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Open Access

Peer-reviewed

Research Article

Acquired Type III Secretion System Determines Environmental Fitness of Epidemic Vibrio parahaemolyticus in the Interaction with Bacterivorous Protists

Abstract

Genome analyses of marine microbial communities have revealed the widespread occurrence of genomic islands (GIs), many of which encode for protein secretion machineries described in the context of bacteria-eukaryote interactions. Yet experimental support for the specific roles of such GIs in aquatic community interactions remains scarce. Here, we test for the contribution of type III secretion systems (T3SS) to the environmental fitness of epidemic Vibrio parahaemolyticus. Comparisons of V. parahaemolyticus wild types and T3SS-defective mutants demonstrate that the T3SS encoded on genome island VPaI-7 (T3SS-2) promotes survival of V. parahaemolyticus in the interaction with diverse protist taxa. Enhanced persistence was found to be due to T3SS-2 mediated cytotoxicity and facultative parasitism of V. parahaemolyticus on coexisting protists. Growth in the presence of bacterivorous protists and the T3SS-2 genotype showed a strong correlation across environmental and clinical isolates of V. parahaemolyticus. Short-term microcosm experiments provide evidence that protistan hosts facilitate the invasion of T3SS-2 positive V. parahaemolyticus into a coastal plankton community, and that water temperature and productivity further promote enhanced survival of T3SS-2 positive V. parahaemolyticus. This study is the first to describe the fitness advantage of GI-encoded functions in a microbial food web, which may provide a mechanistic explanation for the global spread and the seasonal dynamics of V. parahaemolyticus pathotypes, including the pandemic serotype cluster O3:K6, in aquatic environments.

Citation: Matz C, Nouri B, McCarter L, Martinez-Urtaza J (2011) Acquired Type III Secretion System Determines Environmental Fitness of Epidemic Vibrio parahaemolyticus in the Interaction with Bacterivorous Protists. PLoS ONE 6(5): e20275. https://doi.org/10.1371/journal.pone.0020275

Editor: Ching-Hong Yang, University of Wisconsin-Milwaukee, United States of America

Received: December 10, 2010; Accepted: April 28, 2011; Published: May 23, 2011

Copyright: © 2011 Matz et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.

Funding: Work supporting the construction of the T3SS-2 mutants in LM5674 was supported by The University of Iowa Carver College of Medicine Initiative Grant (to Linda McCarter). This work was supported by the German Science Foundation (DFG) grant Ma 2491/4-1 (to Carsten Matz) and by the Spanish Ministry of Science and Innovation grant CGL2009-10488 (to Jaime Martinez-Urtaza). The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.

Competing interests: The authors have declared that no competing interests exist.

Introduction

Horizontal gene transfer and the acquisition of foreign DNA is a fundamental process in the ecology and evolution of most bacterial species. Analysis of the increasing number of bacterial genome sequences has revealed considerable genomic variation among closely related strains, which is concentrated in mobile genetic elements, the genome islands (GIs) [1], [2]. GIs have been classified based on the different functions they encode, which include metabolic islands, degradation islands, resistance islands, symbiosis islands, and pathogenicity islands [3], [4]. The acquisition of GIs allows bacteria to instantly obtain a range of genetic traits that may increase fitness under different environmental conditions. The cyanobacterium Prochlorococcus and γ-proteobacteria of the genus Vibrio have become important models for the study of island genes, dynamics of genome diversity and niche partitioning in the marine environment [5], [6]. Despite initial convincing evidence for the adaptive significance of island genes among environmental bacteria, the precise functions of their products have rarely been characterized and their potential role in the evolution of independent bacterial lineages remains poorly understood.

Vibrio parahaemolyticus is a ubiquitous member of natural bacterioplankton communities in marine and estuarine environments [7], [8]. With one of the largest Vibrio genomes [9], V. parahaemolyticus is likely one of the most ecologically versatile. While many isolates of V. parahaemolyticus are considered non-pathogenic, infections among marine wildlife and humans have increased globally in the last years leading to the bacterium's classification as a newly emerging pathogen [10], [11], [12]. In 1996 the first appearance of a pandemic clone of V. parahaemolyticus occurred, a new O3:K6 serotype strain that has now been identified worldwide as the major cause of acute seafood-borne gastroenteritis [13], [14], [15], [16]. Genome sequence analyses show that there is considerable genomic flux in this species and that the new highly virulent clone arose from an O3:K6 isolate that acquired at least seven novel V. parahaemolyticus island regions (VPaI-1 to 7) [9], [17], [18]. Among these genome islands, VPaI-7 (VPA1312–VPA1396), an 81 kb region present on chromosome II, is considered the most relevant for pathogenicity to humans as it locates an additional set of type III secretion system genes (T3SS-2) and two copies of tdh genes encoding the thermostable direct hemolysin TDH [19]. Both sets of genes are key virulence factors in human gastroenteritis causing cytotoxicity and enterotoxicity, respectively [20], [21]. The occurrence of VPaI-7 in environmental strains suggests that T3SS-2 is not exclusively linked to enterotoxicity in humans but also contributes to the fitness and pandemic spread of V. parahaemolyticus pathotypes in marine environments [14], [11], [22]. The rapid global dissemination and recurring epidemics of V. parahaemolyticus raise the question as to whether VPaI-7 encoded T3SS-2 and TDH contribute to the environmental fitness of V. parahaemolyticus epidemic pathotypes.

As members of the natural bacterioplankton community, Vibrio spp. are an integral part of marine plankton communities. Like V. cholerae, V. parahaemolyticus has been found to associate with plankton organisms and suspended particulates as well as to be free-living in water [23], [24]. While chitinous zooplankton may primarily serve as recombination niche and transmission vehicle [25], [26], [27], protist populations appear to be hotspots of dissolved organic matter (DOM) supplemented growth or responsible for grazing-driven suppression and selection [28], [29], [30]. Hence, life of V. parahaemolyticus in association with auto- and heterotrophic protists suggests the possibility that the protein secretion machinery encoded on genome island VPaI-7 may bear specific functions in the interaction with aquatic protists.

In an initial effort to determine the potential roles of VPaI-7 encoded phenotypes in planktonic food webs, we conducted laboratory experiments in which wildtype strains and mutants defective in VPaI-7 encoded phenotypes were exposed to a range of bacterivorous protists. Specifically, we tested the contribution of T3SS-2 to fitness parameters relevant for the seasonal accumulation and global dissemination of V. parahaemolyticus, such as bacterial growth, persistence and invasion of microbial communities.

