- Research Article
- Open Access
Several strains, one disease: experimental investigation of Vibrio aestuarianus infection parameters in the Pacific oyster, Crassostrea gigas
© The Author(s) 2017
- Received: 13 February 2017
- Accepted: 4 May 2017
- Published: 26 May 2017
This study investigated oyster infection dynamics by different strains of Vibrio aestuarianus isolated before and after the apparent re-emergence of this pathogen observed in France in 2011. We conducted experiments to compare minimal infective dose, lethal dose 50 and bacterial shedding for six V. aestuarianus strains. Whatever the strain used, mortality was induced in juvenile oysters by intramuscular injection and reached 90–100% of mortality within 5 days. Moreover, bacterial shedding was comparable among strains and reached its maximum after 20 h (≈10 EXP5 bacteria/mL/animal). Similarly, our first estimations of lethal dose 50 were comparable among strains (minimal infective dose around 0.4 × 10EXP5 bacteria/mL and LD50 around 10EXP5 bacteria/mL) by using seawater containing freshly shed bacteria. These results indicate that, at least with these criteria, despite V. aestuarianus strains genetic diversity, the disease process is similar. The strains isolated after the apparent re-emergence of the bacteria in 2011, do not present a more acute virulence phenotype than the reference strains isolated between 2002 and 2007. Finally, our study provides original and noteworthy data indicating that infected oysters shed bacteria at a level above the threshold of LD50 a few days before they die, meaning that infection is expected to spread in a susceptible population.
Vibrio aestuarianus is a gamma proteobacterium causing oyster disease in France since 2001 [1–3]. Since 2011, the recent increase in adult oyster mortalities points again to this pathogen as a major concern for aquaculture. This bacterium has thus far been isolated in France, Ireland and Scotland [1, 4, 5] in association with chronic mortalities, and without any reported mortalities in Spain and Italy [6–8]. As other vibrios, V. aestuarianus can colonize different niches and has been isolated episodically from seawater, plankton, sediment and regularly from diseased animals (oysters and fish) [3, 7, 9–11].
Different strains isolated from oysters in the years 2000, all present different virulence degrees (i.e. inducing different levels of oyster mortalities after intramuscular injection) [1, 3]. Genome-based analyses and phylogenetic studies revealed the existence of two clades being equivalent in terms of virulence and of recent/ancient strain distribution. The ecological significance of these two subclasses remains therefore still unknown .
In term of pathology, studies with reference strains (01/032 and 02/041) demonstrated that after injection, V. aestuarianus can be found in the oyster hemolymph, where it inhibits hemocyte adhesion and phagocytosis capacity, and proliferates abundantly [13, 14]. Some virulence factors were identified like the metalloprotease Vam or one regulating gene (varS) [12, 15].
In a more physiological setting, the bacteria can also be transmitted by horizontal waterborne transmission: in cohabitation experiments  or in cohabitation experiments coupling V. aestuarianus with another recognized oyster pathogen, Vibrio tasmaniensis . To render detection and quantification easier, green fluorescent protein (GFP)-tagging of strains can be used ; an approach also used in the current study. All these studies demonstrated that in lab experiments, the bacteria can pass from one animal to another through the seawater.
Even if V. aestuarianus’ ecology and virulence mechanisms are more and more studied, little is known about the infection processes and propagation dynamics inside an oyster population. Many infection parameters such as the minimum infective dose or the bacterial shedding during the pathogenesis are still unknown. In this publication, we developed new experimental protocols to estimate these parameters to better understand V. aestuarianus infection dynamics. Moreover, different strains, isolated before or after the recent re-emergence of the bacteria, will be compared with regard to these characteristics.
Bacteria: growth conditions, detection and quantification
Strains used in this study
2002, Oyster, Brittany, V. aestuarianus subsp. francensis reference strain
2002, Oyster, Brittany, France
2007, Oyster, Brittany, France
2012, Oyster, Charente-Maritime, France
2012, Oyster, Brittany, France
Vibrio aestuarianus DNA quantities in oyster tissues or seawater were estimated by qPCR  after DNA extraction following QiaAmp® tissue kit procedures (Qiagen®) and dilutions for oyster tissue extracts to adjust total DNA concentration to 5 ng/µL. A standard curve was established applying “diluted genomes”.
