We took advantage of the vancomycin-dependent phenotype of Streptomyces coelicolor femX null mutants to isolate a collection of spontaneous, drug-independent femX suppressor mutants that expressed the vancomycin-resistance (van) genes constitutively. All of the suppressor mutations were in vanS but, unexpectedly, many were predicted to be loss-of-function mutations. Confirming this interpretation, a constructed vanS deletion mutation also resulted in constitutive expression of the van genes, suggesting that VanS negatively regulated VanR function in the absence of drug. In contrast, a vanS pta ackA triple mutant, which should not be able synthesize acetyl phosphate, failed to express the van genes, whereas a pta ackA double mutant showed wild-type, regulated induction of the van genes. These results suggest that in the absence of vancomycin, acetyl phosphate phosphorylates VanR, and VanS acts as a phosphatase to suppress the levels of VanR∼P. On exposure to vancomycin, VanS activity switches from a phosphatase to a kinase and vancomycin resistance is induced. In S. coelicolor, the van genes are induced by both vancomycin and the glycopeptide A47934, whereas in Streptomyces toyocaensis (the A47934 producer) resistance is induced by A47934 but not by vancomycin. We exploited this distinction to replace the S. coelicolor vanRS genes with the vanRS genes from S. toyocaensis. The resulting strain acquired the inducer profile of S. toyocaensis, providing circumstantial evidence that the VanS effector ligand is the drug itself, and not an intermediate in cell wall biosynthesis that accumulates as result of drug action. Consistent with this suggestion, we found that non-glycopeptide inhibitors of the late steps in cell wall biosynthesis such as moenomycin A, bacitracin and ramoplanin were not inducers of the S. coelicolor VanRS system, in contrast to results obtained in enterococcal VanRS systems.
Vancomycin is clinically important for treating enterococcal infections arising after abdominal surgery and is vital as the only widely effective treatment for infections caused by methicillin-resistant Staphylococcus aureus (MRSA), a major killer in hospital-acquired infections. Vancomycin and other glycopeptide antibiotics inhibit cell wall biosynthesis by binding to the d-alanyl-d-alanine (d-Ala-d-Ala) terminus of lipid-attached peptidoglycan precursors on the outside of the cytoplasmic membrane (Williams et al., 1983; Barna and Williams, 1984). This interaction blocks formation of mature peptidoglycan, principally by denying transpeptidase access to its substrate, thereby preventing formation of the peptide crosslinks between polysaccharide strands that give the cell wall its rigidity. The first clinical isolates of vancomycin-resistant strains of pathogenic Enterococcus faecalis and Enterococcus faecium (VRE) appeared in the late 1980s, and were shown to reprogramme cell wall biosynthesis such that the stem pentapeptide of peptidoglycan precursors terminated in d-alanyl-d-lactate (d-Ala-d-Lac), rather than in d-Ala-d-Ala (Bugg et al., 1991; Walsh et al., 1996; Healy et al., 2000; Pootoolal et al., 2002a). The affinity of vancomycin for precursors terminating in d-Ala-d-Lac is ∼1000-fold lower than for precursors terminating d-Ala-d-Ala (Bugg et al., 1991), rendering the modified bacteria resistant. This remodelling of cell wall precursors requires three enzymes: VanH, which converts pyruvate into d-lactate; VanA, a d-Ala-d-Lac ligase; and VanX, a d-Ala-d-Ala dipeptidase that cleaves any residual circulating d-Ala-d-Ala dipeptide, ensuring that peptidoglycan precursors terminate uniformly in d-Ala-d-Lac. Because vancomycin is the front-line therapy for treating problematic infections caused by MRSA, the spread of vancomycin resistance through bacterial populations is an acute public health issue, highlighted by the recent emergence of vancomycin-resistant, methicillin-resistant Staphylococcus aureus (VRSA) in hospitals (Pearson, 2002; Chang et al., 2003; Weigel et al., 2003; Tenover et al., 2004).