Materials and Methods

Organisms and culture conditions

The V. parahaemolyticus strains and mutants used in this study are listed in Table 1. The pre-1995 wild type LM5312 originates from coastal waters off Bangladesh (Robert Belas, personal communication), and the post-1995 wild type RIMD2210633 had been isolated during a gastroenteritis epidemic in Japan [31]. In addition, twenty-seven V. parahaemolyticus isolates were included in this analysis, eleven from environmental and sixteen from clinical sources (Table S1). These isolates were collected from Asia, Europe, South America, and the United States between 1951 and 2005, six of which belong to the pandemic pathotype O3:K6. Strains were routinely grown in Luria-Bertani (LB) broth with 3% NaCl or on equivalent agar plates and, prior to the experiments, in 40% artificial seawater (ASW) containing 10% LB broth.

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Table 1. Bacterial strains.

https://doi.org/10.1371/journal.pone.0020275.t001

The protists used in this study were marine and freshwater representatives of three common taxonomic groups: the flagellates Cafeteria roenbergensis, Rhynchomonas nasuta and Ochromonas sp., the ciliates Tetrahymena sp. and Strombidium sp., and the amoebae Acanthamoeba castellanii ATCC 30234 and Dictyostelium discoideum. Cultures of R. nasuta, C. roenbergensis, Ochromonas sp., Tetrahymena sp., A. castellanii and D. discoideum were axenic and maintained as described previously [32], [29], [33]. For all experiments, protists were taken from 5-day-old stock cultures.

Construction of deletion mutants of V. parahaemolyticus

Deletion mutants with defects in T3SS-1 and T3SS-2 were made in V. parahaemolyticus LM5674. LM5674 was derived from BB22 [34]; it contains an 85-bp deletion in the upstream and N-terminal coding region of opaR (ΔopaR1) [35]. Deletion-insertion mutations were introduced into each of the T3SS genes encoding the EscR-type orthologs to make Δvp1672::Camr (418 bp deletion) and Δvpa1342::Kanr (263 bp deletion). The mutations were constructed on V. parahaemolyticus-derived cosmids carrying T3SS genes by using a λ Red recombinase system in Escherichia coli [36]. The deletion-insertion constructs were then conjugated into V. parahaemolyticus and subsequently transferred to the chromosome of strain LM5674 by allelic exchange [37]. The allelic replacements were confirmed by Southern blot analysis.

Grazing and cytotoxicity experiments

Experiments testing the survival of V. parahaemolyticus in the presence of bacterivorous protists were performed in 24-well tissue culture plates. Overnight cultures of the V. parahaemolyticus strains were diluted to 106 cells mL−1 in 40% ASW, transferred into tissue culture plates and incubated at room temperature with moderate shaking. Subsequently, protists were added at a final concentration of 1×103 cells mL−1. Numbers of flagellates and bacteria were followed over seven days. Generally each treatment was run in replicate wells of four.

Plankton community experiment

A surface water sample (0–0.5 m) was collected from the Baltic Sea (Dahme Pier, Germany) in August 2007 with a thoroughly rinsed and autoclaved 5-L polycarbonate bottle (Nalgene). The water was stored at in situ temperature until filtration. Water was filtered through pre-rinsed glass-fibre filters with a nominal pore size of 1.0 mm (Whatman GF/C). For the microcosm experiment, 450 mL of filtered seawater was distributed into each of eight acid-cleaned 500-mL glass flasks. The protist-free treatment received seawater, which was first passed through a 0.8-µm pore-size membrane filter to remove nano- and microplankton while retaining the natural bacterial community. Prior to the experiments, a loopful of each V. parahaemolyticus strain was suspended in 150 mL of 40% ASW amended with 0.1% (wt/vol) tryptone and incubated at room temperature (23±1°C) overnight. Cells were then harvested by centrifugation and the remaining pellet was suspended in 40% ASW. This washing process was repeated four times in order to prevent the carryover of medium nutrients. Finally, the pellet was suspended in 40% ASW for subsequent inoculation of microcosm flasks.

Protist-free microcosm and protist microcosm were amended with either V. parahaemolyticus T3SS-2 positive RIMD2210633 or T3SS-2 negative POR3. V. parahaemolyticus was added to an average initial concentration of 105 cells mL−1. Each of the four different treatments was performed in duplicate, yielding a total of eight experimental microcosms. Additional controls contained only the natural plankton community. Microcosms were incubated for five days at 22±1°C (under ambient laboratory light conditions) and moderate mixing on a rotary shaker. Each microcosm was sampled daily for direct cell counts of immunofluorescent V. parahaemolyticus and photoautrophic and heterotrophic protists.

Temperature and productivity experiment

To study the effect of elevated temperature and productivity on the outcome of Vibrio-protist interactions, we exposed the T3SS-positive V. parahaemolyticus RIMD2210633 and the T3SS-negative mutant POR3 to the thermo- and osmotolerant ciliate T. pyriformis. Cocultures of V. parahaemolyticus and T. pyriformis were incubated in 24-well tissue culture plates containing 40% ASW, with initial bacteria and protist concentrations of 1×105 cells mL−1 and 1×103 cells mL−1, respectively. Temperature treatments were supplemented with 2 mg tryptone mL−1 and were incubated at 16, 23 and 30°C, respectively. Productivity effects were tested by adding tryptone to a final concentration of 2, 10, and 20 mg mL−1, respectively and were incubated at 23°C. Each treatment was run in replicate wells of four for 5 days.

Detection of tdh and T3SS genes

Polymerase chain reaction assays were performed to test for the presence of T3SS-2 positive V. parahaemolyticus in coastal bacterioplankton samples. After enrichment in alkaline peptone water (1% (wt/vol) peptone, 1% (wt/vol) NaCl; pH 8.2), seawater aliquots showing bacterial growth were analyzed by PCR targeting tdh and T3SS-2 genes. Primers and amplification conditions were those reported previously [38], [39].

Enumeration of bacteria and protists

Numbers of V. parahaemolyticus and protists were determined by means of epifluorescence microscopy by using the nonspecific DNA-stain DAPI after adding 4% glutaraldehyde to each well to get a final concentration of 2%. In the plankton community experiment, V. parahaemolyticus was detected by immunofluorescence microscopy employing mouse polyclonal antiserum (BioGenes, Berlin, Germany) that was raised against strain RIMD2210633 and a Cy3-conjugated goat anti-mouse immunoglobulin G (Jackson ImmunoResearch Laboratories) [32]. In all experiments, cell densities of V. parahaemolyticus were also assessed by plating serial dilutions on LB and TCBS agar.