Briefly, the standard was prepared using the relation between the concentration of DNA in the V. aestuarianus 02/041 and the theoretical number of genomes, calculated on the basis of the DNA mass divided by the genomic molecular weight for V. aestuarianus (2.77 × 109 g/mol, based on a genome size of 4.20 Mbp for V. aestuarianus ). Assays were performed on MX3000P and MX3005P machines (Agilent®) with the Brillant III Ultrafast kit (Stratagene®) following the manufacturer’s instruction. Bacterial concentrations were also estimated by Flow Cytometry (Coulter Epics XL cytometer, Beckman®) on 10 000 events or after 5 min with a threshold fixed on FL1 fluorescence.
Specific pathogen-free oysters
Batches of Pacific oyster Crassostrea gigas were produced in March and April 2013 at the Ifremer hatcheries in Argenton, France and La Tremblade, France, and in April 2015 in La Tremblade. Oysters were kept in experimental facilities from spawning to the experiments described below with UV-treated and filtered seawater and under biosecurity conditions to avoid contamination with major pathogens inducing oyster mortalities: the Ostreid herpesvirus (OsHV-1) and V. aestuarianus. Twelve oysters were screened for the detection of these pathogens by standard protocols [18, 19]. Briefly, after hemolymph sampling in the adductor muscle sinus with a syringe equipped with a needle (0.9 × 25 mm), pieces of 50 mg of mantle and gills were dissected. Dilutions of hemolymph were plated on Zobell agar (10−1, 10−2). DNA from gills and mantle was extracted using a QiAmp® kit. Presence of OsHV-1 and V. aestuarianus DNA was detected by qPCR as described [18, 19].
Bacterial shedding experiments (Additional file 1)
Experiments were performed under static (closed circuit) conditions in aerated seawater maintained at 22 °C during all experiments. Oysters (mean individual weight 12.1 and 13.2 g) were anaesthetized with MgCl2 at a concentration of 50 g/L in tap water. Each oyster was intramuscularly injected with 50–100 µL of a V. aestuarianus suspension and placed into 0.5 L of UV-treated seawater. In a first part, we tested the 02/041-GFP strain at different doses, in two experiments. A total of sixty oysters were placed individually in a beaker (ten oysters for each of the four tested injected doses: 5 × 106, 5 × 107 (tested twice) 1 × 108 and 5 × 108 bacteria/animal). In a second part, the six strains were compared. Three groups containing each 10 animals were infected together with 5 × 108 bacteria/animal in a single tank. Water was daily sampled and bacterial concentrations were estimated by flow cytometry and qPCR as described above. Estimated shedding rates were expressed as Bacteria/mL/oyster/day.
Minimum infectious dose experiments (Additional file 1)
Experiments were performed under static conditions in aerated seawater maintained at 20 °C during all tests. Contaminated seawater was produced by placing 20 injected oysters in 10 L of UV-treated, filtered seawater (intramuscular (IM) injection with 5 × 107 bacteria/animal) for 18 h. Bacterial concentration was checked by flow cytometry for GFP-tagged bacteria and qPCR.
In a first experiment, groups of 30 oysters were immersed in contaminated seawaters in 3 L tanks containing the different strains (six strains) at 5 × 107 bacteria/animal for 24 h before seawater renewal. In a second experiment, oysters were individually exposed in 300 mL beakers to six different dilutions of contaminated seawater produced with 02/041 strain. After 24 h of contact, contaminated seawaters were replaced by fresh UV-treated seawater. Finally, in a third experiment, oysters were individually exposed for 24 h to contaminated seawater containing the different strains (six strains) at different doses (three doses). Control seawater corresponds to seawater collected from tanks with artificial sterile seawater (ASW) injected-oysters. Oysters were monitored daily and dead or moribund animals were removed and frozen for subsequent analysis for the duration of the experiment (15 days). Survivors were sacrificed at the end of the experiment. Individual mantle and gill samples, or whole animals in case of survivors, were tested for the presence of V. aestuarianus DNA.