We previously showed that the non-pathogen, Streptomyces coelicolor, carries a gene cluster conferring inducible, high-level resistance to vancomycin (Hong et al., 2004). S. coelicolor is the model species of a genus of Gram-positive, mycelial soil bacteria responsible for production of two-thirds of the commercially important antibiotics. S. coelicolor itself does not make a glycopeptide, but all of the known glycopeptide antibiotics are produced by actinomycetes, the bacterial order to which the streptomycetes belong. As most non-pathogenic actinomycetes live in the soil, it seems likely that S. coelicolor encounters glycopeptide producers and that the van gene cluster therefore confers a selective advantage. The S. coelicolor resistance genes are clearly associated with a laterally acquired DNA element (H.-J. Hong, unpublished); it therefore seems likely that S. coelicolor ultimately acquired the van genes from an actinomycete glycopeptide producer, which must carry these genes to avoid auto-toxicity.
The S. coelicolor cluster consists of seven genes, vanSRJKHAX, divided into four transcription units: vanRS, vanJ, vanK and vanHAX(Fig. 1; Hong et al., 2004). The VanRS two-component signal transduction system, the principal focus of the work reported here, activates transcription from the four van promoters in response to extracellular vancomycin. VanJ is a membrane protein of unknown function, and VanHAX, which are orthologous to the VRE enzymes, alter the cell wall precursors to terminate d-Ala-d-Lac (Hong et al., 2004; 2005).
vanK is a particularly interesting gene because it is essential for vancomycin resistance in S. coelicolor, despite the fact that it has no orthologues in the vancomycin-resistance gene clusters of pathogenic enterococci (Hong et al., 2004). VanK is a member of the Fem family of enzymes, which add the branch amino acid(s) to the stem pentapeptide of PG precursors. In S. coelicolor, the branch is a single glycine residue and, in the absence of vancomycin, this glycine is added by an enzyme called FemX (Hong et al., 2005). However, the constitutive FemX activity of S. coelicolor can recognize only precursors that terminate in d-Ala-d-Ala as a substrate, and VanK is therefore required for vancomycin resistance because it is the only enzyme that can add the Gly branch to precursors terminating in d-Ala-d-Lac (production of precursors lacking the Gly branch is lethal in Streptomyces because it prevents cross-linking of the peptidoglycan by transpeptidase, leading to cell lysis) (Hong et al., 2005).
femX is essential under normal growth conditions (Hong et al., 2005). However, because VanK replaces the function of FemX during vancomycin-induced cell wall precursor remodelling, femX null mutants are viable in the presence of vancomycin, but die in its absence, when VanK is not expressed (Hong et al., 2005). We took advantage of this drug-dependent phenotype to isolate a collection of spontaneous, drug-independent femX suppressor mutants that expressed the vancomycin-resistance genes constitutively, all of which mapped to the vanS sensor kinase gene. Here we report the resulting genetic and biochemical dissection of the VanRS two-component signal transduction system.
Suppressors of femX map to vanS
When the vancomycin-dependent femX null mutant strain of S. coelicolor was plated for confluent lawns on medium lacking vancomycin, it gave rise to spontaneous suppressor mutants that grew in the absence of the antibiotic (Fig. 2). Using S1 nuclease protection analysis we found that, in two suppressor mutants chosen at random, the vanH promoter was transcribed in the absence of vancomycin, and that transcription was not induced to higher levels by addition of the drug, contrasting with the inducible transcription of the van genes seen in the wild type (Fig. 3). Based on a classical model of two-component systems (Hakenbeck and Stock, 1996), we expected these suppressor mutants to carry gain-of-function mutations in either vanR or vanS, causing constitutive activity of the signal transduction system. Accordingly, we isolated 23 independent spontaneous suppressor mutants and from each sequenced the vanRS operon plus 100 bp of flanking DNA on either side. In every case, the vanR sequence was wild type but a mutation was found in vanS(Table 1). Significantly, most of the sequenced changes were not compatible with gain-of-function mutations. For example, two suppressors (J3135 and J3137) had IS element insertions in vanS, and many contained frame-shift alleles that could not conceivably give rise to a functional VanS protein (Table 1).
