Molecular characterization of the PhoPQ-PmrD-PmrAB mediated pathway regulating polymyxin B resistance in Klebsiella pneumoniae CG43
© Cheng et al; licensee BioMed Central Ltd. 2010
Received: 16 April 2010
Accepted: 24 July 2010
Published: 24 July 2010
The cationic peptide antibiotic polymyxin has recently been reevaluated in the treatment of severe infections caused by gram negative bacteria.
In this study, the genetic determinants for capsular polysaccharide level and lipopolysaccharide modification involved in polymyxin B resistance of the opportunistic pathogen Klebsiella pneumoniae were characterized. The expressional control of the genes responsible for the resistance was assessed by a LacZ reporter system. The PmrD connector-mediated regulation for the expression of pmr genes involved in polymyxin B resistance was also demonstrated by DNA EMSA, two-hybrid analysis and in vitro phosphor-transfer assay.
Deletion of the rcsB, which encoded an activator for the production of capsular polysaccharide, had a minor effect on K. pneumoniae resistance to polymyxin B. On the other hand, deletion of ugd or pmrF gene resulted in a drastic reduction of the resistance. The polymyxin B resistance was shown to be regulated by the two-component response regulators PhoP and PmrA at low magnesium and high iron, respectively. Similar to the control identified in Salmonella, expression of pmrD in K. pneumoniae was dependent on PhoP, the activated PmrD would then bind to PmrA to prolong the phosphorylation state of the PmrA, and eventually turn on the expression of pmr for the resistance to polymyxin B.
The study reports a role of the capsular polysaccharide level and the pmr genes for K. pneumoniae resistance to polymyxin B. The PmrD connector-mediated pathway in governing the regulation of pmr expression was demonstrated. In comparison to the pmr regulation in Salmonella, PhoP in K. pneumoniae plays a major regulatory role in polymyxin B resistance.
Klebsiella pneumoniae, an important nosocomial pathogen, causes a wide range of infections including pneumonia, bacteremia, urinary tract infection, and sometimes even life-threatening septic shock . The emergence of multi-drug resistant K. pneumoniae has reduced the efficacy of antibiotic treatments and prompted the reevaluation of previously but not currently applied antibiotics [2, 3] or a combined therapy . Polymyxins, originally isolated from Bacillus polymyxa, have emerged as promising candidates for the treatment of infections . As a member of antimicrobial peptides (APs), the bactericidal agent exerts its effects by interacting with the lipopolysaccharide (LPS) of gram-negative bacteria. The polycationic peptide ring on polymyxin competes for and substitutes the calcium and magnesium bridges that stabilize LPS, thus disrupting the integrity of the outer membrane leading to cell death [5, 6].
The Klebsiella capsular polysaccharide (CPS), which enabled the organism to escape from complement-mediated serum killing and phagocytosis [7, 8], has been shown to physically hinder the binding of C3 complement  or polymyxin B . The assembly and transport of Klebsiella CPS followed the E. coli Wzy-dependent pathway , in which mutations at wza encoding the translocon protein forming the complex responsible for CPS polymer translocation and export resulted in an inability to assemble a capsular layer on the cell surface . The CPS biosynthesis in K. pneumoniae was transcriptionally regulated by the two-component system (2CS) RcsBCD  where the deletion of the response regulator encoding gene rcsB in K. pneumoniae caused a loss of mucoid phenotype and reduction in CPS production .
In Escherichia coli and Salmonella enterica serovar Typhimurium, polymyxin B resistance is achieved mainly through the expression of LPS modification enzymes, including PmrC, an aminotransferase for the decoration of the LPS with phosphoethanolamine  and the pmrHFIJKLM operon [16, 17] (also called pbgP or arn operon [18, 19]) encoding enzymes. Mutations at pmrF, which encoded a transferase for the addition of 4-aminoarabinose on bactoprenol phosphate, rendered S. enterica and Yersinia pseudotuberculosis more susceptible to polymyxin B [16, 20]. The S. enterica ugd gene encodes an enzyme responsible for the supply of the amino sugar precursor L-aminoarabinose for LPS modifications and hence the Ugd activity is essential for the resistance to polymyxin B . On the other hand, the E. coli ugd mutant with an impaired capsule also became highly susceptible to polymyxin B .
The 2CS PmrA/PmrB, consisting of the response regulator PmrA and its cognate sensor kinase PmrB, has been identified as a major regulatory system in polymyxin B resistance [23, 24]. The resistance in S. enterica or E. coli has been shown to be inducible by the extracellular iron . In addition to acidic pH , the role of ferric ions as a triggering signal for the expression of PmrA/PmrB has been demonstrated . The 2CS PhoP/PhoQ which regulates the magnesium regulon  could also activate polymyxin B resistance under low magnesium in S. enterica, in which the PhoP/PhoPQ-dependent control is connected by the small basic protein PmrD. The expression of pmrD could be activated by PhoP while repressed by PmrA forming a feedback loop [28, 29]. The activated PmrD could then bind to the phosphorylated PmrA leading to a persistent expression of the PmrA-activated genes .
The PmrD encoding gene was also identified in E. coli and K. pneumoniae. However, pmrD deletion in E. coli had no effect on the bacterial susceptibility to polymyxin B . Recently, the PhoP-dependent expression of pmrD has also been demonstrated in K. pneumoniae. According to the predicted semi-conserved PhoP box in the pmrD upstream region, a direct binding of PhoP to the pmrD promoter for the regulation was speculated .
In this study, specific deletions of genetic loci involved in CPS biosynthesis and LPS modifications were introduced into K. pneumoniae CG43, a highly virulent clinical isolate of K2 serotype . Involvement of the genetic determinants in polymyxin B resistance was investigated.