Virulotyping of V. parahaemolyticus isolates

We determined the pathogenic potential of eleven environmental and sixteen clinical isolates of V. parahaemolyticus (Table S1) by analysing bacterial growth on amoeba-seeded agar plates [40]. Briefly, six-day-old cultures of A. castellanii were harvested by centrifugation (500 g, 5 min) and resuspended in 40% ASW to give a final concentration of 2×106 cells mL−1. Seeded agar plates were prepared by spreading 1.5 mL of the amoeba concentrate onto LB agar and allowed to dry for 1–2 h in a biohazard hood. Stationary-phase cultures of V. parahaemolyticus strains were adjusted to an identical OD600 and serially diluted in 96-well microtiter dish. Approximately 3 µL of each dilution step were spotted onto amoeba-seeded agar plates by using a 96-pin replicator. Agar plates were prepared in replicates of four and incubated for four days at 22°C. Minimum survival concentrations were determined for each V. parahaemolyticus strain from the highest dilution of V. parahaemolyticus that gives rise to robust colonies in the presence of A. castellanii.

Statistical analysis

Changes in bacterial and protist numbers over time were tested for significance with repeated measures ANOVA. Survival percentages were arcsine-square root transformed. Pairwise comparisons of means were done by Student's t-tests.

Results

Genome island VPaI-7 promotes survival of V. parahaemolyticus in the interaction with marine protist

Protists can function as microbial predators, competitors or hosts, and thus play important roles in the adaptation and evolution of aquatic bacteria. We studied the contribution of genome island VPaI-7, which encodes the accessory type III secretion system T3SS-2 and the temperature-dependent hemolysin TDH, to growth and survival of V. parahaemolyticus in the presence of the marine nanoflagellate C. roenbergensis. We compared two marine isolates of V. parahaemolyticus (VPaI-7 negative strain PM220 and VPaI-7 positive LM5674) with the pandemic strain RIMD2210633 harboring VPaI-7. VPaI-7 mediated effects were tested by using isogenic mutants of V. parahaemolyticus LM5674 and RIMD2210633 (Table 1).

Cell suspensions of the VPaI-7 negative strain PM220, which represents the dominant genotype in marine environments, were rapidly eliminated and supported growth of the nanoflagellate C. roenbergensis (Figure 1). Abundances of the VPaI-7 positive environmental strain LM5674, however, remained stable in the three days of co-culture (Figure 1A). Successful survival of LM5674 coincided with a more than 85% reduction of flagellate cell numbers indicating protist-targeting cytotoxicity (Figure 1B). By contrast, the T3SS-2 defective mutant LM7026 was rapidly reduced by 80%, which also resulted in increasing numbers of C. roenbergensis relative to initial flagellate numbers. Notably, survival and cytotoxicity of the isogenic T3SS-1 mutant LM7035 were comparable to the effects observed for the wild-type strain LM5674 (P>0.05).

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Figure 1. Accessory type III secretion system promotes survival of V. parahaemolyticus.

Cell suspensions of environmental (filled bars) and clinical strains (open bars) of V. parahaemolyticus were co-cultured with the marine flagellate C. roenbergensis. Bacterial (A) and flagellate (B) survival are given as relative change of initial cell numbers after 24 h of co-incubation of C. roenbergensis with V. parahaemolyticus strains: the environmental isolates PM220 (tdh−/T3SS-2−) and LM5674 (tdh+/T3SS-2+) versus mutants defective in T3SS-2 (LM7026) and T3SS-1 (LM7035); and the clinical isolate RIMD2210633 (tdh+/T3SS-2+) versus mutants defective in TDH (POR1), T3SS-1 (POR2) and T3SS-2 (POR3). Error bars represent standard deviations (n = 4).

https://doi.org/10.1371/journal.pone.0020275.g001

Similar observations were made for the post-1995 clinical isolate RIMD2210633 and derived mutants. The tdhAS double-deletion mutant POR1 showed significantly lower bacterial survival and significantly higher flagellate survival compared to the wild type (both P<0.001). POR2, carrying an additional deletion in vcrD1 encoding an inner membrane protein of the T3SS-1, showed no significant change on bacterial and flagellate survival rates relative to the tdhAS double-deletion mutant POR1 (both P>0.05). While the cytotoxicity of T3SS-1 defective mutant was indistinguishable from that of the parent strain, the T3SS-2 defective mutant POR3, carrying a deletion in vcrD2, showed the most significant decrease in cytotoxicity (P<0.001). Besides the significantly stronger effect of T3SS-2 relative to the T3SS-1 (P<0.001), the strain comparison revealed that the temperature-dependent hemolysin TDH contributed to the survival of V. parahaemolyticus. Consistent for both the environmental and the clinical isolates, genome island VPaI-7 encoding a functional T3SS-2 and the temperature-dependent hemolysin TDH is a key determinant of cytotoxicity and survival for V. parahaemolyticus in the presence of the marine protist C. roenbergensis.

Prey-to-parasite lifestyle switch of V. parahaemolyticus mediated by the accessory type III secretion system

To study potential longer-term effects of T3SS-2 mediated cytotoxicity in Vibrio-protist interactions, we followed bacterial and flagellate cell numbers over a one-week-period by employing immunofluorescence microscopy. In treatments containing the T3SS-2 defective mutant POR3, V. parahaemolyticus was effectively reduced by C. roenbergensis below a concentration of 104 cells mL−1 (Figure 2A). By contrast, populations of the T3SS-2 positive wild type RIMD2210633 remained unaffected due to the instant lysis of C. roenbergensis (Figure 2B). Direct cell counts revealed that upon the lytic break-down of C. roenbergensis populations V. parahaemolyticus increased significantly by about 3-fold relative to the initial cell number (P<0.001). CFU-based abundances of V. parahaemolyticus confirmed this finding as these numbers increased to the same extent (data not shown). Both datasets suggest that T3SS-2 positive V. parahaemolyticus is capable of killing protists and growing on the cell lysate, thus acting as facultative parasite for protist populations.

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Figure 2. Prey-parasite lifestyle switch of V. parahaemolyticus as mediated by the accessory type III secretion system.

Cell suspensions of the T3SS-2 deficient mutant POR3 (A) and the T3SS-2 positive wild type RIMD2210633 (B) were exposed to the flagellate C. roenbergensis. Flagellate numbers include only structurally intact cells and are given as means ± standard deviation (n = 4).

https://doi.org/10.1371/journal.pone.0020275.g002

T3SS-2 elicits cytotoxicity towards broad range of protist taxa

In natural microbial communities V. parahaemolyticus encounters a wide range of protist taxa, which raises the question as to how specific and effective T3SS-2 elicited pathogenicity is to different protistan hosts. We exposed seven protists representing major taxonomic phyla to suspensions of the T3SS-2 positive wild type RIMD2210633 and the T3SS-2 defective mutant POR3. The T3SS-2 positive wild type revealed acute cytotoxicity towards all seven protists tested (Table 2), resulting in a rapid decline in protist cell numbers within 48 h. Species-specific LT50 values, describing the time needed to kill 50% of the initial protist population, indicated the highest sensitivity of the three nanoflagellates C. roenbergensis, R. nasuta and Ochromonas sp. Protist numbers on the T3SS-2 defective mutant POR3, however, multiplied at rates comparable to those of C. roenbergensis depicted in Fig. 2A. By not considering LT50 values of Strombidium sp. due to the non-axenic state of the protist culture, we found a significant negative correlation between protist-specific susceptibility to the T3SS-2 positive wild type RIMD2210633 and protist cell size (R2 = 0.96, P<0.001).