Table 1. femX suppressor mutations.
Single base pair deletion in codon 92
Insertion element (SCO0022) between codons 266 and 267
Six base pair insertion in codon 197
Insertion element IS466A (SCO3490) between codons 302 and 303
P91L (in HAMP linker domain)
A18V (in first transmembrane domain)
L191P (in H-box domain)
Single base pair insertion in codon 256
Single base pair deletion in codon 25
Single base pair insertion in codon 315
Single base pair insertion in codon 92
L216P (in ATPase domain)
G271V (in ATPase domain)
Single base pair insertion in codon 272
Six base pair insertion in codon 340 (identical to J3197)
Single base pair insertion in codon 92
Single base pair insertion in codon 2
Single base pair insertion in codon 2 and single base pair deletion in codon 92
A124T (in HAMP linker domain)
Single base pair insertion between codon 8 and codon 9
G322V (in ATPase domain)
Six base pair insertion in codon 340 (identical to J3189)
Single base pair insertion in codon 91
The van genes are transcribed constitutively in a vanS null mutant
Sequence analysis suggested that most (and therefore conceivably all) of the 23 characterized spontaneous femX suppressor mutations in vanS were loss-of-function mutations. To confirm and extend this interpretation, we constructed vanS and vanRS deletion mutants. While the vanRS mutant failed to grow on 10 µg ml−1 vancomycin, the minimum inhibitory concentration (MIC) for the vanS mutant was 160 µg ml−1 (Figs 2 and 3). Furthermore, in the vanS null mutant the vanH promoter was transcribed in the absence of vancomycin and transcription was not induced to higher levels by addition of the drug (Fig. 3). Thus, while in the wild-type expression of the van genes is inducible, it is constitutive in the vanS null mutant. The level of constitutive van gene transcription was higher in the two ΔfemX suppressor strains examined than in the ΔvanS mutant (Fig. 3); the molecular basis of this observation is currently unclear.
A vanR D51A allele is inactive
As an explanation for the constitutive expression of the van genes in a vanS null mutant, we first considered the possibility that unphosphorylated VanR might be the active form of the protein. To test this hypothesis, aspartate 51, the predicted site of phosphorylation in VanR, was changed to alanine. The D51A and wild-type vanR alleles were used to generate two otherwise identical constructs, based on the integrative vector pMS82 (Gregory et al., 2003), and each was introduced into the vanRS double mutant. The vancomycin-sensitive phenotype of the vanRS deletion strain was complemented in trans by wild-type vanR but not by the D51A allele (Fig. 2), suggesting that phosphorylation of D51 is required for van gene activation.
Construction of a vanS pta ackA triple mutant suggests that VanR can be activated by acetyl phosphate in vivo
An alternative explanation for constitutive expression of the van genes in a vanS null mutant would be that VanR∼P can be generated in a VanS-independent manner and that VanS acts as a VanR∼P phosphatase in the absence of vancomycin. VanS-independent synthesis of VanR∼P might arise through crosstalk with one of the other 83 sensor-kinases in S. coelicolor (Hutchings et al., 2004). Alternatively, VanR could be activated by a small molecule phosphodonor such as acetyl phosphate. Acetyl phosphate is routinely used to phosphorylate response regulators in vitro in the absence of their cognate sensor kinases (Hakenbeck and Stock, 1996) and, in Escherichia coli at least, there is genetic evidence that acetyl phosphate can act as a phosphodonor in vivo, for example to the response regulator RssB, the σS regulator (Bouchéet al., 1998). Synthesis and degradation of acetyl phosphate is controlled by acetate kinase (Ack) and phosphotransacetylase (Pta); in E. coli, an ackA mutant overproduces acetyl phosphate, a pta mutant has very low levels of acetyl phosphate, and an ackA pta double mutant cannot produce acetyl phosphate from acetate or acetyl CoA (Pruss and Wolfe, 1994). To see if acetyl phosphate might be responsible for generating VanR∼P in a vanS null mutant, we introduced a further lesion into the vanS null mutant background, removing the pta and ackA genes, which are adjacent to each other in S. coelicolor. In contrast to the vanS mutant that grew readily on vancomycin, the vanS pta ackA triple mutant was vancomycin-sensitive (Fig. 2) and transcription from the vanH promoter was virtually undetectable in the presence or absence of vancomycin (Fig. 3), suggesting that acetyl phosphate can act as a phosphodonor to VanR in vivo.
