- Research article
- Open Access
Characterization of Plp, a phosphatidylcholine-specific phospholipase and hemolysin of Vibrio anguillarum
© Li et al.; licensee BioMed Central Ltd. 2013
- Received: 12 August 2013
- Accepted: 20 November 2013
- Published: 27 November 2013
Vibrio anguillarum is the causative agent of vibriosis in fish. Several extracellular proteins secreted by V. anguillarum have been shown to contribute to virulence. While two hemolysin gene clusters, vah1-plp and rtxACHBDE, have been previously identified and described, the activities of the protein encoded by the plp gene were not known. Here we describe the biochemical activities of the plp-encoded protein and its role in pathogenesis.
The plp gene, one of the components in vah1 cluster, encodes a 416-amino-acid protein (Plp), which has homology to lipolytic enzymes containing the catalytic site amino acid signature SGNH. Hemolytic activity of the plp mutant increased 2-3-fold on sheep blood agar indicating that plp represses vah1; however, hemolytic activity of the plp mutant decreased by 2-3-fold on fish blood agar suggesting that Plp has different effects against erythrocytes from different species. His6-tagged recombinant Plp protein (rPlp) was over-expressed in E. coli. Purified and re-folded active rPlp exhibited phospholipase A2 activity against phosphatidylcholine and no activity against phosphatidylserine, phosphatidylethanolamine, or sphingomyelin. Characterization of rPlp revealed broad optimal activities at pH 5–9 and at temperatures of 30-64°C. Divalent cations and metal chelators did not affect activity of rPlp. We also demonstrated that Plp was secreted using thin layer chromatography and immunoblot analysis. Additionally, rPlp had strong hemolytic activity towards rainbow trout erythrocytes, but not to sheep erythrocytes suggesting that rPlp is optimized for lysis of phosphatidylcholine-rich fish erythrocytes. Further, only the loss of the plp gene had a significant effect on hemolytic activity of culture supernatant on fish erythrocytes, while the loss of rtxA and/or vah1 had little effect. However, V. anguillarum strains with mutations in plp or in plp and vah1 exhibited no significant reduction in virulence compared to the wild type strain when used to infect rainbow trout.
The plp gene of V. anguillarum encoding a phospholipase with A2 activity is specific for phosphatidylcholine and, therefore, able to lyse fish erythrocytes, but not sheep erythrocytes. Mutation of plp does not affect the virulence of V. anguillarum in rainbow trout.
- Vibrio anguillarum
Vibrio anguillarum, a highly motile marine member of the γ-Proteobacteria, is one of the causative agents of vibriosis, a fatal hemorrhagic septicemic disease of both wild and cultured fish, crustaceans, and bivalves . Fish infected with V. anguillarum display skin discoloration and erythema around the mouth, fins, and vent. Necrotic lesions are also observed in the abdominal muscle . Mortality rates in infected fish populations range as high as 30-100% [1, 3]. Vibriosis has caused severe economic losses to aquaculture worldwide [1, 3] and affects many farm-raised fish including Pacific salmon, Atlantic salmon, sea bass, cod, and eel [3, 4]. V. anguillarum enters its fish host through the gastrointestinal tract (GI) and quickly colonizes this nutrient rich environment [2, 5]. Garcia et al.  have shown that V. anguillarum grows extremely well in salmon intestinal mucus and that mucus-grown cells specifically express a number of different proteins, including several outer membrane proteins  and the extracellular metalloprotease EmpA [2, 5].
Several genes have been reported to be correlated with virulence by V. anguillarum, including the vah1 hemolysin cluster [7, 8], the rtx hemolysin cluster , the siderophore mediated iron transport system , the empA metalloprotease [2, 5], and the flaA gene . Hemolytic activity of V. anguillarum has been considered to be the virulence factor responsible for hemorrhagic septicemia during infection . We have identified two hemolysin gene clusters in V. anguillarum that contribute to the virulence of this pathogen [8, 9]. One gene cluster, rtxACHBDE, encodes a MARTX toxin and its type I secretion system . The second hemolysin gene cluster in V. anguillarum strain M93Sm contains the hemolysin gene vah1 flanked by two putative lipase-related genes (llpA and llpB) immediately downstream and upstream by a divergently transcribed hemolysin-like gene (plp) that appears to function as a repressor of vah1-dependent hemolytic activity . The plp-encoded protein has very high sequence similarity to phospholipases found in other pathogenic Vibrio species . However, the enzymatic characteristics of Plp in V. anguillarum were not described.
Generally, phospholipases are divided into several subgroups depending on their specificity for hydrolysis of ester bonds at different locations in the phospholipid molecule. Phospholipases A (PLAs) cleave long chain fatty acids at sn-1 (PLA1) or sn-2 (PLA2) position from phospholipid to yield lysophospholipid and free fatty acid; phospholipases C (PLCs) cleave phospholipid into diacylglycerol and a phosphate-containing head group; and phospholipases D (PLDs) cleave phospholipid into phosphatidic acid and an alcohol. It is known that some phospholipid products are used as secondary messages, which play a central role in signal transduction .
In this study, we determined that plp encodes a phospholipase A2 in V. anguillarum, and then purified recombinant Plp protein (rPlp) from E. coli to investigate its biochemical properties. We also described the contribution and specificity of rPlp for hydrolysis of phospholipids, and its ability to lyse fish erythrocytes.
Identification of a putative phospholipase gene plp
Plp affects hemolysis of fish erythrocytes
Plp has phospholipase A2 activity
Enzymatic characteristics of rPlp protein
To examine the enzymatic characteristics of Plp, the entire coding sequence of plp was cloned and inserted into the expression vector pQE60, which adds a His6 (His-6×) tag to the carboxyl end of Plp. The over-expressed recombinant Plp (rPlp) formed inclusion bodies in E. coli. To recover active rPlp, purification of the inclusion bodies followed by solubilization under mild conditions and re-folding was performed as described in the Methods. Purity of refolded rPlp protein was confirmed by SDS-PAGE and silver staining (data not shown). The final concentration of purified rPlp protein was 8 μg/ml with a recovery of <10%.