Plasmids, bacterial strains, and growth conditions
Bacterial strains and plasmids used in this study
Strain or plasmid
Reference or source
CG43S3ΔlacZ ΔphoP Smr
CG43S3ΔlacZ ΔpmrD Smr
CG43S3ΔlacZ ΔpmrA Smr
CG43S3ΔpmrA ΔphoP Smr
CG43S3ΔpmrA ΔrcsB Smr
CG43S3ΔpmrD ΔrcsB Smr
CG43S3ΔphoP ΔrcsB Smr
hsdR recA pro RP4-2 (Tc::Mu; Km::Tn7)(λpir)
XL1-Blue MRF' Kan
Δ(mcrA)183 Δ(mcrCB-hsdSMR-mrr)173 endA1 supE44 thi-1 recA1 gyrA96 relA1 lac [F' proAB lacIqZ ΔM15 Tn5 (Kanr)]
F- ompT hsdS B (r B - m B - ) gal dcm trxB 15::kan (DE3)
T/A-type PCR cloning vector, Apr
His-tagged protein expression vector, Kmr
Bait plasmid, p15A origin of replication, lac-UV5 promoter, λ-cI open reading frame, Cmr
Target plasmid, ColE1 origin of replication, lac-UV5 promoter, RNAP αopen reading frame, Tcr,
Control plasmid containing a fragment encoding the yeast transcriptional activator Gal4 fused with λ-cI, Cmr
Control plasmid containing a fragment encoding a mutant form of Gal11 protein, called Gal11P, fused with RNAPα, Tcr
Suicide vector, rpsL, Apr, Kmr
Shuttle vector, mob+, Tcr
promoter selection vector, lacZ+, Cmr
1.3-kb fragment containing a pmrF allele cloned into pRK415, Tcr
1.2-kb fragment containing the entire rcsB locus cloned into pRK415, Tcr
1.1-kb fragment containing a pmrA allele cloned into pRK415, Tcr
900-bp fragment containing a phoP allele cloned into pRK415, Tcr
550-bp fragment containing a pmrD allele cloned into pRK415, Tcr
500-bp fragment containing the upstream region of the K. pneumoniae pbgP genes cloned into placZ15, Cmr
350-bp fragment containing the upstream region of the K. pneumoniae pmrD genes cloned into placZ15, Cmr
711-bp fragment encoding full-length PhoP cloned into pET30b, Kmr
447-bp fragment encoding residues 1-149 of PhoP cloned into pET30b, Kmr
828-bp fragment encoding residues 90-365 of PmrB cloned into pET30b, Kmr
669-bp fragment encoding full-length PmrA cloned into pET29b, Kmr
243-bp fragment encoding full-length PmrD cloned into pET29b, Kmr
669-bp fragment encoding full-length RcsB cloned into pBT, Cmr
243-bp fragment encoding full-length RcsA cloned into pTRG, Tcr
Oligonucleotide primers used in this study
-161 relative to the pmrF start codon
+1116 relative to the pmrF start codon
+682 relative to the pmrA start codon
-424 relative to the pmrA start codon
-171 relative to the phoP start codon
+729 relative to the phoP start codon
+250 relative to the pmrD start codon
-278 relative to the pmrD start codon
+75 relative to the pmrD start codon
-425 relative to the pmrH start codon
+34 relative to the pmrH start codon
+753 relative to the phoP start codon
-25 relative to the phoP start codon
+283 relative to the pmrB start codon
+1095 relative to the pmrB start codon
+1 relative to the pmrA start codon
+672 relative to the pmrA start codon
+1 relative to the pmrD start codon
+243 relative to the pmrD start codon
+1 relative to the pmrA start codon
+672 relative to the pmrA start codon
+1 relative to the pmrD start codon
+243 relative to the pmrD start codon
Construction of specific gene-deletion mutants
Specific gene deletion was individually introduced into the chromosome of K. pneumoniae CG43S3 by allelic exchange strategy . In brief, two approximately 1000-bp DNA fragments flanking both sides of the deleted region were cloned into the suicide vector pKAS46 . The resulting plasmid was then mobilized from E. coli S17-1 λpir to K. pneumoniae CG43S3, K. pneumoniae CG43S3ΔlacZ, or K. pneumoniae CG43S3ΔrcsB, by conjugation. The transconjugants were selected with ampicillin and kanamycin on M9 agar plates. Colonies were grown overnight in LB broth at 37°C and then spread onto an LB agar plate containing 500 μg/ml of streptomycin. The streptomycin-resistant and kanamycin-sensitive colonies were selected, and the deletion was verified by PCR and Southern analysis using gene-specific probe. The resulting K. pneumoniae mutants are listed Table 1.
To obtain the complementation plasmids, DNA fragments containing the coding sequence of pmrA, phoP, pmrF, or pmrD were PCR-amplified with primer sets pmrAp03/pmrA06, phoP01/phoP02, ppmrF01/ppmrF02 or pmrDp01/pmrDe02 (Table 2) and cloned into the shuttle vector pRK415  to generate pRK415-PmrA, pRK415-PhoP, pRK415-PmrF and pRK415-PmrD (Table 1), respectively.
Extraction and quantification of CPS
Bacterial CPS was extracted using the method described . Briefly, 500 μl of overnight culture was mixed with 100 μl of 1% Zwittergent 3-14 (Sigma-Aldrich) in 100 mM citric acid (pH 2.0) and incubated at 50°C for 20 min. After centrifugation, 250 μl of the supernatant was used to precipitate CPS with 1 ml of absolute ethanol. The pellet was dissolved in 200 μl distilled water, and then 1,200 μl of 12.5 mM borax in H2SO4 was added. The mixture was vigorously mixed, boiled for 5 min, cooled, and then 20 μl 0.15% 3-hydroxydiphenol (Sigma-Aldrich) was added. OD520 was measured and the uronic acid content was determined from a standard curve of glucuronic acid and expressed as μg per 109 CFU.