VanS is both a kinase and phosphatase
The data given above were consistent with VanS acting as a VanR phosphatase in the absence of vancomycin, but they did not show whether exposure to vancomycin converted VanS into an active VanR kinase, or simply turned off its phosphatase activity. We addressed this question genetically and biochemically. First, we constructed a pta ackA double mutant in a vanS+ background and found that this strain was vancomycin resistant (Fig. 2) and that transcription of the van genes was induced in response to vancomycin (Fig. 3), suggesting that VanS can generate VanR∼P in vivo. Second, we overexpressed VanR and the cytosolic domain of VanS (c-VanS, corresponding to residues 85–364) in E. coli and purified them to homogeneity as his-tagged proteins. Incubation of c-VanS with [γ-32P] ATP resulted in autophosphorylation, with maximum phosphorylation occurring after 60 min (Fig. 4A). When radiolabelled c-VanS was mixed with VanR in the presence of ATP, rapid phosphotransfer was observed (Fig. 4B, lane 2), confirming that c-VanS has kinase activity. Purified VanR protein could also be phosphorylated using radiolabelled acetyl phosphate (Fig. 4B, lane 3). Incubation of VanR∼P generated in this way with c-VanS resulted in removal of the phosphate group from VanR, confirming that c-VanS has phosphatase activity. This dephosphorylation is unlikely to involve reverse phosphotransfer to VanS because no radiolabelled c-VanS was detected in this reaction.
The femX mutant provides a novel bioassay for inducers of VanS
In enterococci, the nature of the effector ligand that binds the sensor domain of VanS to activate the signal transduction pathway is controversial. Although glycopeptides activate the enterococcal van genes, several structurally unrelated compounds that inhibit late steps in cell wall biosynthesis, such as moenomycin A, bacitracin and ramoplanin, have also been reported to induce van gene expression (Handwerger and Kolokathis, 1990; Allen and Hobbs, 1995; Baptista et al., 1996; 1999; Lai and Kirsch, 1996; Ulijasz et al., 1996; Grissom-Arnold et al., 1997; Mani et al., 1998). Because these compounds have no structural similarity to each other or to the glycopeptides, the general consensus has been that the VanS effector ligand must be an intermediate in cell wall biosynthesis, such as Lipid II, which accumulates as a result of the action of the inhibition of cell wall biosynthesis, rather than the antibiotic itself.
We previously established a bioassay for inducers of the S. coelicolor VanRS signal transduction system by making a multicopy construct in which the vanJ promoter (vanJp) drove expression of the neo gene, which confers resistance to neomycin and kanamycin (Hong et al., 2004). Using this bioassay, we showed that a variety of glycopeptides induced van gene expression, but that cephalosporins and penicillins did not. However, we did not test moenomycin A, bacitracin or ramoplanin. In constructing the drug-dependent femX null mutant, we created an optimal bioassay for inducers in S. coelicolor. This strain is viable only in the presence of compounds that activate the VanRS signal transduction system, the readout is simple growth, and there are no plasmids or reporter genes involved. We therefore extended our previous analysis of van gene inducer specificity in S. coelicolor using the femX null mutant. Confluent lawns of spores of the femX null mutant (J3130) were spread on MMCGT plates and potential inducers were applied on paper discs to the freshly spread plates. Inducers of the VanRS signal transduction system caused a halo of growth around the disc (Fig. 5). As we had previously found using the vanJp-neo bioassay (Hong et al., 2004), vancomycin, ristocetin, chloroeremomycin and A47934 acted as inducers. Significantly, however, moenomycin A, bacitracin and ramoplanin completely failed to rescue the growth defect of the femX null mutant (Fig. 5), showing that these compounds are not inducers of the VanRS signal transduction system in S. coelicolor.