The effect of pH on enzyme activity was determined for pH values ranging from 2 to 12. The data showed that rPlp had a broad pH optimum from pH 5.3 to pH 8.7 with activity dropping off rapidly at pH values above and below the optimum (Figure 4C). rPlp activity was not affected by treatment with the chelating reagents EGTA (Figure 4D) or EDTA (data not shown) at concentrations up to 100 mM. Additionally, treatment with divalent metal ions, such as calcium or magnesium had no effect on activity (data not shown).
Plp is a secreted protein in V. anguillarum
In order to confirm that Plp was localized in the supernatant of V. anguillarum, protein samples prepared from various subcellular fractions were separated by SDS-PAGE and analyzed by western blot analysis using polyclonal rabbit anti-Plp antiserum. An immuno-reactive band of ~45 kDa was detected only in the supernatant of M93Sm, but was absent in the supernatant of plp mutant (Figure 5C). Taken together with the phospholipase A2 activity data, these data indicate that Plp is a secreted protein in V. anguillarum.
rPlp has a specific activity against phosphatidylcholine
rPlp is able to lyse the fish erythrocytes directly
Plp is one of the hemolysins of V. anguillarum
Bacterial strains and plasmids used in this study
Strain or plasmid
V. anguillarum strains
Spontaneous Smr mutant of M93 (serotype O2a); parental strain isolated from a diseased ayu (Plecoglossus altivelis) from Lake Biwa, Japan
Smr Cmrvah1; insertional vah1 mutant of M93Sm
Smr Cmr Tcrvah1+; vah1 complement strain of JR1
Smr Cmrplp; insertional plp mutant of M93Sm
Smr Cmr Tcrplp+; plp complement strain of S262
Smr CmrrtxA; insertional rtxA mutant of M93Sm
Smr Cmr Kmrvah1 plp; insertional vah1mutant of JL01
Smr Cmr Kmrvah1 rtxA; insertional rtxA mutant of S171
Smr Cmr Kmr Tcrvah1+ rtxA; vah1 complement strain of S183
Smr Cmr Kmrplp rtxA; insertional rtxA mutant of JL01
Smr Cmr Kmrvah1 plp rtxA; insertional plp mutant of S264
Smr Cmr Kmr Tcrvah1 plp + rtxA; plp complement strain of XM90
Smr Kmrplp; mini-Tn10Km insertion into plp
Smr Kmrvah1; allelic exchange vah1 mutant
Smr Kmrvah1 rtxA; allelic exchange vah1 and rtxA mutant
E. coli strains
thi thr leu tonA lacY supE recA RP4-2-Tc::Mu::Km (λ pir)
Kmr Cmr; Sm10 containing plasmid pNQ705-plp
Kmr Cmr; Sm10 containing plasmid pNQ705-rtxA
Kmr Cmr; Sm10 containing plasmid pDM4-rtxA5'
Kmr Cmr; Sm10 containing plasmid pDM4-rtxA5'-rtxA3'
Kmr Apr Tcr; Sm10 containing plasmid pSUP202-vah1
Kmr Apr Tcr; Sm10 containing plasmid pSUP202-plp
NalS StrS RifSthi–lac–ara+gal+mtl– F–recA+uvr+lon+ (pREP4)
Kmr Apr; M15 containing plasmid pQE30UA-plp
Kmr Apr; M15 containing plasmid pQE60-plp
Kmr Apr; Cloning vector
Cmr; suicide vector with R6K origin
Cmr; for insertional vah1mutation
Cmr; for insertional plp mutation
Cmr; for insertional rtxA mutation
Cmr SacBCr; suicide vector with R6K origin
Cmr SacBCr; for allelic exchange rtxA mutation
Cmr Apr Tcr; E. coli – V. anguillarum shuttle vector
Apr Tcr; for complementation of vah1
Apr Tcr; for complementation of plp
Apr; expression vector with N-terminal His6-tag
Apr; for expression of rPlp that is used to make anti-Plp
Apr; expression vector with C-terminal His6-tag
Apr; for expression of rPlp for enzymatic activity analysis
Hemolytic activity of culture supernatant from V. anguillarum wild-type and various V. anguillarum mutant strains against rainbow trout blood cells
V. anguillarumstrain or treatment
Hemolytic activity (Relative to wild-type control ± SD)a
JR03 (plp vah1)
S183 (vah1 rtxA)
XM62 (vah1+ rtxA)
S187 (plp rtxA)
XM90 (vah1 rtxA plp)
XM93 (vah1 rtxA plp+)
Water (positive control)
In contrast to the strong hemolytic activity against 5% rainbow trout blood mixed with culture supernatant from the wild type strain M93Sm, hemolytic activity of culture supernatant from strain S262 (plp) declined by >70% (Table 2). Additionally, all mutants containing a knockout of plp exhibited significant declines (P < 0.05) in hemolytic activity. The triple hemolysin mutant, XM90 (plp vah1 rtxA) had no ability to lyse fish erythrocytes (Table 2). However, mutations in either vah1 or rtxA, but not plp, resulted in little or no decline in hemolytic activity against fish erythrocytes compared to supernatants from wild type cells (Table 2). Further, complementation of plp restored the hemolytic activity of supernatants from both the plp-complemented strains (XM31, plp + and XM93, vah1 rtxA plp+) (Table 2). Taken together, these data clearly demonstrate that Plp is the major hemolytic enzyme responsible for the lysis of rainbow trout erythrocytes by culture supernatants of V. anguillarum.
