Kaplan RS. A strategy for identification and quantification of detergents frequently used in the purification of membrane proteins. Anal Biochem. 2003;323(2):234–41. Epub 2003/12/06. pmid:14656530.

33. Vergis JM, Purdy MD, Wiener MC. A high-throughput differential filtration assay to screen and select detergents for membrane proteins. Anal Biochem. 2010;407(1):1–11. pmid:20667442; PubMed Central PMCID: PMCPMC4586162.

34. Zoonens M, Zito F, Martinez KL, Popot J-L. Amphipols: A general introduction and some protocols. In: Mus-Veteau I, editor. Membrane Proteins Production for Structural Analysis. New York: Springer; 2014. p. 173–203.

35. Carlson HK, Plate L, Price MS, Allen JJ, Shokat KM, Marletta MA. Use of a semisynthetic epitope to probe histidine kinase activity and regulation. Anal Biochem. 2010;397(2):139–43. pmid:19819215; PubMed Central PMCID: PMCPMC2812668.

36. Schneider CA, Rasband WS, Eliceiri KW. NIH Image to ImageJ: 25 years of image analysis. Nat Methods. 2012;9(7):671–5. pmid:22930834; PubMed Central PMCID: PMCPMC5554542.

37. Molday LL, Molday RS. 1D4: a versatile epitope tag for the purification and characterization of expressed membrane and soluble proteins. Methods Mol Biol. 2014;1177:1–15. pmid:24943310; PubMed Central PMCID: PMCPMC4227631.

38. Gao R, Stock AM. Biological insights from structures of two-component proteins. Annu Rev Microbiol. 2009;63:133–54. pmid:19575571; PubMed Central PMCID: PMCPMC3645274.

39. Bourret RB. Receiver domain structure and function in response regulator proteins. Curr Opin Microbiol. 2010;13(2):142–9. pmid:20211578; PubMed Central PMCID: PMCPMC2847656.

40. Loll PJ. Membrane proteins, detergents and crystals: what is the state of the art? Acta Crystallogr F Struct Biol Commun. 2014;70(Pt 12):1576–83. pmid:25484203; PubMed Central PMCID: PMCPMC4259217.

41. Cheung J, Hendrickson WA. Sensor domains of two-component regulatory systems. Curr Opin Microbiol. 2010;13(2):116–23. pmid:20223701; PubMed Central PMCID: PMCPMC3078554.

42. Gao R, Stock AM. Quantitative Analysis of Intracellular Response Regulator Phosphatase Activity of Histidine Kinases. Methods Enzymol. 2018;607:301–19. Epub 2018/08/29. pmid:30149863; PubMed Central PMCID: PMCPMC6116529.

43. Kinoshita E, Kinoshita-Kikuta E, Takiyama K, Koike T. Phosphate-binding tag, a new tool to visualize phosphorylated proteins. Mol Cell Proteomics. 2006;5(4):749–57. pmid:16340016.

44. Barbieri CM, Stock AM. Universally applicable methods for monitoring response regulator aspartate phosphorylation both in vitro and in vivo using Phos-tag-based reagents. Anal Biochem. 2008;376(1):73–82. Epub 2008/03/11. pmid:18328252; PubMed Central PMCID: PMC2504525.

45. Silva JC, Haldimann A, Prahalad MK, Walsh CT, Wanner BL. In vivo characterization of the type A and B vancomycin-resistant enterococci (VRE) VanRS two-component systems in Escherichia coli: a nonpathogenic model for studying the VRE signal transduction pathways. Proc Natl Acad Sci U S A. 1998;95(20):11951–6. pmid:9751771; PubMed Central PMCID: PMCPMC21746.

46. Willett JW, Tiwari N, Muller S, Hummels KR, Houtman JC, Fuentes EJ, et al. Specificity residues determine binding affinity for two-component signal transduction systems. MBio. 2013;4(6):e00420–13. pmid:24194534; PubMed Central PMCID: PMCPMC3892784.

47. King ST, Kenney LJ. Application of fluorescence resonance energy transfer to examine EnvZ/OmpR interactions. Methods Enzymol. 2007;422:352–60. pmid:17628148.

48. Mattison K, Kenney LJ. Phosphorylation alters the interaction of the response regulator OmpR with its sensor kinase EnvZ. J Biol Chem. 2002;277(13):11143–8. pmid:11799122.