The origin of the VanRS signal transduction system, not the host, determines inducer specificity
Streptomyces toyocaensis produces the glycopeptide antibiotic A47934, and the sequence of the entire A47934 biosynthetic gene cluster has been determined (Pootoolal et al., 2002b). Associated with the cluster are homologues of the S. coelicolor vanSRJKHAX genes. In S. coelicolor, the van genes are induced by both A47934 and vancomycin (Fig. 5; Hong et al., 2004). In contrast, in S. toyocaensis, resistance is induced by A47934 but not by vancomycin (Neu and Wright, 2001), perhaps implying that the ligands recognized by the VanS proteins from these two Streptomyces species are different. To test this hypothesis, we swapped the signal transduction systems of the two species by introducing the S. toyocaensis vanRS genes (vanRSst) into the S. coelicolor vanRS deletion mutant, using the integrative vector pRT801 (Gregory et al., 2003). Significantly, the resulting strain was resistant to A47934, but sensitive to vancomycin (Fig. 6A). Consistent with this result, vancomycin did not induce transcription from the vanH promoter in this strain, but A47934 did (Fig. 6B). Thus, switching the VanRS signal transduction system from one species to the other also switched inducer specificity.
Taken together, our data suggest the following model for the regulation of the VanRS signal transduction system in S. coelicolor(Fig. 7). In the absence of vancomycin, acetyl phosphate phosphorylates D51 of VanR, and VanS acts as a phosphatase to suppress the levels of VanR∼P. In the presence of vancomycin, VanS is converted from a phosphatase to a kinase, leading to accumulation of VanR∼P and activation of the four promoters of the van gene cluster. Transcription of the vanRS operon is itself under VanRS control (Hong et al., 2004) and so there will be very little VanR or VanS protein in S. coelicolor growing constantly in the absence of vancomycin. Thus, the ‘futile cycle’ of VanR phosphorylation and dephosphorylation shown occurring in the absence of vancomycin in Fig. 7 will occur at a high level only after the organism has been transiently exposed to the antibiotic. The duration of high level futile cycling will therefore depend on the half-lives of VanR and VanS in vivo.
An unresolved question is how much, if at all, acetyl phosphate contributes to VanR phosphorylation when the kinase activity of VanS is turned on in the presence of vancomycin. Certainly an ackA pta vanS+ strain is resistant to vancomycin (Fig. 2) and still shows strong induction of the van genes (Fig. 3). If acetyl phosphate does make a significant contribution and thereby influences the organism's ability to respond to challenge by the antibiotic, then further questions arise: how widely do acetyl phosphate levels fluctuate in S. coelicolor, and what factors influence that fluctuation. It will be interesting to discover how many of the other 79 response-regulators in S. coelicolor can be phosphorylated by acetyl phosphate in vivo (Hutchings et al., 2004).
Similar results have previously been obtained in pathogenic enterococci. Depardieu et al. (2003) identified an E. faecium clinical isolate that expressed vancomycin resistance constitutively and showed that it carried an 18-bp in-frame deletion in vanS that resulted in a VanS protein deficient in phosphatase activity. Arthur et al. (1997) showed that the van promoters of E. faecium were constitutively activated by VanR in the absence of VanS, and concluded that VanS negatively controls VanR in the absence of glycopeptide inducer, presumably by dephosphorylation. Furthermore, Haldimann et al. (1997) demonstrated that heterologous expression of E. faecium VanR in an E. coli ackA strain harbouring a vanH–lacZ fusion stimulated high levels of β-galactosidase production, suggesting that acetyl phosphate could act as a phosphodonor to the E. faecium VanR protein in E. coli in vivo.