Plp is not a major virulence factor for V. anguillarumduring fish infection
In this report, we describe the characteristics of the V. anguillarum phospholipase protein (Plp) encoded by plp, and its contribution to the hemolytic activity of V. anguillarum. Specifically, we show that Plp is a secreted phospholipase with A2 activity with specificity for phosphatidylcholine. The enzyme has a broad temperature optimum (37 – 64°C) and a broad pH optimum (pH 5.5 – 8.7). Phospholipases are broadly distributed among the Vibrionaceae and often contribute to the virulence of the pathogenic members of this family. For example, the TLH or LDH of V. parahaemolyticus[23–25] was the first well-studied lecithin-dependent PLA/lysophospholipase . A lecithinase (encoded by lec) was also identified in V. cholerae. Fiore et al. found that a lec mutant strain was unable to degrade lecithin and the culture supernatant exhibited decreased cytotoxicity. However, the mutant did not exhibit decreased fluid accumulation in a rabbit ileal loop assay, suggesting that fluid accumulation in animals is not affected by lecithinase activity. Additionally, the phospholipase A (PhlA) in V. mimicus was found to exhibit hemolytic activity against trout and tilapia erythrocytes and was cytotoxic to the fish cell line CHSE-214 . Recently, the V. harveyi hemolysin (VHH) was shown to be a virulence factor during flounder infection and also had phospholipase activity on egg yolk agar . Rock and Nelson  reported that the putative phospholipase gene (plp) from V. anguillarum exhibits 69% amino acid identity with the V. cholerae lec gene. Both plp and lec are located divergently adjacent to a hemolysin gene (vah1 and hlyA, respectively) [8, 27]. Additionally, Rock and Nelson  demonstrated that functional plp repressed transcription of its adjacent hemolysin gene, vah1, in V. anguillarum. However, the enzymatic characteristics of Plp in V. anguillarum were not described.
Usually, phospholipases are divided into phospholipases A (A1 and A2), C, and D according to the cleavage position on target phospholipids. Most of lipolytic enzymes contain a putative lipid catalytic motif (GDSL) that was previously demonstrated in other bacterial and eukaryotic phospholipases . However, Molgaard  demonstrated that four amino acid residues (SGNH) form a catalytic site, and are conserved in all members of the phospholipase family; therefore, phospholipases were re-named as the SGNH subgroup of the GDSL family . Multiple alignment analysis of 17 phospholipase homologues (Figure 1) demonstrates that V. anguillarum Plp belongs to the SGNH hydrolase subgroup, since the GSDL motif was not fully conserved in these proteins (Figure 1). Recently, it was reported that mutation of the serine residue in the SGNH motif resulted in the complete loss of the phospholipase and hemolytic activities of VHH in V. harveyi demonstrating the importance of this motif on the activity of phospholipase.
In contrast to the similarities of their catalytic motifs, the biochemical characteristics of bacterial phospholipases appear to be variable. For example, V. mimicus PhlA has a phospholipase A activity, which cleaves the fatty acid at either sn-1or sn-2 position, but no lysophospholipase activity . Two phospholipases identified from mesophilic Aeromonas sp. serogroup O:34 show phospholipase A1 and C activity . In addition, TLH of V. parahaemolyticus has PLA2 and lysophospholipase activity, and demonstrates a loss of activity at 55°C for 10 min . In this report, we show that V. anguillarum Plp has PLA2 activity, and is able to maintain activity at 64°C for 1 h (Figures 6 and 7). Therefore, the enzymatic characteristics of specific phospholipases are distinct even when they all belong to the SGNH hydrolase family (Figure 1).
Phospholipases have been implicated in the pathogenic activities of a number of bacteria [33, 34]. It is known that phospholipase activities often lead to cell destruction by degrading the phospholipids of cell membranes [33, 35]. However, the relationships between phospholipases and virulence are not always clear. While the purified rPlp exhibits strong hemolytic activity against Atlantic salmon erythrocytes (Figure 7), Rock and Nelson  showed that a knock-out mutation of either the plp gene or the vah1 gene in V. anguillarum did not affect virulence of V. anguillarum during an infection study on juvenile Atlantic salmon. In this report, we show that when groups of rainbow trout are infected with either a plp mutant or a plp vah1 double mutant there is no significant difference in mortalities compared to fish infected with the wild type strain. Our data suggest that neither plp nor vah1 are major virulence factors during pathogenesis of salmonids. It was also reported that the deletion of lecithinase (Lec) activity in V. cholerae did not significantly diminish fluid accumulation in the rabbit ileal loop assay, indicating the lecithinase activity does not contribute significantly to enterotoxin activity . Lec is a homologue of Plp . In contrast, the direct IP injection of purified V. harveyi VHH protein caused the death of flounder with an LD50 of about 18.4 μg protein/fish . The rPhlA of V. mimicus also has a direct cytotoxic effect on the fish cell line CHSE-214  suggesting that this phospholipase is a virulence factor during fish infection. In addition, the lecithinase purified from A. hydrophila (serogroup O:34) has been shown to be an important virulence factor to rainbow trout and mouse . We note that infection experiments in both Atlantic salmon and rainbow trout demonstrate that mutation of plp does not attenuate virulence. We propose that V. anguillarum is able to compensate for the loss of Plp-mediated hemolytic activity in vivo by up-regulating the transcription of vah1, as previously described by Rock and Nelson . Additionally, transcription of rtxA is also increased in a plp mutant (Mou and Nelson, unpublished data).
Generally, the hemolytic activity of phospholipases is dependent upon the hydrolysis of the phospholipids that reside in the erythrocyte membrane. Erythrocytes contain various phospholipids including phosphatidylcholine (PC), phosphatidylethanolamine (PE), phosphatidylserine (PS), phosphatidylinositol (PI), and sphingomyelin (SM). PC makes up 58% of the total erythrocyte phospholipids in the Atlantic salmon , but only 34% and 1% in rabbit and sheep erythrocytes, respectively . Taken together with the high specificity of rPlp for PC (Figure 6), it was not surprising that rPlp was able to lyse the fish erythrocytes, but not sheep erythrocytes (Figure 7), and that the plp mutant had decreased hemolytic activity on LB20-fish blood agar (Figure 2). Our results are consistent were those reported for V. mimicus PhlA  and V. harveyi VHH , in which PhlA and VVH specifically lyse the fish erythrocytes.