Polymyxin B resistance assay
Cell line, cell culture and phagocytosis assay
The mouse macrophage cell line RAW264.7 was cultivated in Dulbecco's Modified Eagle Medium (DMEM) (Gibco) supplemented with 10% fetal bovine serum (Gibco), 100 units/ml of penicillin and 100 μg/ml of streptomycin (Gibco) at 37°C under 5% CO2. The evaluation of bacterial phagocytosis was carried out as described with some modifications . In brief, cells were washed, resuspended in DMEM containing 10% FBS, and approximately 106 cells per well were seeded in a 24 well tissue culture plate and incubated at 37°C for 16 h. Then 100 μl of the bacterial suspension (approximately 3 × 108 CFU/ml in PBS) was used to infect each well to obtain a ratio of ca. 30 bacteria per macrophage. After incubation for 2 h, the cells were washed thrice, then 1 ml of DMEM containing 100 μg/ml of gentamycin was added and incubated for another 2 h to kill the extracellular bacteria. Cells were washed thrice, 1 ml of 0.1% Triton X-100 was added and incubated at room temperature for 10 min with gentle shaking to disrupt the cell membrane. The cell lysate was diluted serially with PBS, plated onto LB agar plates and incubated overnight for determining viable bacteria count. The relative survival rates after phagocytosis were expressed as the colony counts of viable bacteria divided by those of the original inoculums and multiplied by 100. Three independent trials were performed, and the data shown were the average ± standard deviation from five replicas.
Construction of reporter fusion plasmid and measurement of promoter activity
The approximately 350 or 500-bp DNA fragments containing the upstream region of the K. pneumoniae pmrD or pmrHFIJKLM gene cluster were PCR-amplified with primers pmrDp01/pmrDp02 or pmrHp01/pmrHp02 (Table 2), respectively and cloned in front of a promoter-less lacZ gene of the promoter selection plasmid placZ15 . The resulting plasmids, placZ15-PpmrD and placZ15-PpmrH were mobilized from E. coli S17-1 λpir to K. pneumoniae strains by conjugation. β-galactosidase activity was determined as previously described . In brief, overnight cultures were washed twice with saline and subcultured in LB alone or supplemented with 10 mM MgCl2, 0.1 mM FeCl3, or 0.1 mM FeCl3 plus 0.3 mM ferric iron scavenger deferoxamine (Sigma-Aldrich) to mid-log phase (OD600 of 0.7). Then 100 μl of the culture was mixed with 900 μl of Z buffer (60 mM Na2HPO4, 40 mM NaH2PO4, 10 mM KCl, 1 mM MgSO4, 50 mM β-mercaptoethanol), 17 μl of 0.1% SDS, and 35 μl of chloroform and the mixture was shaken vigorously. After incubation at 30°C for 10 min, 200 μl of 4 mg/ml ONPG (o-nitrophenyl-β-D-galactopyranoside) (Sigma-Aldrich) was added. Upon the appearance of yellow color, the reaction was stopped by adding 500 μl 1 M Na2CO3. OD420 was recorded and the β-galactosidase activity was expressed as Miller units . Each sample was assayed in triplicate, and at least three independent experiments were carried out. The data shown were calculated from one representative experiment and shown as the means and standard deviation from triplicate samples.
Cloning, expression and purification of recombinant proteins
The DNA fragment of PhoP coding region was PCR amplified from the genomic DNA of K. pneumoniae CG43S3 with primers phoP05/phoP06 (Table 2). The amplified PCR products were cloned into the PCR cloning vector yT&A (Yeastern Biotech, Taiwan). The Eco RI/Bam HI and Sal I fragments from the resulting plasmid were then cloned individually into pET30b (Novagen, Madison, Wis) to generate pET30b-PhoP and pET30b-PhoPN to allow the in-frame fusion to the N-terminal His codons. Plasmid pET30b-PmrBC was constructed by cloning DNA fragments PCR-amplified with pmrBe03/pmrBe04 (Table 2) into a Bam HI/Hin dIII site on pET30b. Plasmids pET-PmrA and pET-PmrD (courtesy of Dr. Chinpan Chen, Academia Sinica, Taipei, Taiwan) were constructed by cloning DNA fragments PCR-amplified with KP1760-1/KP1760-2 and KP3573-1/KP3573-2 (Table 2) into an Nde I/Xho I site, respectively into pET29b. The resulting plasmids were transformed into E. coli BL21(DE3) (Invitrogen, USA), and the recombinant proteins were over-expressed by induction with 0.5 mM isopropyl 1-thio-β-D-galactopyranoside (IPTG) for 3 h at 37°C. The proteins were then purified from total cell lysate by affinity chromatography using His-Bind resin (Novagen, Madison, Wis). After purification, the eluent was dialyzed against 1× protein storage buffer (10 mM Tris-HCl pH 7.5, 138 mM NaCl, 2.7 mM KCl, and 10% glycerol) at 4°C overnight, followed by condensation with PEG20000, and the purity was determined by SDS-PAGE analysis.
DNA electrophoretic mobility shift assay (EMSA)
EMSA was performed as previously described . In brief, the DNA fragment encompassing the putative pmrD promoter region was obtained by PCR amplification and then end-labeled with [γ-32P]ATP by T4 polynucleotide kinase. The purified His-PhoP or His-PhoPN149 protein was mixed with the DNA probe in a 50-μl reaction mixture containing 20 mM Tris-HCl pH 8.0, 50 mM KCl, 1 mM MgCl2, 1 mM dithiothreitol, and 7.5 mM acetyl phosphate. The mixture was incubated at room temperature for 30 min, mixed with 0.1 volume of DNA loading dye, and then loaded onto a 5% nondenaturing polyacrylamide gel containing 5% glycerol in 0.5× TBE buffer (45 mM Tris-HCl pH 8.0, 45 mM boric acid, 1.0 mM EDTA). After electrophoresis at a constant current of 20 mA at 4°C, the result was detected by autoradiography.