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Table 2. Susceptibility of diverse protist taxa to V. parahaemolyticus RIMD2210633.

https://doi.org/10.1371/journal.pone.0020275.t002

Strain-specific fitness of V. parahaemolyticus correlates with T3SS-2 and tdh genotype

Based on our finding of T3SS-2 mediated survival in V. parahaemolyticus LM5674 and RIMD2210633, we extended our examinations to a total of 27 strains isolated from across the globe. These isolates included eleven environmental and sixteen clinical V. parahaemolyticus strains, six of which belong to the pandemic pathotype O3:K6 (Table S1). By using the amoeba-seeded agar plate assay, we analysed growth of V. parahaemolyticus strains in the presence of the amoeba A. castellanii. Stationary-phase cultures of V. parahaemolyticus strains were spotted in tenfold serial dilutions onto amoebae-seeded agar plates. Minimum survival concentrations were determined for each strain from the lowest cell concentration of V. parahaemolyticus to form robust colonies in the presence of A. castellanii.

Bacterial concentrations growing to robust colonies varied from 101 to 106 cells µL−1 (Figure 3). Strain-specific minimum survival concentrations were found to correlate with the presence/absence of TDH and T3SS-2 genes. Strains containing T3SS-2 had minimum survival concentrations as low as 101 to 102 cells µL−1, indicating that low cell densities are sufficient to grow and survive in the presence of A. castellanii. The highest cell densities to survive amoebal grazing were required by strains harboring neither T3SS-2 nor TDH genes; their minimum survival concentrations ranged from 105 to 106 cells µL−1. Strains containing tdh genes but the VPaI-8 encoded T3SS-trh instead of the T3SS-2 had minimum survival concentrations ranging from 102 to 104 cells µL−1. These findings are in full support of the data reported from our wild type versus mutant experiments as shown above.

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Figure 3. Antipredator effects correlate with T3SS-2 and TDH genotype in environmental and clinical strains of V. parahaemolyticus.

Minimum survival concentrations of 27 strains of V. parahaemolyticus were calculated from the minimum bacterial concentration to form robust colony forming units on amoeba-seeded agar plates. Error bars indicate standard deviations of three repeated experiments.

https://doi.org/10.1371/journal.pone.0020275.g003

Invasion of T3SS-2 positive V. parahaemolyticus into coastal plankton

Epidemiological and biogeographical data indicate that T3SS-2 positive strains of V. parahaemolyticus have undergone a rapid global dissemination across marine and brackish habitats. To assess the contribution of T3SS-2 to the capacity of V. parahaemolyticus to invade local plankton communities, we added T3SS-2 positive wild type and T3SS-2 negative mutant to microcosms containing a naïve coastal plankton assemblage. PCR targeting tdh and T3SS-2 genes as well as immunofluorescence microscopy of plankton samples prior to the experiment revealed that the plankton community was free of T3SS-2 positive and immuno-positive V. parahaemolyticus, respectively.

Treatments containing natural protist communities were compared with protist-free bacterioplankton treatments. In protist-free bacterioplankton (−PROT), populations of T3SS-2 positive wild type and T3SS-2 negative mutant decreased by about 10% over a five-day-period without significant differences between wild type and mutant (Figure 4A). In the presence of heterotrophic and photoautotrophic protists (+PROT), T3SS-2 negative V. parahaemolyticus showed a population decline by about 100-fold and was not able to establish V. parahaemolyticus populations at detectable densities. At the same time protists abundances increased from 1.7 to 3.2×103 cells mL−1 (Figure 4B). Plankton communities inoculated with T3SS-2 positive V. parahaemolyticus were characterized by a stable V. parahaemolyticus population despite the presence of heterotrophic protists. However, numbers of heterotrophic and photoautotrophic protists in these treatments dropped by 59%, which coincided with an increase of T3SS-2 positive V. parahaemolyticus by 20% at day 5 (P<0.001, Figure 4A). These data confirm the cytotoxicity towards protists as described above and suggest a high capacity of the T3SS-2 positive genotype for biological invasion of natural plankton communities by using photoautotrophic and heterotrophic protist as facultative hosts.

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Figure 4. Invasion of T3SS-2 positive V. parahaemolyticus into coastal plankton community.

Microcosms containing natural plankton communities were inoculated with the T3SS-2 positive wild type RIMD2210633 and the T3SS-2 deficient mutant POR3. (A) Survival of V. parahaemolyticus is given as relative change of initial cell numbers in the presence (+PROT) and absence (−PROT) of the natural protist community. (B) relative changes in total protist numbers are given for the protist microcosms. Error bars represent standard deviations (n = 4).

https://doi.org/10.1371/journal.pone.0020275.g004

Temperature and productivity promote selective enrichment of T3SS-2 positive V. parahaemolyticus

Based on the fact that water temperature and eutrophication control Vibrio population dynamics in the field, we used the thermo- and osmotolerant ciliate T. pyriformis to study the effect of elevated temperature and nutrient richness on the outcome of Vibrio-protist interactions. Temperature was found to have no effect on maximum population densities of V. parahaemolyticus in the absence of T. pyriformis (Figure 5A). Both T3SS-2 positive wild type and T3SS-2 negative mutant performed equally well by responding to increased temperatures at similar rates (P>0.05). The presence of the ciliate T. pyriformis promoted growth of T3SS-2 positive relative to T3SS-2 negative V. parahaemolyticus (Figure 5C). However, maximum cell densities of T3SS-2 positive V. parahaemolyticus increased steadily from 16 to 30°C while growth of the T3SS-2 negative strain remained suppressed by the ciliate grazer. These significant temperature effects suggest population dynamics that are based on temperature-dependent growth or virulence of T3SS-2 positive V. parahaemolyticus and/or temperature-dependent clearance rates of T. pyriformis.

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Figure 5. Effects of temperature and productivity on selective enrichment of T3SS-2 positive V. parahaemolyticus.