We have previously reported that there are two hemolysin gene clusters in V. anguillarum M93Sm, the vah1-plp cluster and rtxACHBDE cluster  and have described their regulation by H-NS and HlyU [17, 37]. Mutation of both vah1 and rtxA results in the loss of all hemolytic activity on TSA-sheep blood agar , which is consistent with the data reported here that Plp has no activity on sheep erythrocytes. We have also previously demonstrated that Plp is a putative repressor of Vah1, since mutation of plp increases vah1 expression by 2–3 fold . In this report, we examined the hemolytic activity of various hemolysin mutants using freshly collected Rainbow trout blood (Table 2) to investigate the relationships among three hemolysins of V. anguillarum. While culture supernatants from two of the three single mutants (JR1 and S123) and one of three double mutants (S183) exhibited ≥94% of the hemolytic activity as supernatants from the wild type strain M93Sm (Table 2), the hemolytic activity of one single mutant (S262, plp) and two double mutants (JR03, plp vah1 and S187, plp rtxA) were reduced to 28%, 14%, and 12% of that in M93Sm, respectively. Our data indicate that only the loss of the plp gene has a significant effect on hemolysis of fish erythrocytes by V. anguillarum culture supernatant, while the loss of rtxA and/or vah1 has little effect. Further, supernatant from the hemolysin triple mutant XM90 (vah1 rtxA plp) exhibits no hemolytic activity on fish blood compared to M93Sm (Table 2), indicating that Vah1, RtxA, and Plp are responsible for all secreted hemolytic activity by V. anguillarum. Finally, complementation of any plp mutant with plp (in trans) restores hemolytic activity to V. anguillarum culture supernatant (Table 2).
V. anguillarum Plp is a secreted hemolysin with phosphatidylcholine-specific phospholipase A2 activity. The ability of Plp to digest the abundant phosphatidylcholine found in the membrane of fish erythrocytes causes their lysis. The three hemolysins, Plp, Vah1 and RtxA, account for all hemolytic activity in V. anguillarum culture supernatant under the experiment conditions described in this study. Finally, infection studies in rainbow trout demonstrate that the plp and vah1 genes are not required for virulence.
Bacterial strains, plasmids, and growth conditions
All bacterial strains and plasmids used in this report are listed in Table 1. V. anguillarum strains were routinely grown in Luria-Bertani broth plus 2% NaCl (LB20) , supplemented with the appropriate antibiotic, in a shaking water bath at 27°C. E. coli strains were routinely grown in Luria-Bertani broth plus 1% NaCl (LB10). Antibiotics were used at the following concentrations: streptomycin, 200 μg/ml; ampicillin, 100 μg/ml (Ap100); chloramphenicol, 20 μg/ml (Cm20) for E. coli and 5 μg/ml (Cm5) for V. anguillarum; kanamycin, 50 μg/ml (Km50) for E. coli and 80 μg/ml (Km80) for V. anguillarum; tetracycline, 15 μg/ml (Tc15) for E. coli, 1 μg/ml (Tc1) for V. anguillarum grown in liquid medium, and 2 μg/ml (Tc2) for V. anguillarum grown on agar plates.
Primers used in this study
Sequence (5' to 3', italicized sequences are designed restriction sites)
Purpose and description
For whole Plp protein, forward
For whole Plp protein, reverse
For truncated Plp protein, forward
For truncated Plp protein, reverse
For insertional plp mutation, forward, with SacI site
SD Lip/Heme R1
For insertional plp mutation, reverse, with XbaI site
For plp complement, forward, with EcoRI site
For plp complement, reverse, with AgeI site
For vah1 complement, forward, with EcoRI site
For vah1 complement, reverse, with AgeI site
For allelic exchange rtxA mutation, flanking the 5' region, forward, with XhoI site
For allelic exchange rtxA mutation, flanking the 5' region, reverse, with XbaI site
For allelic exchange rtxA mutation, flanking the 3' region, forward, with XbaI site
For allelic exchange rtxA mutation, flanking the 3' region, reverse, with SacI site
For sequencing of the DNA fragment inserted in pCR2.1 TA-ligation site
For sequencing of the DNA fragment inserted in pSUP202 AgeI site
For sequencing of the DNA fragment inserted in pNQ705-1 Multi-cloning site
Allelic exchange mutagenesis
The allelic exchange rtxA mutation in V. anguillarum S264 was made by using a modification of the procedure described by Milton et al.. The 5′ region of rtxA was amplified using the primer pair pm256 and pm257 (Table 3), digested with XhoI and XbaI, and then cloned into the region between the XhoI and XbaI sites on pDM4 (GenBank accession no. KC795686), deriving pDM4-rtxA5′. The 3′ region of rtxA was amplified using the primer pair pm258 and pm259 (Table 3), digested with XbaI and SacI, and then cloned into the region between the XbaI and SacI sites on the pDM4-rtxA5′. The resulting pDM4-rtxA5′-rtxA3′ was transformed into E. coli Sm10 to produce the transformant strain S252, which was mated with V. anguillarum S171 (vah1). Single-crossover transconjugants were selected with LB20 Kan80 Sm200 Cm5 plates and, subsequently, double-crossover transconjugants (resulting in a 3345 bp deletion in C-terminal of RtxA) were selected with LB20 Kan80 Sm200 5% sucrose plates. The resulting V. anguillarum colonies were transferred to TSA-sheep blood agar (Northeast Laboratories Service, Waterville, ME) and screened for none-hemolytic colonies (vah1 rtxA). The resulting colonies were checked for the desired allelic exchange using PCR amplification.
Complementation of mutants
The various mutants were complemented by cloning the appropriate target gene fragment into the shuttle vector pSUP202 (GenBank accession no. AY428809) as described previously by . Briefly, primers (Table 3) were designed with EcoRI and AgeI sites and then used to amplify the entire target gene plus ~500 bp of the 5′ and ~200 bp 3′flanking regions from genomic DNA of V. anguillarum M93Sm. The DNA fragment was then ligated into pSUP202 after digestion with EcoRI and AgeI, and the ligation mixture was introduced into E. coli Sm10 by electroporation using a BioRad Gene Pulser II. Transformants were selected on LB10 Tc15 Ap100 agar plates. The complementing plasmid was transferred from E. coli Sm10 into the V. anguillarum mutant by conjugation. Transconjugants were selected by tetracycline resistance (Tc2). The transconjugants were then confirmed by PCR amplification and restriction digestion.