Bacterial two-hybrid assay
The bacterial two-hybrid assay was performed as described previously [20, 30]. The DNA fragments encoding full-length PmrA and PmrD were PCR-amplified with primer pairs pmrA10/pmrA11 and pmrDe15/pmrDe16 (Table 2) respectively, and cloned into the 3' end of genes encoding the α subunit of RNA polymerase (RNAPα) domain on pBT and λ-cI repressor protein domain on pTRG. The resulting RNAPα-PmrA and λ-cI-PmrD encoding plasmids, pBT-PmrA and pTRG-PmrD, were confirmed by DNA sequencing. The positive control plasmids used were pTRG-Gal11P and pBT-LGF2 (Stratagene). The pBT and pTRG derived plasmids were co-transformed into E. coli XL1-Blue MRF' Kan cells and selected on LB agar plates supplemented with 12.5 μg/ml tetracycline, 25 μg/ml chloramphenicol, and 50 μg/ml kanamycin. To investigate the protein-protein interaction in vivo, cells were grown until the OD600 reached 0.3 and then diluted serially (10-1, 10-2, 10-3, and 10-4 order). Two-microliters of the bacterial culture were spotted onto LB agar plates supplemented with 350 μg/ml carbenicillin, 25 μg/ml chloramphenicol, 50 μg/ml kanamycin, 12.5 μg/ml tetracycline, 50 μg/ml X-gal (5-bromo-4-chloro-3-indolyl-β-D-galactopyranoside), and 20 μM IPTG. Growth of the bacterial cells was observed after incubation at 30°C for 36 h.
In vitro phosphotransfer assay
The in vitro phosphotransfer assay was performed essentially as described . The phospho-PmrBC276 protein was obtained by pre-incubation of His-PmrBC276 protein (5 μM) with 40 μCi of [γ-32P]ATP in 80 μl of 1× phosphorylation buffer (10 mM Tris-HCl, pH 7.5; 138 mM NaCl; 2.7 mM KCl; 1 mM MgCl2; 1 mM DTT) for 1 h at room temperature. The reaction mixture was then chilled on ice, and 5 μl of the mixture was removed and mixed with 2.5 μl of 5× SDS sample buffer as a reference sample. The phospho-PmrBC276 protein mixture (30 μl) was then mixed with equal volumes of 1× phosphorylation buffer containing either PmrA (10 μM) or PmrA with PmrD (each at 10 μM) to initiate the phosphotransfer reaction. A 10-μl aliquot was removed at specific time points, mixed with 2.5 μl of 5× SDS sample buffer to stop the reaction, and the samples were kept on ice until the performance of SDS-PAGE. After electrophoresis at 4°C, the signal was detected by autoradiography.
Kinase/phosphatase and autokinase assay
The assays were performed essentially as described . The recombinant protein His-PmrBC276 (2.5 μM) was incubated with His-PmrA (5 μM) alone or with His-PmrD (5 μM) for kinase/phosphatase assay or incubated with His-PmrD (5 μM) alone for autokinase assay. The reactions were carried out in 30 μl of 1× phosphorylation buffer with 3.75 μCi [γ-32P]ATP at room temperature and started with the addition of His-PmrBC276. An aliquot of 10-μl was removed at specific time points, mixed with 5× SDS sample buffer to stop the reaction, and the samples were kept on ice until the performance of SDS-PAGE. After electrophoresis at 4°C, the signal was detected by autoradiography.
Student's t test was used to determine the significance of the differences between the CPS amounts and the levels of β-galactosidase activity. P values less than 0.01 were considered statistically significant.
Reduced production of capsular polysaccharide had minor effect on polymyxin B resistance in K. pneumoniae
K. pneumoniae CG43 is a highly encapsulated virulent strain . In order to verify the role of CPS in polymyxin B resistance, the Δugd and Δwza mutants were generated by allelic exchange strategy, and their phenotype as well as the amount of CPS produced were compared with the parental strain CG43S3 and ΔrcsB mutant . As shown in Figure 1A, the Δugd and Δwza mutants formed apparently smaller colonies on LB agar plate compared with the glistering colony of the parental strain CG43S3. Although the colony morphology of the ΔrcsB mutant was indistinguishable from CG43S3, the CPS-deficient phenotype was evident as assessed using sedimentation assay and the amount of K2 CPS produced (Figure 1B). Deletion of rcsB resulted in an approximately 50% reduction of the CPS, while the Δwza mutant produced less than 20% of that of its parental strain CG43S3. The CPS biosynthesis in Δugd mutant was almost abolished, indicating an indispensible role of Ugd in CPS biosynthesis. To investigate how the CPS level was associated with polymyxin B resistance, the survival rates of the strains challenged with polymyxin B were compared. The Δugd mutant producing the lowest amount of CPS was extremely sensitive to the treatment of polymyxin B (Figure 1C). Although the Δugd mutant was CPS-deficient, the impaired polymyxin resistance may have been largely attributed to the defect in LPS biosynthesis since the survival rates of Δwza and ΔrcsB mutants appeared to be comparable with the parental strain CG43S3. This argues against the notion that the level of polymyxin B resistance is positively correlated to the amount of CPS . Nevertheless, the possibility that a higher amount of CPS was required for the resistance could not be ruled out. As shown in Figure 1D, the introduction of pRK415-RcsB  resulted in a significantly higher resistance to polymyxin B in both ΔrcsB mutant and its parental strain. This indicated a protective effect of large amounts of CPS in polymyxin resistance.
PmrF is involved in polymyxin B resistance and survival within macrophage
To investigate if the K. pneumoniae pmr homologues played a role in polymyxin B resistance, a pmrF deletion mutant strain and a plasmid pRK415-PmrF were generated. As shown in Figure 2A, when the strains were grown in LB medium, a low magnesium condition , differences in the survival rates were not apparent. When the strains were grown in LB supplemented with 1 mM FeCl3, an apparent deleting effect of pmrF in polymyxin B resistance was observed, and the survival rate could be restored by the introduction of pRK415-PmrF. The results indicated a role of PmrF in the polymyxin B resistance in high iron condition.