Streptomyces coelicolor femX null mutants are viable only in the presence of compounds that activate the VanRS signal transduction system, because they rely on expression of VanK for survival. We took advantage of this discovery to create a simple bioassay for inducers of the van genes in S. coelicolor. The structurally closely related glycopeptide antibiotics vancomycin, ristocetin, chloroeremomycin and A47934 all acted as inducers. However, in contrast to the enteroccocal VanRS systems, moenomycin A, bacitracin and ramoplanin did not act as inducers of the VanRS system in S. coelicolor.
To address the effector ligand issue further, we carried out a ‘VanRS swap’ experiment between two glycopeptide-resistant Streptomyces species with differing spectra of inducer molecules, to see if inducer specificity was determined by VanRS itself or by the host background. In S. coelicolor, the van genes are induced by both A47934 and vancomycin, while in S. toyocaensis, resistance is induced by A47934 but not by vancomycin (Neu and Wright, 2001). Introducing the S. toyocaensis VanRS signal transduction system into an S. coelicolor vanRS null mutant switched inducer specificity to that of S. toyocaensis. Thus, inducer specificity is determined by the origin of VanRS. There are two potential explanations for this observation. If Streptomyces VanS is activated by accumulation of a cell wall intermediate, vancomycin must induce a radically different spectrum of cell wall intermediates in S. coelicolor and S. toyocaensis, which seems unlikely. The more likely alternative is that VanS is directly activated by binding antibiotic (or possibly antibiotic bound to d-Ala-d-Ala-containing cell wall precursors, such as Lipid II), and that S. toyocaensis VanS interacts productively with A47934 but not with vancomycin. This would also be consistent with the fact that structurally unrelated compounds that also inhibit late steps in cell wall biosynthesis, such as moenomycin A, bacitracin and ramoplanin, are not inducers of VanS in Streptomyces.
Whether the VanS effector ligand is a cell wall intermediate or the drug itself, the ability to respond differentially to vancomycin and A47934 must reside in differences between the sensor domains of the S. toyocaensis and S. coelicolor VanS proteins. Alignment of the VanS primary sequences from these two species shows that the proteins are very similar, with 65% identity overall (Fig. 8). It is striking, however, that this high level of identity breaks down in the 26–27-residue stretch between the two predicted transmembrane helices, corresponding to the putative VanS sensor domain (Fig. 8).
Bacterial strains, plasmids, oligonucleotides and growth conditions
Protoplast transformation and conjugal plasmid transfer from E. coli to Streptomyces spp.
To bypass the methyl-specific restriction system of S. coelicolor, cosmids and plasmids were passed through the dam dcm hsdS E. coli strain ET12567 prior to protoplast transformation or conjugation. E. coli ET12567 carrying the non-transmissible, oriT-mobilizing ‘driver’ plasmid pUZ8002 was used for conjugation. Streptomyces protoplast transformation and conjugation from E. coli to Streptomyces were carried out as described by Kieser et al. (2000).
Isolating suppressors of femX
J3130 was streaked on MS agar containing 10 µg ml−1 vancomycin and 23 single colonies were restreaked on MS agar without vancomycin. A single femX suppressor was then isolated from each of these plates to ensure the mutants were not clonal. Genomic DNA was isolated from each suppressor strain as described (Kieser et al., 2000) and the vanRS genes, including 100 bp flanking DNA on either side, were amplified by polymerase chain reaction (PCR) using the primers vanRFLANKI plus vanRFLANKII, and vanSFLANKI plus vanSFLANKII (Table 2) and sequenced using the same primers.