Bacterial conjugation were carried out using the procedure modified from Varina et al.. Briefly, 100 μl V. anguillarum grown overnight was added into 2.5 ml nine salts solution (NSS) ; 100 μl E. coli culture overnight was added into 2.5 ml 10 mM MgSO4. The resulting V. anguillarum and E. coli suspension was mixed, vacuum filtered onto an autoclaved 0.22-μm-pore-diameter nylon membrane (Millipore, USA), placed on an LB15 agar plate (LB-plus-1.5% NaCl), and allowed to incubate overnight at 27°C. Following incubation, the cells were removed from the filter by vigorous vortex mixing in 1 ml NSS. Cell suspensions (70 μl) were spread on LB20 plated with appropriate antibiotics and the plates were incubated at 27°C until V. anguillarum colonies were observed (usually 24 to 48 h).
Cloning, over-expression, purification, and refolding of the Plp protein
The whole length of the plp gene (stop codon not included) was amplified by PCR with a sense primer introducing a BamHI site and an antisense primer introducing BglII site, respectively. Genomic DNA extracted from V. anguillarum M93Sm was used as template. The amplified PCR product was digested with BamHI and BglII, and ligated into a pQE60 (QIAGEN, USA) vector, which was also cut with BamHI and BglII. The ligation mix was transformed into E. coli M15 (pREP4) and clones with pQE60-plp were selected on LB10 agar containing kanamycin and ampicillin. A clone harboring plasmid pQE60-plp was selected and the plasmid DNA sequence isolated from the clone confirmed by sequencing. The clone was designated as S269. Subsequently, E. coli strain S269 was grown at 37°C in 500 ml LB10 broth to OD600 = 0.5, and isopropyl-β-D-thiogalactopyranoside (IPTG) was added to the culture (final concentration, 1 mM) to induce the expression of Plp. Then, the induced E. coli cells grown for 4 h at 37°C were harvested at 8000 × g for 10 min. The cell pellet was stored at −20°C overnight to improve lysis. Inclusion bodies of Plp were crudely purified using Cellytic B reagent (Sigma, USA). Refolding of Plp protein from the inclusion body preparation was carried out using a modification of the method described by Santa et al.. Briefly, 500 μl of purified inclusion body (2 mg protein/ml) was completely solubilized in 1 ml of 50 mM Tris buffer (pH 12) containing 2 M urea. The solubilized Plp was diluted into 20 ml dilution buffer (50 mM Tris–HCl, pH 8.0; 0.2 M glycine; 10% glycerol; 2 M urea; 0.5 mM EDTA, and 0.2 mM DTT) at 4°C. No aggregation was observed during the dilution. The diluted Plp protein was dialyzed with the addition of 500 ml 50 mM Tris–HCl (pH8.0) until the total dialysis volume up to 3 L. The dialyzed Plp protein was concentrated with QIAGEN Ni-NTA Protein Purification Kit (QIAGEN) under native purification condition according to the instructions of the manufacturer. The protein concentration was determined using the BCA protein assay (Pierce).
The hemolytic activity of V. anguillarum strains was measured by two methods. First, single V. anguillarum colonies were transferred onto TSA-sheep blood agar, LB20-sheep blood agar (LB20 agar plus 5% sheep blood with heparin, obtained from Hemostat Laboratories) or LB20-fish blood agar (LB20 agar plus 5% rainbow trout or Atlantic salmon blood with heparin). Hemolytic activity of each colony was determined by measuring hemolytic zone surrounding the colonies after 24 h at 27°C. Additionally, the level of hemolytic activity was also quantitated using a microcentrifuge tube assay. The tubes contained 500 μl 5% erythrocytes (fish or sheep, suspended in 10 mM Tris-Cl, pH 7.5 – 0.9% NaCl buffer) were mixed with 500 μl of bacterial supernatant or rPlp and incubated for 20 h at 27°C. The samples were centrifuged at 1500 × g for 2 min at 4°C, and the optical density of the resulting supernatant was read at 428 nm.
Phospholipase assay and thin-layer chromatography (TLC) analysis
Phospholipase assays were performed in vitro with a BODIPY-phosphatidylcholine (BPC or 2-decanoyl-1-(O-(11-(4,4-difluoro-5,7-dimethyl-4-bora-3a,4a-diaza-s-indacene-3-propionyl)amino)undecyl)-sn-glycero-3-phosphocholine; Invitrogen), NBD-phosphatidylethanolamine (NBD-PE, N-(NBD-Aminododecanoyl)L-1,2-dihexanoyl-sn-glycero-3-phosphoethanolamine; Sigma), NBD-phosphatidylserine (NBD-PS or 1-Palmitoyl-2-[12-[(7-nitro-2-1,3-benzoxadiazol-4-yl)amino]dodecanoyl]-sn-Glycero-3-Phospho-L-Serine; Avanti Polar Lipid), NBD-sphingomyelin (NBD-SM, N-[12-[(7-nitro-2-1,3-benzoxadiazol-4-yl)amino]dodecanoyl]-Sphingosine-1-Phosphocholine; Avanti Polar Lipid). 20 μM phospholipid substrates (10 μl) were reacted with an equal volume (10 μl) of various samples, and incubated at different conditions, as described for each experiment. For some experiments, purified standard phospholipases were used: PLA2 (Sigma) from porcine pancreas, PLC (Sigma) from Clostridium perfringens, and PLD (Sigma) from cabbage. The reaction products were analyzed by thin-layer chromatography (TLC). Briefly, 20 μl of 1-butanol was added to the above reaction mixes (20 μl), followed by vigorous vortex mixing for 30 s and centrifugation (10,000 × g, 1 min). The upper lipid extract layer (5 μl) was loaded onto a plastic-backed silica gel G60 plate without fluorescent indicator (Sigma) and air-dried for 20 min. TLC was performed either with chloroform-methanol–water-acetic acid (45/45/10/1 by vol.) when BODIPY-PC was used as the substrate, or with chloroform-methanol-acetic acid (60/20/1 by vol.) when NBD-PE, NBD-PS, or NBD-SM used as the substrates. For some experiments, an apolar solvent (n-hexane (70): diethyl ether (30): acetic aid (4)) was used. Fluorescence was detected and quantified using a Typhoon 9410 laser scanner.