In addition to the mucosa surfaces, antimicrobial peptides and proteins play important roles in the microbicidal activity of phagosome . To investigate the effect of pmrF deletion in the bacterial survival within phagosome, phagocytosis assay was carried out. Since K. pneumoniae CG43S3 was highly resistant to engulfment by phagocytes in our initial experiments, the ΔrcsB mutant which produced less CPS was used as the parental strain to generate ΔpmrF ΔrcsB mutant. As shown in Figure 2B, deletion of pmrF resulted in an approximately four-fold reduction in the recovery rate, which was restored after the introduction of pRK415-PmrF. This indicated an important role of pmrF not only in polymyxin B resistance but also in bacterial survival within macrophage.
Deletion effect of pmrA, pmrD or phoP on polymyxin B resistance in K. pneumoniae
To investigate how PmrA, PhoP and PmrD were involved in the regulation of polymyxin B resistance in K. pneumoniae, ΔpmrA, ΔphoP and ΔpmrD mutant strains were generated. Deletion of either one of these genes resulted in a dramatic reduction of resistance to polymyxin B when the strains were grown in LB medium (Figure 3A). The deleting effects were no longer observed when the strains grown in LB supplemented with 10 mM magnesium, implying an involvement of the PhoP-dependent regulation in LB, a low magnesium environment. Under high-iron conditions, the deletion of pmrA caused the greatest reduction in the survival rate. Introduction of pRK415-PmrA or pRK415-PhoP into the ΔpmrA ΔphoP double mutant strain not only restored but also enhanced the bacterial resistance to polymyxin B (Figure 3B), which is likely due to an over-expression level of phoP or pmrA by the multicopy plasmid. Finally, whether the deletion of pmrA, phoP or pmrD affected the survival rate in phagosomes was also investigated. Interestingly, deletion of phoP resulted in most apparent effect while the pmrA deletion had less effect on the bacterial survival in macrophages. This was probably due to low iron concentration in the phagosomes . The introduction of pRK415-PhoP or pRK415-PmrD could restore the recovery rates of ΔphoP ΔrcsB and ΔpmrD ΔrcsB, although not to the extent displayed by the parental strain. Taken together, our results indicate the presence of two independent pathways in the regulation of polymyxin B resistance and the bacterial survival within macrophage phagosomes.
Effect of pmrA, phoP or pmrD deletion on P pmrH ::lacZ or P pmrD ::lacZ activity
Analysis of EMSA indicates a direct binding of the recombinant PhoP to pmrD
Two-hybrid analysis of the in vivo interaction between Klebsiella PmrD and PmrA
The PmrD binds to PmrA to prevent dephosphorylation
In S. enterica, the phosphorylation of PmrA by the cognate sensor protein PmrB has been demonstrated to enhance its affinity in binding to its target promoter. The subsequent dephosphorylation of PmrA by PmrB helped to relieve from over-activation of this system (1). In Salmonella, PmrD has been shown to be able to protect PmrA from both intrinsic and PmrB-mediated dephosphorylation (22). To verify if Klebsiella PmrD also participates in the phosphorylation, in vitro phosphotransfer assay was carried out with the recombinant proteins His-PmrA, His-PmrD and His-PmrBC276. As shown in Figure 6B, the His-PmrA was rapidly phosphorylated upon addition of the autophosphorylated His-PmrBC276 and then gradually dephosphorylated. Addition of His-PmrD apparently prolong the phosphorylation state of the His-PmrA, which could be maintained for at least 60 min (Figure 6B). The phosphorylated His-PmrA appeared to be very stable in the presence of the His-PmrD since the phosphorylation signal was still detectable 4 h later (data not shown). As shown in Figure 6C, the specificity of the interaction between His-PmrD and His-PmrA was also demonstrated since the phosphorylation state of His-PmrA could not be detected when incubated with the small cationic proteins RNase A or cytochrome C . Similar levels of phospho-PmrBC276 were observed in the presence or absence of PmrD (Figure 6D), suggesting the His-PmrD had no effect on the phorphorylation state of His-PmrBC276.
Although the amount of CPS produced by ΔrcsB mutant was more than twice of that produced by Δwza mutant, no apparent difference between the wild type strain CG43S3, Δwza mutant, and ΔrcsB mutant in polymyxin B resistance could be observed. This is different from the previous finding that K. pneumoniae CPS was an important physical barrier for the APs . This discrepancy may be attributed to some of the K. pneumoniae strains used for comparison in the previous study produced extremely low level of the CPS. Nevertheless, a higher amount of CPS was protective for the bacterial resistance to polymyxin B.
On the other hand, the deletion of ugd resulted in the loss of resistance to polymyxin B. Sequence analysis of the available K. pneumoniae genome NTHU-K2044 , MGH78578 (http://genome.wustl.edu/) and 342  revealed no PmrA  or PhoP box  in the upstream region of the manC-manB-ugd genes . This implies the involvement of a regulatory mechanism different from that for S. enterica ugd, which was positively regulated by the three 2CS regulators PhoP, PmrA and RcsB .
Consistent with the reported findings , deletion of Klebsiella pmrF which encodes one of the enzymes required for synthesis and incorporation of aminoarabinose in LPS resulted in decreased resistance to polymyxin B and survival within macrophages. The pmr expression has been shown to be directly regulated by PhoP under low magnesium or by PmrA in high ferric ions, or by the connector-mediated pathway reported for Salmonella,. Similar to the observations in E. coli, S. enterica, Yersinia pestis, and Pseudomonas aeruginosa, a positive regulatory role of PmrA and PhoP in polymyxin B resistance in K. pneumoniae was also demonstrated.