Differences in cumulated mortalities were compared by Chi squared analysis. Survival data were analyzed using Kaplan–Meier survivor functions and compared using the log-rank test. Kruskal–Wallis tests were applied to assess significant differences between the shedding of the different strains, as a normal distribution was not assumed on log-transformed bacterial concentrations (Shapiro–Wilk test). For all tests, the significance threshold was p < 0.05. All these statistical analyses were gathered using biostaTGV . Finally, the LD50 was estimated from dose effect curves by non-linear regression curve fitting using GraphPad Prism software (San Diego, CA, USA) when enough data were available. For comparison of strains, doses bracketing the LD50 (i.e. inducing more or less than 50% mortalities) were used.
Bacterial shedding experiments
Minimum infectious dose experiments
Induced mortality after 24 h of immersion in seawater contaminated with different concentrations of V. aestuarianus 02/041 on oyster batch 1 (N = 70, individual beakers)
Induced mortality (%)
First day of mortalities
0.3 × 104
0.8 × 104
3 × 104
0.5 × 105
5.1 × 105
7.9 × 105
A lethal dose 50 (LD50), i.e. a dose inducing 50% mortality at the end of the experiment, can be estimated at 1.3 × 105 bacteria/mL [i.e. 5.11 Log(bacteria/mL)] on this oyster batch, after an initial 24 h contamination by immersion in undiluted contaminated seawater at 20 °C (Table 2). Twelve surviving individuals (sampled at day 15, on the 60 initially infected animals) were crushed in their totality before analyses of V. aestuarianus content. In none of them bacterial DNA could be amplified by qPCR even if we cannot exclude the presence of small amounts of DNA with the actual detection limit of our diagnostic tool (1.6 × 102 cells/mL ).
Doses of bacteria (bacteria/mL) in contaminated seawater inducing more or less than 50% of mortality after 24 h of immersion of 10 oysters per condition in individuals beakers (oyster batch 2)
Dose inducing less than 50% mortality
Dose inducing more than 50% mortality
7.5 × 104 − 2.82 × 105
1.27 × 106
6.7 × 104 − 5.75 × 105
1.70 × 106
2.4 × 104 − 3.90 × 105
2.26 × 106
5.3 × 104 − 1.34 × 105
0.61 × 106
1.48 × 106
This study provides first insights into V. aestuarianus infection dynamics by conducting experimental infections to quantify bacterial shedding from infected oysters over time and to determine a minimal infective dose and an LD50. Moreover, the different strains were compared for properties other than and complementary to the classically “rate of mortality after intramuscular injection” .
To investigate bacterial shedding from oysters, animals were intramuscularly injected with different doses of bacteria, to ensure that the animals were synchronously infected with a standardized amount of bacteria. Bacteria released into the surrounding seawater were quantified by qPCR and flow cytometry using a GFP-tagged strain, previously demonstrated as comparable to the wild-type strain in terms of induced mortality. Even if GFP-tagged bacteria allow a real-time monitoring of bacteria in suspension, such tools present a moderate sensitivity, previously estimated for this strain around 103 cells/mL . On the other side, classical qPCR allows the detection of as little as 102 cells/mL  but does not distinguish dead bacteria from living ones. By combining these tools, a quick shedding was observed leading to detection, as soon as 1 h post infection of bacteria reaching 103 to 105 cells/mL/animal depending on the injected dose.
Progressive accumulation of bacteria was observed in each tank, reaching a plateau after 24 h for the highest dose and 50 h for the lowest one. It is noticeable that animal death was not observed until 50 h, which corresponds to the time limit of detection. These results are consistent with other models, in which moribund animals are well-known as important shedders, via thus far still unknown mechanisms. For instance, in the Aeromonas salmonicida–Salmo salar model, release of bacteria from morbid animals was estimated in the order of 105 to 108 cfu/fish/h . For the bacteria Vibrio harveyi infecting the abalone Haliotis tuberculata, bacterial shedding was estimated around 104 bacteria/abalone/mL .