V. anguillarum cells were fractionated as described previously  and the subcellular location of Plp determined. Briefly, 100 ml NSS-washed overnight grown bacterial cells were resuspended in 10 ml of ultrapure water for 20 min to cause osmotic shock and centrifuged (10,000 × g, 5°C, 10 min) to collect the periplasmic fraction (the supernatant). The remaining pellets were washed twice with ultrapure water and lysed by sonication (four cycles at 35% power for 20 s, then allowed to cool for 1 min). The sonicated cells were centrifuged (10,000 × g, 5°C, 20 min) to remove cell debris and any unlysed cells, and the supernatant cell lysate was separated by ultracentrifugation (200,000 × g, 1 h, 4°C) to yield the cytosolic (supernatant) and membrane (pellet) fractions. The membrane fraction was treated with 1% Sarkosyl to obtain Sarkosyl-soluble (inner membrane) and -insoluble (outer membrane) fractions. Protein concentration in various fractions was measured using BCA protein determination kit (Pierce).
Preparation of polyclonal antibody
Truncated Plp protein was over-expressed and purified to serve as the antigen to create polyclonal antibody against Plp. Briefly, primer Pm212 and Pm213 (listed in Table 3) were used to amplify central portion of the plp gene, which encodes the truncated Plp protein (amino acid 93 to 293). PCR product was ligated into pQE30UA vector (QIAGEN), and transformed into E. coli M15 and transformants were selected on LB10 agar containing kanamycin and ampicillin. Plasmid DNA was purified and the sequence confirmed by DNA sequencing. Protein purification was performed under denaturing conditions according to the instructions of the manufacturer (QIAGEN, USA) and protein purity was determined by SDS-PAGE and Coomassie blue staining. Subsequently, the purified truncated Plp was used as antigen to prepare polyclonal antibody in two New Zealand White rabbits (Charles River Lab, MA). Briefly, 1 ml purified antigen (concentration = 100 μg/ml) was vigorously mixed with 1 ml TiterMax Gold adjuvant (Sigma) into a homogeneous suspension. About 10 ml of blood was withdrawn from the rabbits before immunization as a control. For the first injection, antigen-adjuvant mix was subcutaneously injected at 4 sites (over each shoulder and thigh; 100 μl/site). The rabbits were boosted with single injections of antigen-adjuvant (100 μl) at day 28, 42, and 56. Blood was withdrawn 7–10 days after the 2nd and 3rd boosts to test the titer of antiserum using the western blot analysis. Antiserum with a high titer (> 1: 10,000) was aliquoted and stored at −70°C.
Sodium dodecyl sulfate-polyacrylamide gel electrophoresis (SDS-PAGE) and Western blot analysis
Purified proteins or other protein samples were separated in 10% SDS-polyacrylamide gels. Prestained protein standards (Bio-Rad) and Laemmli sample buffer (Sigma) were used in all gels. Electrophoresis was performed at 100 V for 60–90 min. Gels were stained with either Coomassie blue G-250 or silver stain (Pierce, USA) to visualize the protein bands. Alternatively, proteins were transferred to nitrocellulose membranes for western blot analysis using the mini-Protean II system (Bio-Rad). Protein transfers were performed as described by Towbin et al. at 100 V for 1 h. Nitrocellulose membranes were blocked with the addition of 5% skim milk. Detection of specific protein bands was accomplished by reacting the blot with the 1:5000 diluted anti-Plp antibody, followed by the addition of the secondary antibody goat anti-rabbit IgG conjugated with peroxidase, and then developed by TMB Development Liquid (Sigma, USA).
DNA sequence and analysis
All DNA sequencing was done at the URI Genomics and Sequencing Center (University of Rhode Island, Kingston, RI), using an ABI 3170xl Genetic Analyzer unit (Applied Biosystems). Multiple alignment and phylogenic tree were analyzed using the Clustal-W method in DNA-STAR Lasergene7 program.
Fish infection studies
Various V. anguillarum strains were tested for virulence with rainbow trout (Oncorhynchus mykiss) by intraperitoneal (IP) injection as described by Mou et al.. Briefly, V. anguillarum cells grown in LB20 supplemented with appropriate antibiotics for 22 h at 27°C were harvested by centrifugation (9,000 × g, 5 min, 4°C), washed twice in NSS, and resuspended in NSS (~2 × 109 cells ml-1). Initial cell density was estimated by measurement of optical density at 600 nm. The actual cell density of NSS suspensions was determined by serial dilution and spot plating. All fish were examined prior to the start of each experiment to determine that they were free of disease or injury. Fish were anesthetized with tricaine methanesulfonate (Western Chemical, Ferndale, WA), with 100 mg/L for induction and 52.5 mg/L for maintenance. V. anguillarum strains were IP-injected into fish in 100 μl NSS vehicle. Fish that were between 15 and 25 cm long were injected with bacteria diluted with NSS at various doses or NSS only as negative control. Five fish were used for each experimental group. Fish inoculated with different bacterial strains were maintained in separate 10-gallon tanks with constant water flow (200 ml/min) at 19 ± 1°C. The tanks were separated to prevent possible cross-contamination. Death due to vibriosis was determined by the observation of gross clinical signs and confirmed by the recovery and isolation of V. anguillarum cells resistant to the appropriate antibiotics from the head kidney of dead fish. The presence of the appropriate strains was tested by PCR analysis. Observations were made for 14 days. All fish used in this research project were obtained from the URI East Farm Aquaculture Center. All fish infection protocols were reviewed and approved by the University of Rhode Island Institutional Animal Care and Use Committee (URI IACUC reference number AN06-008-002; protocols renewed 14 January 2013).