The deletion of phoP resulted in more drastic effect on the bacterial survival in macrophage than the pmrA deletion, implying a different level of control between PhoP and PmrA in K. pneumoniae resistance to phagocytosis. During phagocytosis, phagosomal maturation and phagolysosomes formation are accompanied by progressive acidification and acquisition of various hydrolases, reactive oxygen, nitrogen species, and APs . Low pH and low-magnesium have been shown to be able to stimulate expression of the PhoP-activated genes [40, 49]. Apart from its microbicidal activity, the APs inside phagosomes has even been reported as an inducing signal for the activation of the PhoP/PhoQ system . The deletion of pmrF or phoP caused a significant reduction in intramacrophage survival of the bacterial, implying a role of the AP resistance regulation in the bacterial pathogenesis.
Until now, PmrD was only found in E. coli, Shigella flexneri, S. enterica and K. pneumoniae. Although PmrD in Klebsiella appeared to act in a way similar to the PmrD in S. enterica, they share only about 40% sequence identity. The expression of K. pneumoniae pmrD was shown to be PhoP-dependent and the regulation was achieved through a direct binding of PhoP to the putative pmrD promoter. In addition, the binding of PmrD was shown to efficiently protect the PmrA from dephosphorylation. The in vivo interaction between PmrD and PmrA demonstrated using 2-hybrid analysis further supported the presence of the connector-mediated pathway in K. pneumoniae.
In summary, involvement of Klebsiella pmr in polymyxin B resistance and the regulation for the expression of pmr genes were analyzed. The regulatory network for the expression of the pmr genes is comprised of 2CS response regulators PhoP and PmrA, and the connector protein PmrD. The demonstration of PmrD in prolonging the phosphorylation state of phosphor-PmrA further confirmed the presence of a connector-mediated pathway in K. pneumoniae. The complexity in the control of pmr genes expression may provide ecological niches for K. pneumoniae in response to a variety of environmental clues; for example, in the process of infection.
We thank Dr. Chinpan Chen (Academia Sinica, Taipei, Taiwan) for providing the plasmids pET-PmrD and pET-PmrA. The work is supported by the grants from the National Research Program for Genome Medicine (NSC96-3112-B009-001) and National Science Council (97-2320-B-009-001-MY3).
- Podschun R, Ullmann U: Klebsiella spp. as nosocomial pathogens: epidemiology, taxonomy, typing methods, and pathogenicity factors. Clin Microbiol Rev. 1998, 11: 589-603.PubMed CentralPubMedGoogle Scholar
- Falagas ME, Kopterides P: Old antibiotics for infections in critically ill patients. Current opinion in critical care. 2007, 13: 592-597. 10.1097/MCC.0b013e32827851d7.View ArticlePubMedGoogle Scholar
- Falagas ME, Bliziotis IA: Pandrug-resistant Gram-negative bacteria: the dawn of the post-antibiotic era?. Int J Antimicrob Agents. 2007, 29: 630-636. 10.1016/j.ijantimicag.2006.12.012.View ArticlePubMedGoogle Scholar
- Kasiakou SK, Michalopoulos A, Soteriades ES, Samonis G, Sermaides GJ, Falagas ME: Combination therapy with intravenous colistin for management of infections due to multidrug-resistant Gram-negative bacteria in patients without cystic fibrosis. Antimicrob Agents Chemother. 2005, 49: 3136-3146. 10.1128/AAC.49.8.3136-3146.2005.PubMed CentralView ArticlePubMedGoogle Scholar
- Zavascki AP, Goldani LZ, Li J, Nation RL: Polymyxin B for the treatment of multidrug-resistant pathogens: a critical review. The Journal of antimicrobial chemotherapy. 2007, 60: 1206-1215. 10.1093/jac/dkm357.View ArticlePubMedGoogle Scholar
- Hancock RE: Peptide antibiotics. Lancet. 1997, 349: 418-422. 10.1016/S0140-6736(97)80051-7.View ArticlePubMedGoogle Scholar
- Kabha K, Nissimov L, Athamna A, Keisari Y, Parolis H, Parolis LA, Grue RM, Schlepper-Schafer J, Ezekowitz AR, Ohman DE: Relationships among capsular structure, phagocytosis, and mouse virulence in Klebsiella pneumoniae. Infect Immun. 1995, 63: 847-852.PubMed CentralPubMedGoogle Scholar
- Domenico P, Salo RJ, Cross AS, Cunha BA: Polysaccharide capsule-mediated resistance to opsonophagocytosis in Klebsiella pneumoniae. Infect Immun. 1994, 62: 4495-4499.PubMed CentralPubMedGoogle Scholar
- Cortes G, Borrell N, de Astorza B, Gomez C, Sauleda J, Alberti S: Molecular analysis of the contribution of the capsular polysaccharide and the lipopolysaccharide O side chain to the virulence of Klebsiella pneumoniae in a murine model of pneumonia. Infect Immun. 2002, 70: 2583-2590. 10.1128/IAI.70.5.2583-2590.2002.PubMed CentralView ArticlePubMedGoogle Scholar
- Campos MA, Vargas MA, Regueiro V, Llompart CM, Alberti S, Bengoechea JA: Capsule polysaccharide mediates bacterial resistance to antimicrobial peptides. Infect Immun. 2004, 72: 7107-7114. 10.1128/IAI.72.12.7107-7114.2004.PubMed CentralView ArticlePubMedGoogle Scholar