Construction of insertion and deletion mutants
ΔvanS::apr (J3199), ΔvanRS::apr (J2175) and Δ(pta ackA)::apr (J3202) insertion mutants were constructed by replacing most or all of the entire coding sequence with a cassette carrying the apramycin resistance gene (apr) and oriT of RK2, using the PCR-targeting method of Gust et al. (2003). The appropriate cosmid (H66 or IF6) was introduced into E. coli BW25113 carrying pIJ790, and the target gene was disrupted by electroporation of the cells with the PCR-amplified apr-oriT cassette, generated using primers carrying the appropriate gene-specific extensions (Table 2). The resulting cosmids [H66ΔvanS::apr, H66ΔvanRS::apr and IF6Δ(pta ackA)::apr] were introduced into E. coli ET12567 carrying pUZ8002 and transferred into S. coelicolor M600 by conjugation. Apramycin-resistant (AprR), kanamycin-sensitive (KanS) exconjugants were identified and purified, and the disruptions were confirmed by PCR and Southern analysis. Unmarked ΔvanS (J3200) and ΔvanRS (J3201) deletion mutants were also constructed; cosmids H66ΔvanS::apr and H66ΔvanRS::apr were individually introduced into E. coli BT340 and deletion of the apr-oriT cassette (which is flanked by FRT sites) was obtained after induction of the FLP recombinase (Gust et al., 2003). The mutant cosmids thus obtained, H66ΔvanS and H66ΔvanRS, were introduced into J3199 and J2175, respectively, by protoplast transformation, and KanR transformants were selected. After growth in the absence of antibiotic selection, colonies that had lost both apramycin and kanamycin resistance were selected and purified (J3200 and J3201; Table 2) and analysed by PCR to confirm replacement of apr-oriT cassette by the non-polar ‘scar’ sequence (Gust et al., 2003). J3203 [Δ(pta ackA)::aprΔvanS] was constructed by introducing the Δ(pta ackA)::apr allele into the unmarked ΔvanS mutant, J3200, using the method described above.
Construction of a D51A allele of vanR and complementation of a vanR null mutant
A D51A allele of vanR was created using a pair of complementary primers containing the point mutation (D51A1 and D51A2; Table 2) and two flanking primers from the 5′-and 3′ regions of vanR (vanRFLANKI and vanRFLANKII; Table 2). Briefly, two PCR reactions were set up using vanRFLANKI plus D51A2 and vanRFLANKII plus D51A1. The two PCR products were gel purified, mixed, and used as template for a third PCR reaction containing only the flanking primers, and the resulting full-length PCR product was gel purified. The wild-type vanR allele was amplified from M600 genomic DNA using only vanRFLANKI and vanRFLANKII. The PCR products were cloned into SmaI-cut pUC19, sequenced and subcloned into HindIII-KpnI-cut pMS82 (Gregory et al., 2003) to create pIJ6959 (D51A) and pIJ6961 (wild-type), which were introduced into the vanRS mutant J2175 by conjugal transfer from E. coli strain ET12567 (pUZ8002), selecting exconjugants with hygromycin.
Overexpression of VanS and VanR
Full-length vanR was amplified using primers vanRFOR and vanRREV, and the cytosolic domain of VanS (c-VanS, corresponding to codons 85–364) was amplified using primers vanSFOR and vanSREV. The forward primers contained NdeI sites in frame with the translation start codon. The PCR products were cloned into SmaI-cut pUC19, sequenced and subcloned into NdeI-HindIII-cut pET15b (Stratagene). The His-tagged proteins were overexpressed in BL21λDE3 (2 l) by induction with 0.1 mM IPTG at OD600 = 0.6 at 37°C for 3 h.
Purification of VanR
Cells were resuspended in 38 ml of binding buffer (50 mM Tris-HCl, pH 7.5, 150 mM NaCl, 5 mM imidazole), passed twice through a French Press, and the lysate was clarified by centrifugation. The supernatant and pellet both contained VanR, but only the soluble protein was further purified. The supernatant was filtered through a 0.2 µm filter (Millipore) and applied to a 5 ml HiTrap Chelating Ni2+ column. The column was washed with binding buffer until the UV trace was stable, and VanR was eluted with a linear 5–500 mM imidazole gradient (30 ml). Fractions containing VanR were stored at 4°C in elution buffer.