Maximum bacterial abundances of the T3SS-2 positive wild type RIMD2210633 and the T3SS-2 deficient mutant POR3 were determined in the absence (open symbols) and the presence (closed symbols) of the ciliate T. pyriformis. Temperature effects (A and C) were tested using media containing 2 mg tryptone ml−1; productivity effects were examined at 23°C. Error bars represent standard deviations (n = 4).

https://doi.org/10.1371/journal.pone.0020275.g005

Similar to increasing temperature, elevated nutrient concentrations in the absence of T. pyriformis did not reveal significant differences between the maximum population densities of T3SS-2 positive and T3SS-2 negative V. parahaemolyticus (Figure 5B, P>0.05); tryptone enrichment resulted in increasing population densities for both strains. Ciliate grazing suppressed population growth of the T3SS-2 negative mutant completely while population densities of the T3SS-2 positive wild type were not negatively affected (Figure 5D). Interestingly, population densities of T3SS-2 positive V. parahaemolyticus did not show a significant increase from the intermediate to the highest productivity level (P>0.05). Taken together, fitness of V. parahaemolyticus in the presence of protists not only is strictly dependent upon T3SS-2 but further enhanced by elevated temperatures and productivity levels.

Discussion

As environmental pathogens like V. parahaemolyticus are integral members of natural microbial communities, it is anticipated that some virulence factors studied in the context of human disease may have their functional origin in the interaction with coexisting eukaryotes. Toxins secreted by the V. parahaemolyticus T3SS are suspected to have profound effects on the progression and severity of gastroenteritis in humans [20], [21], [41]. Yet the pressures driving evolution of these toxins have been unclear, because humans are predominantly an accidental host of V. parahaemolyticus. The present findings suggest that the natural targets of one of the bacterium's T3SS may be environmental protists.

Our experiments demonstrate that the T3SS encoded on genome island VPaI-7 confers V. parahaemolyticus with a fitness advantage in the interaction with aquatic protists. T3SS are found in a wide range of γ-proteobacteria, especially in animal and plant pathogens or symbionts [42], [43]. Although the function of the T3SS as a generalized protein translocation apparatus is conserved in pathogens and mutualists, the precise role of any given T3SS is defined by the effector proteins that are translocated to the eukaryotic host cell. Our recent studies on the opportunistic pathogen Pseudomonas aeruginosa revealed that T3SS can play a central role in bacteria–protist interactions [44]. Studying co-cultures of P. aeruginosa and the amoeba A. castellanii, we found that P. aeruginosa rapidly colonized and killed coexisting amoebae. Analysis of the amoeba-induced transcriptome of P. aeruginosa indicated the expression of T3SS genes upon direct contact with amoebae. A comparison of mutants with specific defects in the T3SS demonstrated the use of the secretion apparatus and the effectors ExoU, ExoS, and ExoT in the killing process, in which ExoU had the greatest impact.

Some effector proteins secreted by V. parahaemolyticus T3SS-2 have recently been identified. VopA/P (VPA1346) is an acetyltransferase that inhibits ATP binding by acetylating the catalytic loop of mitogen-activated protein kinase kinases and shares about 55% similarity with the YopJ-like proteins from Yersinia and Salmonella [45]. VopC (VPA1321) is homologous to Escherichia coli cytotoxic necrotizing factor (38% identity) [46]. VopL (VPA1370) induces formation of actin stress fibers and manipulates actin assembly of HeLa cells [47]. VopT (VPA1327) has ADP-ribosyltransferase (ADPRT) activity and is partially involved in the cytotoxicity observed with Caco-2 cells [46]. Interestingly, VopT shows approximately 45% and 44% identity with the ADPRT domain of ExoT and ExoS of P. aeruginosa, respectively. ExoT and ExoS produced by P. aeruginosa both inactivating Rho family GTPases via GAP activity and are bifunctional proteins capable of interfering with other host signalling molecules via ADP ribosylation. In future experiments, we will elucidate the specific roles of T3SS-2 effector proteins in the cellular interaction of V. parahaemolyticus with marine protists.

In contrast to T3SS-2, homologues of the TTSS-1 genes are present in all V. parahaemolyticus strains examined as well as in some other Vibrio species, such as V. harveyi, V. alginolyticus, and V. tubiashii [21]. Although T3SS-1 is involved in its cytotoxicity of V. parahaemolyticus strain RIMD2210633 to HeLa cells [21], [41], we found that only the accessory T3SS-2 and not the T3SS-1 caused marine protists to lyse. There have been reports of other bacteria that possess two sets of T3SS, such as E. coli, S. enterica and members of the genera Yersinia and Burkholderia [48]. However, except for the case of the T3SSs in Salmonella spp., the differential roles of multiple T3SSs in a single bacterium have not yet been elucidated. In S. enterica, the first set of T3SS, SPI-1, mediates enterocyte invasion while SPI-2 influences survival within macrophages [48]. As we found no indication for the contribution of T3SS-1 to the fitness of V. parahaemolyticus strains interacting with a wide range of protist taxa, we propose that T3SS-1 may bear functions in the interaction with other marine eukaryotes.

A recent study on co-cultures of V. parahaemolyticus and the amoeba A. castellanii found no indication that survival of V. parahaemolyticus in the presence of amoebae is dependent on T3SS, TDH and quorum sensing [49]. However, the use of nutrient rich media (PYG; ATCC medium 712) rather than the marine minimal media used in the present study as well as the use of plate counts in combination with long-term incubation of 10–35 days may have lead to the contrasting results of the study by Laskowski-Arce and Orth. It could be that the experimental setup concealed cytotoxicity and that cryptic grazing and concomitant recycling of growth limiting nutrients contributed to the long-term survival of V. parahaemolyticus.

Like V. cholerae, V. parahaemolyticus is found in the free-living state as well as in association with particles. In a recent study on the interaction of V. cholerae with marine nanoflagellates we reported that biofilms are the protective niche enabling V. cholerae to survive protozoan grazing while their planktonic bacteria are eliminated [29], [50]. Grazing on planktonic V. cholerae was found to select for the biofilm-enhancing rugose variant, which is adapted to the surface-associated niche by the production of VPS exopolymers. Grazing resistance of V. cholerae biofilms was attained by exopolymer production and by the quorum sensing dependent secretion of antiprotozoal factors that inhibit protozoan feeding activity. Although the biofilm forming capacity of V. parahaemolyticus is well documented [35], we found no indication for biofilm-enhanced persistence or cytotoxicity of V. parahaemolyticus in the interaction with marine protists (Nouri et al., unpublished data). Rather, our preliminary data indicate that T3SS-mediated cytotoxicity towards protists is reduced in biofilm-enhancing opaque variants of V. parahaemolyticus and is increased in opaR quorum sensing mutants.