This work was supported by the National Research Initiative of the USDA Cooperative State Research, Education, and Extension Service, grant no. 2008-35204-04605, awarded to D.R.N.
This research was based in part upon work conducted using the Rhode Island Genomics Sequencing Center, which is supported in part by the National Science Foundation under EPSCoR grant 0554548.
We thank Dr. Terence Bradley and Ian Jaffe for their generous help and for supplying the rainbow trout used in this research. We thank Shelby Hillman for her assistance with the fish infection experiment.
- Austin B, Austin DA: Bacterial fish pathogens: disease of farmed and wild fish. Praxis Publishing Co. 2012, New York, NY: Springer, FifthGoogle Scholar
- Denkin SM, Nelson DR: Induction of protease activity in Vibrio anguillarum by gastrointestinal mucus. Appl Environ Microbiol. 1999, 65 (8): 3555-3560.PubMedPubMed CentralGoogle Scholar
- Toranzo AE, Barja JL: Virulence factors of bacteria pathogenic for coldwater fish. Annu Rev Fish Dis. 1993, 3: 5-36.View ArticleGoogle Scholar
- Egidius E: Vibriosis: Pathogenicity and pathology. Aquaculture. 1987, 7: 15-28.View ArticleGoogle Scholar
- Denkin SM, Nelson DR: Regulation of Vibrio anguillarum empA metalloprotease expression and its role in virulence. Appl Environ Microbiol. 2004, 70 (7): 4193-4204.PubMedPubMed CentralView ArticleGoogle Scholar
- Garcia T, Otto K, Kjelleberg S, Nelson DR: Growth of Vibrio anguillarum in Salmon Intestinal Mucus. Appl Environ Microbiol. 1997, 63 (3): 1034-1039.PubMedPubMed CentralGoogle Scholar
- Hirono I, Masuda T, Aoki T: Cloning and detection of the hemolysin gene of Vibrio anguillarum. Microb Pathog. 1996, 21 (3): 173-182.PubMedView ArticleGoogle Scholar
- Rock JL, Nelson DR: Identification and characterization of a hemolysin gene cluster in Vibrio anguillarum. Infect Immun. 2006, 74 (5): 2777-2786.PubMedPubMed CentralView ArticleGoogle Scholar
- Li L, Rock JL, Nelson DR: Identification and characterization of a repeat-in-toxin gene cluster in Vibrio anguillarum. Infect Immun. 2008, 76 (6): 2620-2632.PubMedPubMed CentralView ArticleGoogle Scholar
- Di Lorenzo M, Stork M, Tolmasky ME, Actis LA, Farrell D, Welch TJ, Crosa LM, Wertheimer AM, Chen Q, Salinas P, et al: Complete sequence of virulence plasmid pJM1 from the marine fish pathogen Vibrio anguillarum strain 775. J Bacteriol. 2003, 185 (19): 5822-5830.PubMedPubMed CentralView ArticleGoogle Scholar
- Milton DL, O'Toole R, Horstedt P, Wolf-Watz H: Flagellin A is essential for the virulence of Vibrio anguillarum. J Bacteriol. 1996, 178 (5): 1310-1319.PubMedPubMed CentralGoogle Scholar
- Daugherty S, Low MG: Cloning, expression, and mutagenesis of phosphatidylinositol-specific phospholipase C from Staphylococcus aureus: a potential staphylococcal virulence factor. Infect Immun. 1993, 61 (12): 5078-5089.PubMedPubMed CentralGoogle Scholar
- Gish W, States DJ: Identification of protein coding regions by database similarity search. Nat Genet. 1993, 3 (3): 266-272.PubMedView ArticleGoogle Scholar
- Flieger A, Neumeister B, Cianciotto NP: Characterization of the gene encoding the major secreted lysophospholipase A of Legionella pneumophila and its role in detoxification of lysophosphatidylcholine. Infect Immun. 2002, 70 (11): 6094-6106.PubMedPubMed CentralView ArticleGoogle Scholar
- Flieger A, Rydzewski K, Banerji S, Broich M, Heuner K: Cloning and characterization of the gene encoding the major cell-associated phospholipase A of Legionella pneumophila, plaB, exhibiting hemolytic activity. Infect Immun. 2004, 72 (5): 2648-2658.PubMedPubMed CentralView ArticleGoogle Scholar
- Molgaard A, Kauppinen S, Larsen S: Rhamnogalacturonan acetylesterase elucidates the structure and function of a new family of hydrolases. Structure. 2000, 8 (4): 373-383.PubMedView ArticleGoogle Scholar
- Li L, Mou X, Nelson DR: HlyU is a positive regulator of hemolysin expression in Vibrio anguillarum. J Bacteriol. 2011, 193 (18): 4779-4789.PubMedPubMed CentralView ArticleGoogle Scholar
- Petersen TN, Brunak S, von Heijne G, Nielsen H: SignalP 4.0: discriminating signal peptides from transmembrane regions. Nature methods. 2011, 8 (10): 785-786.PubMedView ArticleGoogle Scholar
- Lee KK, Raynard RS, Ellis AE: The phospholipid composition of Atlantic salmon, Salmo salar L., erythrocyte membranes. J Fish Biol. 1989, 35: 313-314.View ArticleGoogle Scholar
- Nouri-Sorkhabi MH, Agar NS, Sullivan DR, Gallagher C, Kuchel PW: Phospholipid composition of erythrocyte membranes and plasma of mammalian blood including Australian marsupials; quantitative 31P NMR analysis using detergent. Comp Biochem Physiol B Biochem Mol Biol. 1996, 113 (2): 221-227.PubMedView ArticleGoogle Scholar
- Simon R, Priefer U, Pühler A: A broad host range mobilization system for in vivo genetic engineering: transposon mutagenesis in gram negative bacteria. Nat Biotechnol. 1983, 1 (9): 784-791.View ArticleGoogle Scholar