- Whitfield C, Paiment A: Biosynthesis and assembly of Group 1 capsular polysaccharides in Escherichia coli and related extracellular polysaccharides in other bacteria. Carbohydr Res. 2003, 338: 2491-2502. 10.1016/j.carres.2003.08.010.View ArticlePubMedGoogle Scholar
- Drummelsmith J, Whitfield C: Translocation of group 1 capsular polysaccharide to the surface of Escherichia coli requires a multimeric complex in the outer membrane. EMBO J. 2000, 19: 57-66. 10.1093/emboj/19.1.57.PubMed CentralView ArticlePubMedGoogle Scholar
- Majdalani N, Gottesman S: The Rcs phosphorelay: a complex signal transduction system. Annu Rev Microbiol. 2005, 59: 379-405. 10.1146/annurev.micro.59.050405.101230.View ArticlePubMedGoogle Scholar
- Lai YC, Peng HL, Chang HY: RmpA2, an activator of capsule biosynthesis in Klebsiella pneumoniae CG43, regulates K2 cps gene expression at the transcriptional level. J Bacteriol. 2003, 185: 788-800. 10.1128/JB.185.3.788-800.2003.PubMed CentralView ArticlePubMedGoogle Scholar
- Kim SH, Jia W, Parreira VR, Bishop RE, Gyles CL: Phosphoethanolamine substitution in the lipid A of Escherichia coli O157: H7 and its association with PmrC. Microbiology (Reading, England). 2006, 152: 657-666.View ArticleGoogle Scholar
- Gunn JS, Ryan SS, Van Velkinburgh JC, Ernst RK, Miller SI: Genetic and functional analysis of a PmrA-PmrB-regulated locus necessary for lipopolysaccharide modification, antimicrobial peptide resistance, and oral virulence of Salmonella enterica serovar typhimurium. Infect Immun. 2000, 68: 6139-6146. 10.1128/IAI.68.11.6139-6146.2000.PubMed CentralView ArticlePubMedGoogle Scholar
- Wosten MM, Groisman EA: Molecular characterization of the PmrA regulon. The Journal of biological chemistry. 1999, 274: 27185-27190. 10.1074/jbc.274.38.27185.View ArticlePubMedGoogle Scholar
- Yan A, Guan Z, Raetz CR: An undecaprenyl phosphate-aminoarabinose flippase required for polymyxin resistance in Escherichia coli. The Journal of biological chemistry. 2007, 282: 36077-36089. 10.1074/jbc.M706172200.PubMed CentralView ArticlePubMedGoogle Scholar
- Breazeale SD, Ribeiro AA, McClerren AL, Raetz CR: A formyltransferase required for polymyxin resistance in Escherichia coli and the modification of lipid A with 4-Amino-4-deoxy-L-arabinose. Identification and function oF UDP-4-deoxy-4-formamido-L-arabinose. The Journal of biological chemistry. 2005, 280: 14154-14167. 10.1074/jbc.M414265200.View ArticlePubMedGoogle Scholar
- Marceau M, Sebbane F, Ewann F, Collyn F, Lindner B, Campos MA, Bengoechea JA, Simonet M: The pmrF polymyxin-resistance operon of Yersinia pseudotuberculosis is upregulated by the PhoP-PhoQ two-component system but not by PmrA-PmrB, and is not required for virulence. Microbiology (Reading, England). 2004, 150: 3947-3957.View ArticleGoogle Scholar
- Tamayo R, Ryan SS, McCoy AJ, Gunn JS: Identification and genetic characterization of PmrA-regulated genes and genes involved in polymyxin B resistance in Salmonella enterica serovar typhimurium. Infect Immun. 2002, 70: 6770-6778. 10.1128/IAI.70.12.6770-6778.2002.PubMed CentralView ArticlePubMedGoogle Scholar
- Lacour S, Bechet E, Cozzone AJ, Mijakovic I, Grangeasse C: Tyrosine phosphorylation of the UDP-glucose dehydrogenase of Escherichia coli is at the crossroads of colanic acid synthesis and polymyxin resistance. PLoS One. 2008, 3: e3053-10.1371/journal.pone.0003053.PubMed CentralView ArticlePubMedGoogle Scholar
- Wosten MM, Kox LF, Chamnongpol S, Soncini FC, Groisman EA: A signal transduction system that responds to extracellular iron. Cell. 2000, 103: 113-125. 10.1016/S0092-8674(00)00092-1.View ArticlePubMedGoogle Scholar
- Gunn JS: The Salmonella PmrAB regulon: lipopolysaccharide modifications, antimicrobial peptide resistance and more. Trends Microbiol. 2008, 16: 284-290. 10.1016/j.tim.2008.03.007.View ArticlePubMedGoogle Scholar
- Winfield MD, Groisman EA: Phenotypic differences between Salmonella and Escherichia coli resulting from the disparate regulation of homologous genes. Proc Natl Acad Sci USA. 2004, 101: 17162-17167. 10.1073/pnas.0406038101.PubMed CentralView ArticlePubMedGoogle Scholar
- Perez JC, Groisman EA: Acid pH activation of the PmrA/PmrB two-component regulatory system of Salmonella enterica. Molecular microbiology. 2007, 63: 283-293. 10.1111/j.1365-2958.2006.05512.x.PubMed CentralView ArticlePubMedGoogle Scholar
- Kato A, Tanabe H, Utsumi R: Molecular characterization of the PhoP-PhoQ two-component system in Escherichia coli K-12: identification of extracellular Mg2+-responsive promoters. J Bacteriol. 1999, 181: 5516-5520.PubMed CentralPubMedGoogle Scholar
- Kox LF, Wosten MM, Groisman EA: A small protein that mediates the activation of a two-component system by another two-component system. Embo J. 2000, 19: 1861-1872. 10.1093/emboj/19.8.1861.PubMed CentralView ArticlePubMedGoogle Scholar
- Kato A, Latifi T, Groisman EA: Closing the loop: the PmrA/PmrB two-component system negatively controls expression of its posttranscriptional activator PmrD. Proc Natl Acad Sci USA. 2003, 100: 4706-4711. 10.1073/pnas.0836837100.PubMed CentralView ArticlePubMedGoogle Scholar