49. Yoshida T, Cai S, Inouye M. Interaction of EnvZ, a sensory histidine kinase, with phosphorylated OmpR, the cognate response regulator. Mol Microbiol. 2002;46(5):1283–94. pmid:12453215.

50. Bhattacharya M, Biswas A, Das AK. Interaction analysis of TcrX/Y two component system from Mycobacterium tuberculosis. Biochimie. 2010;92(3):263–72. pmid:19962420.

51. Bauer J, Reiss K, Veerabagu M, Heunemann M, Harter K, Stehle T. Structure-function analysis of Arabidopsis thaliana histidine kinase AHK5 bound to its cognate phosphotransfer protein AHP1. Mol Plant. 2013;6(3):959–70. pmid:23132142.

52. Srivastava SK, Rajasree K, Fasim A, Arakere G, Gopal B. Influence of the AgrC-AgrA complex on the response time of Staphylococcus aureus quorum sensing. J Bacteriol. 2014;196(15):2876–88. pmid:24858185; PubMed Central PMCID: PMCPMC4135676.

53. Hornschemeyer P, Liss V, Heermann R, Jung K, Hunke S. Interaction Analysis of a Two-Component System Using Nanodiscs. PLoS One. 2016;11(2):e0149187. pmid:26882435; PubMed Central PMCID: PMCPMC4755656.

54. Arthur M, Depardieu F, Gerbaud G, Galimand M, Leclercq R, Courvalin P. The VanS sensor negatively controls VanR-mediated transcriptional activation of glycopeptide resistance genes of Tn1546 and related elements in the absence of induction. J Bacteriol. 1997;179(1):97–106. Epub 1997/01/01. pmid:8981985; PubMed Central PMCID: PMC178666.

55. Grissom-Arnold J, Alborn WE Jr., Nicas TI, Jaskunas SR. Induction of VanA vancomycin resistance genes in Enterococcus faecalis: use of a promoter fusion to evaluate glycopeptide and nonglycopeptide induction signals. Microb Drug Resist. 1997;3(1):53–64. pmid:9109096.

56. Baptista M, Depardieu F, Reynolds P, Courvalin P, Arthur M. Mutations leading to increased levels of resistance to glycopeptide antibiotics in VanB-type enterococci. Mol Microbiol. 1997;25(1):93–105. Epub 1997/07/01. pmid:11902729.

57. Baptista M, Rodrigues P, Depardieu F, Courvalin P, Arthur M. Single-cell analysis of glycopeptide resistance gene expression in teicoplanin-resistant mutants of a VanB-type Enterococcus faecalis. Mol Microbiol. 1999;32(1):17–28. Epub 1999/04/27. pmid:10216856.

58. Depardieu F, Foucault ML, Bell J, Dubouix A, Guibert M, Lavigne JP, et al. New combinations of mutations in VanD-Type vancomycin-resistant Enterococcus faecium, Enterococcus faecalis, and Enterococcus avium strains. Antimicrob Agents Chemother. 2009;53(5):1952–63. Epub 2009/03/05. pmid:19258279; PubMed Central PMCID: PMCPMC2681503.

59. Willett JW, Kirby JR. Genetic and biochemical dissection of a HisKA domain identifies residues required exclusively for kinase and phosphatase activities. PLoS genetics. 2012;8(11):e1003084. pmid:23226719; PubMed Central PMCID: PMCPMC3510030.

60. Huynh TN, Stewart V. Negative control in two-component signal transduction by transmitter phosphatase activity. Mol Microbiol. 2011;82(2):275–86. Epub 2011/09/08. pmid:21895797; PubMed Central PMCID: PMCPMC3192241.

61. Pocanschi CL, Dahmane T, Gohon Y, Rappaport F, Apell HJ, Kleinschmidt JH, et al. Amphipathic polymers: tools to fold integral membrane proteins to their active form. Biochemistry. 2006;45(47):13954–61. Epub 2006/11/23. pmid:17115690.

62. Tribet C, Audebert R, Popot JL. Amphipols: polymers that keep membrane proteins soluble in aqueous solutions. Proc Natl Acad Sci U S A. 1996;93(26):15047–50. Epub 1996/12/24. pmid:8986761; PubMed Central PMCID: PMCPMC26353.

63. Phillips-Jones MK, Harding SE. Antimicrobial resistance (AMR) nanomachines-mechanisms for fluoroquinolone and glycopeptide recognition, efflux and/or deactivation. Biophys Rev. 2018;10(2):347–62. Epub 2018/03/12. pmid:29525835; PubMed Central PMCID: PMCPMC5899746.