A limited population of V. parahaemolyticus is capable of causing human diseases such as acute gastroenteritis. Almost all of the clinical V. parahaemolyticus isolates exhibit the Kanagawa phenomenon, a beta-type hemolysis on a special blood agar, and this phenomenon is caused by the thermostable direct hemolysin (TDH) [51]. Although a variety of V. parahaemolyticus serovars can cause human diseases, O3:K6 and a few other serotypes (O4:K68, O1:K25, and O1:KUT) have caused an increasing number of worldwide outbreaks of gastroenteritis since 1996 and are referred to as pandemic clonal group [52], [53], [11]. The prevalence of T3SS-2 positive and TDH positive genotypes among these pandemic clones and their isolation from both clinical and environmental samples suggest their involvement in environmental persistence and dissemination of V. parahaemolyticus. Our data show that T3SS-2 positive strains grow and persist better than T3SS-2 negative strains in the presence of environmental protists. The contribution of TDH is less clear. Although we found a small but significant difference of the tdhAS double-deletion mutant in co-culture with the nanoflagellate C. roenbergensis, plankton microcosm experiments of increased complexity did not show a significant effect of the tdh genotype for V. parahaemolyticus environmental invasiveness and persistence (data not shown).

An important factor for the global dissemination across marine environments is the organism's ability to invade local plankton communities. In microcosm experiments, we could demonstrate that T3SS-2 positive V. parahaemolyticus is able to invade coastal microbial communities faster by benefiting from protists as facultative hosts. Declines observed in the number of photoautrophic and heterotrophic protists suggest that both functional guilds are targeted by the V. parahaemolyticus T3SS-2. Studies from other bacteria interacting with higher eukaryotes suggest that T3SS target both animals and plant host cells [42], [43]. More mechanistic studies with representatives of marine phytoplankton are needed to unravel potential similarities of effector proteins and cytotoxicity between phototrophs and heterotrophs. Nevertheless, the present study illustrates the adaptive advantage of V. parahaemolyticus carrying the T3SS-2 encoding genome island VpaI-7. Global transportation via ballast water and aquaculture are thought to have driven the rapid dissemination of T3SS-2 and TDH positive V. parahaemolyticus pathotypes like the pandemic clone O3:K6 [11], [22]. Our experiments suggest that T3SS-2 positive V. parahaemolyticus, although underrepresented in coastal bacterioplankton communities, could persist and become periodically enriched when interacting with pelagic protists.

Cholera outbreaks are temporally related to phytoplankton blooms and have been hypothesized to result from enhanced availability of dissolved organic matter (DOM) for bacterial growth [54], [55]. Environmental surveys have demonstrated that massive increases in phytoplankton biomass (i.e. phytoplankton blooms) can result in enhanced growth of V. cholerae [28], [30]. In our experiments, artificial nutrient enrichment in combination with protist populations favored growth of T3SS-2 positive V. parahaemolyticus. In situ tracking of V. parahaemolyticus in mesocosm studies of increasing complexity should give better insight into processes and interactions in natural communities. Notably, T3SS-2 in V. parahaemolyticus shows similarity to the T3SS present in several pathogenic V. cholerae non-O1 and non-O139 isolates [56], which can cause gastroenteritis in humans. It will be interesting to test for the active roles of V. cholerae and other Vibrio spp. in the decline of phytoplankton populations and DOM release.

One hallmark in the ecology and epidemiology of pathogenic Vibrio spp. is the increased prevalence during warm summer months. The current model for the seasonal occurrence of cholera epidemics involves a number of abiotic factors favoring V. cholerae growth (e.g. temperature, pH, salinity, DOM) [55], [57]. The progressive spread of V. parahaemolyticus and its colonization of new areas has been related to an unusual increase in seawater temperatures in coastal zones [8]. A key issue in the epidemiology of V. parahaemolyticus is whether the emergence of O3:K6 isolates and their serovariants is the consequence of the effects of global warming. Several of the reported outbreaks, especially during the period 1996 to 1998, have been ascribed to elevated environmental temperatures and the El Nino phenomenon [10], [58], [59]. Our data indicate that increased water temperature as found in coastal waters accelerates the selective enrichment of T3SS-positive genotypes in the presence of aquatic protists.

Although much remains to be discovered, our results introduce the direct interaction of V. parahaemolyticus with aquatic protists as the functional context for eukaryote-targeting protein secretion machineries encoded on the pathogenicity island VPaI-7 and identify bacterial facultative parasitism as a mechanism that ensures the persistence and accumulation of V. parahaemolyticus in aquatic environments. We propose that Vibrio-protist interactions contribute to the selective enrichment of T3SS-2 positive V. parahaemolyticus, which may have important implications for seasonal population dynamics and the evolution of pathogenic clones. Recently, Persson et al. reported on the widespread occurrence of gene homologues of virulence-associated protein secretion machineries in a phylogenetically diverse set of genome sequenced marine bacteria and in the Global Ocean Sampling metagenomic databases [60]. Our experiments raise the question of how common and sophisticated facultative parasitism on protist populations is in aquatic bacteria – an interaction that may shape adaptation and biogeochemical fluxes in microbial food webs more than we currently appreciate.

Acknowledgments

We thank Tetsuya Iida (Osaka University) for supplying the POR strains and Michael Steinert (Technical University Braunschweig) for providing original cultures of amoebae, and Christian Erck for supplying polyclonal antibodies.

Author Contributions

Conceived and designed the experiments: CM. Performed the experiments: CM BN. Analyzed the data: CM JM-U. Contributed reagents/materials/analysis tools: LM JM-U. Wrote the paper: CM LM JM-U. Conceived and designed the experiments: CM. Performed the experiments: CM BN. Analyzed the data: CM JM-U. Contributed reagents/materials/analysis tools: LM JM-U. Wrote the paper: CM LM JM-U.