- Kato A, Groisman EA: Connecting two-component regulatory systems by a protein that protects a response regulator from dephosphorylation by its cognate sensor. Genes Dev. 2004, 18: 2302-2313. 10.1101/gad.1230804.PubMed CentralView ArticlePubMedGoogle Scholar
- Mitrophanov AY, Jewett MW, Hadley TJ, Groisman EA: Evolution and dynamics of regulatory architectures controlling polymyxin B resistance in enteric bacteria. PLoS genetics. 2008, 4: e1000233-10.1371/journal.pgen.1000233.PubMed CentralView ArticlePubMedGoogle Scholar
- Chang HY, Lee JH, Deng WL, Fu TF, Peng HL: Virulence and outer membrane properties of a galU mutant of Klebsiella pneumoniae CG43. Microb Pathog. 1996, 20: 255-261. 10.1006/mpat.1996.0024.View ArticlePubMedGoogle Scholar
- Peng HL, Wang PY, Wu JL, Chiu CT, Chang HY: Molecular epidemiology of Klebsiella pneumoniae. Zhonghua Min Guo Wei Sheng Wu Ji Mian Yi Xue Za Zhi. 1991, 24: 264-271.PubMedGoogle Scholar
- Skorupski K, Taylor RK: Positive selection vectors for allelic exchange. Gene. 1996, 169: 47-52. 10.1016/0378-1119(95)00793-8.View ArticlePubMedGoogle Scholar
- Lin CT, Huang TY, Liang WC, Peng HL: Homologous response regulators KvgA, KvhA and KvhR regulate the synthesis of capsular polysaccharide in Klebsiella pneumoniae CG43 in a coordinated manner. J Biochem (Tokyo). 2006, 140: 429-438.View ArticleGoogle Scholar
- Keen NT, Tamaki S, Kobayashi D, Trollinger D: Improved broad-host-range plasmids for DNA cloning in gram-negative bacteria. Gene. 1988, 70: 191-197. 10.1016/0378-1119(88)90117-5.View ArticlePubMedGoogle Scholar
- Domenico P, Schwartz S, Cunha BA: Reduction of capsular polysaccharide production in Klebsiella pneumoniae by sodium salicylate. Infect Immun. 1989, 57: 3778-3782.PubMed CentralPubMedGoogle Scholar
- Miller JH: Experiments in Molecular Genetics. 1972, Cold Spring Harbor Laboratory Press, Cold Spring Harbor, N.Y.Google Scholar
- Cheng HY, Chen YS, Wu CY, Chang HY, Lai YC, Peng HL: RmpA regulation of capsular polysaccharide biosynthesis in Klebsiella pneumoniae CG43. J Bacteriol. 192: 3144-3158. 10.1128/JB.00031-10.
- Groisman EA: The ins and outs of virulence gene expression: Mg2+ as a regulatory signal. Bioessays. 1998, 20: 96-101. 10.1002/(SICI)1521-1878(199801)20:1<96::AID-BIES13>3.0.CO;2-3.View ArticlePubMedGoogle Scholar
- Benincasa M, Mattiuzzo M, Herasimenka Y, Cescutti P, Rizzo R, Gennaro R: Activity of antimicrobial peptides in the presence of polysaccharides produced by pulmonary pathogens. J Pept Sci. 2009, 15: 595-600. 10.1002/psc.1142.View ArticlePubMedGoogle Scholar
- Wu KM, Li LH, Yan JJ, Tsao N, Liao TL, Tsai HC, Fung CP, Chen HJ, Liu YM, Wang JT, Fang CT, Chang SC, Shu HY, Liu TT, Chen YT, Shiau YR, Lauderdale TL, Su IJ, Kirby R, Tsai SF: Genome Sequencing and Comparative Analysis of Klebsiella pneumoniae NTUH-K2044, a Strain Causing Liver Abscess and Meningitis. Journal of bacteriology. 2009Google Scholar
- Fouts DE, Tyler HL, DeBoy RT, Daugherty S, Ren Q, Badger JH, Durkin AS, Huot H, Shrivastava S, Kothari S, Dodson RJ, Mohamoud Y, Khouri H, Roesch LF, Krogfelt KA, Struve C, Triplett EW, Methé BA: Complete genome sequence of the N2-fixing broad host range endophyte Klebsiella pneumoniae 342 and virulence predictions verified in mice. PLoS genetics. 2008, 4: e1000141-10.1371/journal.pgen.1000141.PubMed CentralView ArticlePubMedGoogle Scholar
- Chuang YP, Fang CT, Lai SY, Chang SC, Wang JT: Genetic determinants of capsular serotype K1 of Klebsiella pneumoniae causing primary pyogenic liver abscess. J Infect Dis. 2006, 193: 645-654. 10.1086/499968.View ArticlePubMedGoogle Scholar
- Mouslim C, Groisman EA: Control of the Salmonella ugd gene by three two-component regulatory systems. Molecular microbiology. 2003, 47: 335-344. 10.1046/j.1365-2958.2003.03318.x.View ArticlePubMedGoogle Scholar
- Winfield MD, Latifi T, Groisman EA: Transcriptional regulation of the 4-amino-4-deoxy-L-arabinose biosynthetic genes in Yersinia pestis. J Biol Chem. 2005, 280: 14765-14772. 10.1074/jbc.M413900200.View ArticlePubMedGoogle Scholar
- Moskowitz SM, Ernst RK, Miller SI: PmrAB, a two-component regulatory system of Pseudomonas aeruginosa that modulates resistance to cationic antimicrobial peptides and addition of aminoarabinose to lipid A. J Bacteriol. 2004, 186: 575-579. 10.1128/JB.186.2.575-579.2004.PubMed CentralView ArticlePubMedGoogle Scholar
- Flannagan RS, Cosio G, Grinstein S: Antimicrobial mechanisms of phagocytes and bacterial evasion strategies. Nat Rev Microbiol. 2009, 7: 355-366. 10.1038/nrmicro2128.View ArticlePubMedGoogle Scholar
- Groisman EA: The pleiotropic two-component regulatory system PhoP-PhoQ. J Bacteriol. 2001, 183: 1835-1842. 10.1128/JB.183.6.1835-1842.2001.PubMed CentralView ArticlePubMedGoogle Scholar
- Otto M: Bacterial sensing of antimicrobial peptides. Contrib Microbiol. 2009, 16: 136-149. full_text.PubMed CentralView ArticlePubMedGoogle Scholar
This article is published under license to BioMed Central Ltd. This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/2.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.