Purification of c-VanS
Cells were resuspended in 35 ml of 20 mM Tris-HCl (pH 8.0), passed twice through a French Press, and the lysate was clarified by centrifugation. c-VanS was found only in the pellet, which was washed with distilled water and solubilized in sarkosyl buffer [50 mM Tris-HCl, pH 7.5, 250 mM NaCl, 0.2% (w/v) sarkosyl (N-lauroylsarcosine)]. After solubilization overnight at 4°C, the solution was clarified by centrifugation and filtered through a 0.2-µm filter, and c-VanS was purified by nickel affinity chromatography as described for VanR. Fractions containing c-VanS were stored at 4°C in elution buffer.
In vitro phosphorylation assays
Immediately before use, purified VanR protein (0.5 ml) was applied to a Millipore Ultrafree-0.5 centrifugal filter device and centrifuged for 10 min at 10 000 r.p.m. in an Eppendorf 5415 D microcentrifuge for 10 min. The concentrated protein was diluted back to 0.6 ml with 50 mM Tris-HCl, pH 8.0, 250 mM NaCl, and this was repeated three times. For the autophosphorylation reaction, VanS (40 pmol) was incubated with 10 µCi [γ32P] ATP at room temperature for 1 h in 50 mM HEPES, pH 7.2, 5 mM MgCl2 (50 µl total volume) and samples were taken at 0.5, 1, 2, 5, 15, 30 and 60 min and quenched immediately by addition of an equal volume of SDS-PAGE loading dye. For the phosphotransfer reaction, 40 pmol VanS was incubated for 60 min with 10 µCi [γ32P] ATP and then mixed with VanR protein (20 pmol) at room temperature (50 µl total volume). Samples were taken at 1, 5, 15 and 30 min and quenched by addition of SDS-PAGE loading dye. [32P] acetyl phosphate was prepared as described previously (Molle and Buttner, 2000) and incubated with VanR (20 pmol) at room temperature for 15 min (5 µl total volume). Reactions were quenched by addition of an equal volume of SDS-PAGE loading dye. All samples were loaded onto 15% SDS-polyacrylamide gels and separated at 200 V for 60 min at room temperature. Gels were dried and exposed to X-ray film overnight.
Complementation of the S. coelicolor vanRS null mutant with S. toyocaensis vanRS (vanRSst)
A 3 kb SacI fragment carrying the S. toyocaensis vanRS operon was made blunt-ended using DNA PolI and was cloned into the conjugative vector pRT801 cut with PvuII. The resulting plasmid, pIJ10277, was introduced into the S. coelicolor vanRS null mutant J3201 by conjugal transfer from E. coli strain ET12567/pUZ8002, and exconjugants were selected with apramycin.
RNA preparation and S1 nuclease protection assays
RNA was prepared as described previously (Hong et al., 2002; 2004). Germinated spores of S. coelicolor strains were inoculated into NMMP (Kieser et al., 2000) and grown to an OD450 of 0.3–0.6 at 30°C. Immediately after the first 10 ml sample was taken, inducer (10 µg ml−1 vancomycin or 10 µg ml−1 A47934) was added to the remaining 40 ml of culture broth and 10 ml samples were taken at subsequent 30 min intervals up to 90 min. The vanH probe was a 270 bp 5′ end-labelled fragment generated by PCR using primers vanH S1 FOR and vanH S1 REV (Table 2) and S. coelicolor M600 chromosomal DNA as a template. For all assays, 30 µg RNA and 25 pmol labelled probe were dissolved in 20 µl of NaTCA buffer and hybridized at 45°C overnight after denaturation at 65°C for 15 min.
We thank Nancy Sheeler, Alan Wolfe, David Hopwood, Ray Dixon, Mark Paget and Gerry Wright for helpful discussions and comments on the manuscript, and Xiao Dong Wang and Gerry Wright for the gift of A47934 and the S. toyocaensis vanRS clone. This work was funded by BBSRC Grants 208/P20040 (to H.-J.H. and M.J.B.) and 208/P14575 (to M.J.B.) and by a grant-in-aid to the John Innes Centre from the BBSRC.