References

  1. 1. Joyce EA, Chan K, Salama NR, Falkow S (2002) Redefining bacterial populations: a post-genomic reformation. Nat Rev Genet 3: 462–473.
  2. 2. Thompson JR, Pacocha S, Pharino C, Klepac-Ceraj V, Hunt DE, et al. (2005) Genotypic diversity within a natural coastal bacterioplankton population. Science 307: 1311–1313.
  3. 3. Dobrindt U, Hochhut B, Hentschel U, Hacker J (2004) Genomic islands in pathogenic and environmental microorganisms. Nat Rev Microbiol 2: 414–424.
  4. 4. Hacker J, Kaper JB (2000) Pathogenicity islands and the evolution of microbes. Annu Rev Microbiol 54: 641–679.
  5. 5. Coleman ML, Sullivan MB, Martiny AC, Steglich C, Barry K, et al. (2006) Genomic islands and the ecology and evolution of Prochlorococcus. Science 311: 1768–1770.
  6. 6. Hunt DE, David LA, Gevers D, Preheim SP, Alm EJ, et al. (2008) Resource partitioning and sympatric differentiation among closely related bacterioplankton. Science 320: 1081–1085.
  7. 7. McCarter LL (1999) The multiple identities of Vibrio parahaemolyticus. J Mol Microbiol Biotechnol 1: 51–57.
  8. 8. Baker-Austin C, Stockley L, Rangdale R, Martinez-Urtaza J (2010) Environmental occurrence and clinical impact of Vibrio vulnificus and Vibrio parahaemolyticus: a European perspective. Environ Microbiol Rep 2: 7–18.
  9. 9. Makino K, Oshima K, Kurokawa K, Yokoyama K, Uda T, et al. (2003) Genome sequence of Vibrio parahaemolyticus: a pathogenic mechanism distinct from that of V. cholerae. Lancet 361: 743–749.
  10. 10. Daniels NA, MacKinnon L, Bishop R, Altekruse S, Ray B, et al. (2000) Vibrio parahaemolyticus infections in the United States, 1973–1998. J Infect Dis 181: 1661–1666.
  11. 11. Nair GB, Ramamurthy T, Bhattacharya SK, Dutta B, Takeda Y, et al. (2007) Global dissemination of Vibrio parahaemolyticus serotype O3:K6 and its serovariants. Clin Microbiol Rev 20: 39–48.
  12. 12. Burek KA, Gulland FMD, O'Hara TM (2008) Effects of climate change on Arctic marine mammal health. Ecol Appl 18: S126–S134.
  13. 13. Chowdhury NR, Chakraborty S, Ramamurthy T, Nishibuchi M, Yamasaki S, et al. (2000) Molecular evidence of clonal Vibrio parahaemolyticus pandemic strains. Emerg Infect Dis 6: 631–636.
  14. 14. Yeung PS, Boor KJ (2004) Epidemiology, pathogenesis, and prevention of foodborne Vibrio parahaemolyticus infections. Foodborne Pathog Dis 1: 74–88.
  15. 15. Martinez-Urtaza J, Simental L, Velasco D, DePaola A, Ishibashi M, et al. (2005) Pandemic Vibrio parahaemolyticus O3:K6, Europe. Emerg Infect Dis 11: 1319–1320.
  16. 16. Cabello FC, Espejo RT, Hernandez MC, Rioseco ML, Ulloa J, et al. (2007) Vibrio parahaemolyticus O3:K6 epidemic diarrhea, Chile, 2005. Emerg Infect Dis 13: 655–656.
  17. 17. Boyd EF, Cohen AL, Naughton LM, Ussery DW, Binnewies TT, et al. (2008) Molecular analysis of the emergence of pandemic Vibrio parahaemolyticus. BMC Microbiol 8: 110.
  18. 18. Han H, Wong HC, Kan B, Guo Z, Zeng X, et al. (2008) Genome plasticity of Vibrio parahaemolyticus: microevolution of the ‘pandemic group’. BMC Genomics 9: 570.
  19. 19. Izutsu K, Kurokawa K, Tashiro K, Kuhara S, Hayashi T, et al. (2008) Comparative genomic analysis using microarray demonstrates a strong correlation between the presence of the 80-kilobase pathogenicity island and pathogenicity in Kanagawa phenomenon-positive Vibrio parahaemolyticus strains. Infect Immun 76: 1016–1023.
  20. 20. Park KS, Ono T, Rokuda M, Jang MH, Iida T, et al. (2004) Cytotoxicity and enterotoxicity of the thermostable direct hemolysin-deletion mutants of Vibrio parahaemolyticus. Microbiol Immunol 48: 313–318.
  21. 21. Park KS, Ono T, Rokuda M, Jang MH, Okada K, et al. (2004) Functional characterization of two type III secretion systems of Vibrio parahaemolyticus. Infect Immun 72: 6659–6665.
  22. 22. Rodriguez-Castro A, Ansede-Bermejo J, Blanco-Abad V, Varela-Pet J, Garcia-Martin O, et al. (2010) Prevalence and genetic diversity of pathogenic populations of Vibrio parahaemolyticus in coastal waters of Galicia, Spain. Environ Microbiol Rep 2: 58–66.
  23. 23. Kaneko T, Colwell RR (1973) Ecology of Vibrio parahaemolyticus in Chesapeake Bay. J Bacteriol 113: 24–32.
  24. 24. Baffone W, Tarsi R, Pane L, Campana R, Repetto B, et al. (2006) Detection of free-living and plankton-bound vibrios in coastal waters of the Adriatic Sea (Italy) and study of their pathogenicity associated properties. Environ Microbiol 8: 1299–1305.
  25. 25. Heidelberg JF, Heidelberg KB, Colwell RR (2002) Bacteria of the gamma-subclass Proteobacteria associated with zooplankton in Chesapeake Bay. Appl Environ Microbiol 68: 5498–5507.
  26. 26. Meibom KL, Blokesch M, Dolganov NA, Wu CY, Schoolnik GK (2005) Chitin induces natural competence in Vibrio cholerae. Science 310: 1824–1827.
  27. 27. Pruzzo C, Vezzulli L, Colwell RR (2008) Global impact of Vibrio cholerae interactions with chitin. Environ Microbiol 10: 1400–1410.
  28. 28. Mourino-Perez RR, Worden AZ, Azam F (2003) Growth of Vibrio cholerae O1 in the red tide waters off California. Appl Environ Microbiol 69: 6923–6931.
  29. 29. Matz C, McDougald D, Moreno AM, Yung PY, Yildiz FH, et al. (2005) Biofilm formation and phenotypic variation enhance predation-driven persistence of Vibrio cholerae. Proc Natl Acad Sci USA 102: 16819–16824.
  30. 30. Worden AZ, Seidel M, Smriga S, Wick A, Malfatti F, et al. (2006) Trophic regulation of Vibrio cholerae in coastal marine waters. Environ Microbiol 8: 21–29.
  31. 31. Nasu H, Iida T, Sugahara T, Yamaichi Y, Park KS, et al. (2000) A filamentous phage associated with recent pandemic Vibrio parahaemolyticus O3:K6 strains. J Clin Microbiol 38: 2156–2161.