- Mcgee K, Hörstedt P, Milton DL: Identification and characterization of additional flagellin genes from Vibrio anguillarum. J Bacteriol. 1996, 178 (17): 5188-5198.PubMedPubMed CentralGoogle Scholar
- Miwatani T, Takeda Y, Sakurai J, Yoshihara A, Taga S: Effect of heat (Arrhenius effect) on crude hemolysin of Vibrio parahaemolyticus. Infect Immun. 1972, 6 (6): 1031-1033.PubMedPubMed CentralGoogle Scholar
- Miwatani T, Sakurai J, Yoshihara A, Takeda Y: Isolation and partial purification of thermolabile direct hemolysin of Vibrio parahaemolyticus. Biken J. 1972, 15 (2): 61-66.PubMedGoogle Scholar
- Sakurai J, Matsuzaki A, Takeda Y, Miwatani T: Existence of two distinct hemolysins in Vibrio parahaemolyticus. Infect Immun. 1974, 9 (5): 777-780.PubMedPubMed CentralGoogle Scholar
- Shinoda S, Matsuoka H, Tsuchie T, Miyoshi S, Yamamoto S, Taniguchi H, Mizuguchi Y: Purification and characterization of a lecithin-dependent haemolysin from Escherichia coli transformed by a Vibrio parahaemolyticus gene. J Gen Microbiol. 1991, 137 (12): 2705-2711.PubMedView ArticleGoogle Scholar
- Fiore AE, Michalski JM, Russell RG, Sears CL, Kaper JB: Cloning, characterization, and chromosomal mapping of a phospholipase (lecithinase) produced by Vibrio cholerae. Infect Immun. 1997, 65 (8): 3112-3117.PubMedPubMed CentralGoogle Scholar
- Lee JH, Ahn SH, Kim SH, Choi YH, Park KJ, Kong IS: Characterization of Vibrio mimicus phospholipase A (PhlA) and cytotoxicity on fish cell. Biochem Biophys Res Commun. 2002, 298 (2): 269-276.PubMedView ArticleGoogle Scholar
- Zhong Y, Zhang XH, Chen J, Chi Z, Sun B, Li Y, Austin B: Overexpression, purification, characterization, and pathogenicity of Vibrio harveyi hemolysin VHH. Infect Immun. 2006, 74 (10): 6001-6005.PubMedPubMed CentralView ArticleGoogle Scholar
- Akoh CC, Lee GC, Liaw YC, Huang TH, Shaw JF: GDSL family of serine esterases/lipases. Prog Lipid Res. 2004, 43 (6): 534-552.PubMedView ArticleGoogle Scholar
- Sun B, Zhang XH, Tang X, Wang S, Zhong Y, Chen J, Austin B: A single residue change in Vibrio harveyi hemolysin results in the loss of phospholipase and hemolytic activities and pathogenicity for turbot (Scophthalmus maximus). J Bacteriol. 2007, 189 (6): 2575-2579.PubMedPubMed CentralView ArticleGoogle Scholar
- Merino S, Aguilar A, Nogueras MM, Regue M, Swift S, Tomas JM: Cloning, sequencing, and role in virulence of two phospholipases (A1 and C) from mesophilic Aeromonas sp. serogroup O:34. Infect Immun. 1999, 67 (8): 4008-4013.PubMedPubMed CentralGoogle Scholar
- Banerji S, Aurass P, Flieger A: The manifold phospholipases A of Legionella pneumophila - identification, export, regulation, and their link to bacterial virulence. Int J Med Microbiol. 2008, 298 (3–4): 169-181.PubMedView ArticleGoogle Scholar
- Koo BS, Lee JH, Kim SC, Yoon HY, Kim KA, Kwon KB, Kim HR, Park JW, Park BH: Phospholipase A as a potent virulence factor of Vibrio vulnificus. Int J Mol Med. 2007, 20 (6): 913-918.PubMedGoogle Scholar
- Boyanovsky BB, Webb NR: Biology of secretory phospholipase A2. Cardiovasc Drugs Ther. 2009, 23 (1): 61-72.PubMedView ArticleGoogle Scholar
- Lee KK, Ellis AE: The quantitative relationship of lethality between extracellular protease and extracellular haemolysin of Aeromonas salmonicida in Atlantic salmon (Salmo salar L.). FEMS Microbiol Lett. 1989, 52 (1–2): 127-131.PubMedView ArticleGoogle Scholar
- Mou X, Spinard EJ, Driscoll MV, Zhao W, Nelson DR: H-NS is a Negative Regulator of the Two Hemolysin/Cytotoxin Gene Clusters in Vibrio anguillarum. Infect Immun. 2013, 81 (10): 3566-3576.PubMedPubMed CentralView ArticleGoogle Scholar
- Vaatanen P: Microbiological studies in coastal waters of the Northern Baltic Sea. I. Distribution and abundance of bacteria and yeasts in the Tvarminne area. Walter Andre Nottback Found Sci Rep. 1976, 1: 1-58.Google Scholar
- Varina M, Denkin SM, Staroscik AM, Nelson DR: Identification and characterization of Epp, the secreted processing protease for the Vibrio anguillarum EmpA metalloprotease. J Bacteriol. 2008, 190 (20): 6589-6597.PubMedPubMed CentralView ArticleGoogle Scholar
- Mårdén P, Tunlid A, Malmcrona-Friberg K, Odham G, Kjelleberg S: Physiological and morphological changes during short term starvation of marine bacterial islates. Arch Microbiol. 1985, 142 (4): 326-332.View ArticleGoogle Scholar
- Jovel SR, Kumagai T, Danshiitsoodol N, Matoba Y, Nishimura M, Sugiyama M: Purification and characterization of the second Streptomyces phospholipase A2 refolded from an inclusion body. Protein Expr Purif. 2006, 50 (1): 82-88.PubMedView ArticleGoogle Scholar
- Towbin H, Staehelin T, Gordon J: Electrophoretic transfer of proteins from polyacrylamide gels to nitrocellulose sheets: procedure and some applications. Proc Natl Acad Sci U S A. 1979, 76 (9): 4350-4354.PubMedPubMed CentralView ArticleGoogle Scholar
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