  32. 32. Matz C, Jürgens K (2001) Effects of hydrophobic and electrostatic cell surface properties of bacteria on feeding rates of heterotrophic nanoflagellates. Appl Environ Microbiol 67: 814–820.
  33. 33. Weitere M, Bergfeld T, Rice SA, Matz C, Kjelleberg S (2005) Grazing resistance of Pseudomonas aeruginosa biofilms depends on type of protective mechanism, developmental stage and protozoan feeding mode. Environ Microbiol 7: 1593–1601.
  34. 34. Belas R, Simon M, Silverman M (1986) Regulation of lateral flagella gene transcription in Vibrio parahaemolyticus. J Bacteriol 167: 210–218.
  35. 35. Enos-Berlage JL, Guvener ZT, Keenan CE, McCarter LL (2005) Genetic determinants of biofilm development of opaque and translucent Vibrio parahaemolyticus. Mol Microbiol 55: 1160–1182.
  36. 36. Datsenko KA, Wanner BL (2000) One-step inactivation of chromosomal genes in Escherichia coli K-12 using PCR products. Proc Natl Acad Sci USA 97: 6640–6645.
  37. 37. Jaques S, McCarter LL (2006) Three new regulators of swarming in Vibrio parahaemolyticus. J Bacteriol 188: 2625–2635.
  38. 38. Bej AK, Patterson DP, Brasher CW, Vickery MC, Jones DD, et al. (1999) Detection of total and hemolysin-producing Vibrio parahaemolyticus in shellfish using multiplex PCR amplification of tl, tdh and trh. J Microbiol Methods 36: 215–225.
  39. 39. Meador CE, Parsons MM, Bopp CA, Gerner-Smidt P, Painter JA, et al. (2007) Virulence gene– and pandemic group–specific marker profiling of clinical Vibrio parahaemolyticus isolates. J Clin Microbiol 45: 1133–9.
  40. 40. Albers U, Reus K, Shuman HA, Hilbi H (2005) The amoebae plate test implicates a paralogue of lpxB in the interaction of Legionella pneumophila with Acanthamoeba castellanii. Microbiol 151: 167–182.
  41. 41. Ono T, Park KS, Ueta M, Iida T, Honda T (2006) Identification of proteins secreted via Vibrio parahaemolyticus type III secretion system 1. Infect Immun 74: 1032–1042.
  42. 42. Hueck CJ (1998) Type III protein secretion systems in bacterial pathogens of animals and plants. Microbiol Mol Biol Rev 62: 379–433.
  43. 43. Pallen MJ, Wren BW (2007) Bacterial pathogenomics. Nature 449: 835–842.
  44. 44. Matz C, Moreno AM, Alhede M, Manefield M, Hauser AR, et al. (2008) Pseudomonas aeruginosa uses type III secretion system to kill biofilm-associated amoebae. ISME J 2: 843–852.
  45. 45. Trosky JE, Li Y, Mukherjee S, Keitany G, Ball H, et al. (2007) VopA inhibits ATP binding by acetylating the catalytic loop of MAPK kinases. J Biol Chem 282: 34299–34305.
  46. 46. Kodama T, Rokuda M, Park KS, Cantarelli VV, Matsuda S, et al. (2007) Identification and characterization of VopT, a novel ADP-ribosyltransferase effector protein secreted via the Vibrio parahaemolyticus type III secretion system 2. Cell Microbiol 9: 2598–2609.
  47. 47. Liverman AD, Cheng HC, Trosky JE, Leung DW, Yarbrough ML, et al. (2007) Arp2/3-independent assembly of actin by Vibrio type III effector VopL. Proc Natl Acad Sci USA 104: 17117–17122.
  48. 48. Coburn B, Sekirov I, Finlay BB (2007) Type III secretion systems and disease. Clin Microbiol Rev 20: 535–549.
  49. 49. Laskowski-Arce MA, Orth K (2008) Acanthamoeba castellanii promotes the survival of Vibrio parahaemolyticus. Appl Environ Microbiol 74: 7183–7188.
  50. 50. Matz C, Kjelleberg S (2005) Off the hook - how bacteria survive protozoan grazing. Trends Microbiol 13: 302–307.
  51. 51. Honda T, Iida T (1993) The pathogenicity of Vibrio parahaemolyticus and the role of the thermostable direct haemolysin and related haemolysins. Rev Med Microbiol 4: 106–113.
  52. 52. Okuda J, Ishibashi M, Hayakawa E, Nishino T, Takeda Y, et al. (1997) Emergence of a unique O3:K6 clone of Vibrio parahaemolyticus in Calcutta, India, and isolation of strains from the same clonal group from Southeast Asian travelers arriving in Japan. J Clin Microbiol 35: 3150–3155.
  53. 53. Matsumoto C, Okuda J, Ishibashi M, Iwanaga M, Garg P, et al. (2000) Pandemic spread of an O3:K6 clone of Vibrio parahaemolyticus and emergence of related strains evidenced by arbitrarily primed PCR and toxRS sequence analyses. J Clin Microbiol 38: 578–585.
  54. 54. Lobitz B, Beck L, Huq A, Wood B, Fuchs G, et al. (2000) Climate and infectious disease: use of remote sensing for detection of Vibrio cholerae by indirect measurement. Proc Natl Acad Sci USA 97: 1438–1443.
  55. 55. Lipp EK, Huq A, Colwell RR (2002) Effects of global climate on infectious disease: the cholera model. Clin Microbiol Rev 15: 757–770.
  56. 56. Dziejman M, Serruto D, Tam VC, Sturtevant D, Diraphat P, et al. (2005) Genomic characterization of non-O1, non-O139 Vibrio cholerae reveals genes for a type III secretion system. Proc Natl Acad Sci USA 102: 3465–3470.
  57. 57. Constantin de Magny G, Murtugudde R, Sapiano MR, Nizam A, Brown CW, et al. (2008) Environmental signatures associated with cholera epidemics. Proc Natl Acad Sci USA 105: 17676–17681.
  58. 58. McLaughlin JB, DePaola A, Bopp CA, Martinek KA, Napolilli NP, et al. (2005) Outbreak of Vibrio parahaemolyticus gastroenteritis associated with Alaskan oysters. N Engl J Med 353: 1463–1470.
  59. 59. Martinez-Urtaza J, Huapaya B, Gavilan RG, Blanco-Abad V, Ansede-Bermejo J, et al. (2008) Emergence of Asiatic Vibrio diseases in South America in phase with El Niño. Epidemiology 19: 829–837.
  60. 60. Persson OP, Pinhassi J, Riemann L, Marklund BI, Rhen M, et al. (2009) High abundance of virulence gene homologues in marine bacteria. Environ Microbiol 11: 1348–1357.
  61. 61. McCarter LL (1998) OpaR, a homolog of Vibrio harveyi LuxR, controls opacity of Vibrio parahaemolyticus. J Bacteriol 180: 3166–3173.