Even if V. aestuarianus strains can present genetic diversity, our results suggest that the disease process is similar: comparison of the release of and the impact of different strains isolated in 2002 and 2012, and belonging to clade A or B  did not show noticeable difference. Similar shedding characteristics were observed in the different strains. No remarkable difference of bacterial shedding for the strains from clade A (12/016 or 02/041) or clade B (12/063, 02/092), and no changes in induced mortalities of sentinel oysters could be detected. In all moribund oysters, large amounts of V. aestuarianus were observed after hemolymph plating (more than 107 bacteria/mL), confirming the colonization and multiplication of the pathogen inside the animal.
Cohabitation protocols and immersion protocols in the presence of sediment were already described for this bacterium [11, 17]. However, in our experiments, cohabitation and contamination with cultured bacteria appeared less reproducible (Travers, pers. comm.) than experimental infections with oyster-shedded bacteria, as if the passage through the host homogenized or induced bacterial infectivity. Similarly, studies of the interaction of Vibrio vulnificus with eels suggest that host cell contact is required for its pathogenicity .
This protocol was chosen to estimate bacterial minimal infective doses and LD50s as it most closely mimics natural exposure to a pathogen . Infections, duplicated in time, with different doses of shedded bacteria were performed either on ten separated individuals (10 tanks) or on thirty animals in triplicates (three tanks). With 5 to 8 × 105 bacteria/mL, cumulated mortalities reached in each case 77% in 15 days. However, to limit bacterial exposure to the first 24 h and to avoid potential transmission between animals in a same tank, final LD50 and minimal infective doses were estimated on animals physically separated in ten 0.5 L-tanks. The minimum infective dose required to reliably induce infection after a 24 h immersion period in contaminated seawater, was estimated at 0.4 × 105 bacteria/mL and the LD50 around 105 bacteria/mL. Comparison of the doses inducing 50% of mortality on two oyster batches revealed some differences (for the 02/041 strain) even if oysters were comparable in term of age and size. Genetic background, as well as life history traits can influence oysters sensitivity to pathogens (e.g. effective infectious dose, and survival [16, 26, 27]). This sensitivity may also be linked to other transmission parameters (e.g. shedding). In absence of standardized oyster lineages, we should thus favor (1) experiments in which all epidemiological parameters are recorded in parallel on the same animals and (2) experiments that are repeated on different oyster batches.
Interestingly, taken together, our results indicate that one contaminated oyster placed into 350 mL of seawater can release 5 to 10 × 105 bacteria/mL in 24 h, and the LD50 was estimated at 1 × 105 bacteria/mL. These findings are very significant for the dynamic of the disease because they indicate that shedding begins at a level already above the LD50 before mortalities occur, meaning that an infected oyster can pass the infection to at least one other oyster, clearly favoring disease-spread in a susceptible population. Additionally, by intramuscular injection with the same bacterial isolate (02/041), as little as 100 bacteria/animal can induce more than 80% mortalities . These data highlight the importance of the initial step in the infection process. Moreover, analyses of surviving individuals revealed the absence of bacteria, which might suggest that these animals were not infected during the 24 h-bath or cleared the infection. This observation may be linked to genetic/physiological specificities of these animals. Even if the heritability for survival of C. gigas, when exposed to V. aestuarianus is low to moderate , oysters selected for their higher resistance to V. aestuarianus infection could constitute a future line of research. The basis of the observed resistance may rely on mechanisms developed by the oysters to prevent the bacteria to enter and/or to multiply. However, more sensitive tools and more targeted screening of tissue are needed to confirm this hypothesis. Future efforts on the comprehension of this crucial initial step are thus necessary. First studies suggested that V. aestuarianus could be found after a few hours in the hemolymph and mantle during cohabitation challenges [17, 21]. However the entry site, the targeted tissues, and the timeline are still unknown.
Vibrio aestuarianus cells are difficult to find and culture from environmental samples. Moreover, only little field data on V. aestuarianus concentrations in oyster environments during epidemics are available. Recent intensive field surveys allowed its isolation from oysters, mussels, plankton, sediments and seawater in France, Spain and Italy [6, 7, 11]. V. aestuarianus can reach 103 to 104 cell/g sediment in warm months [7, 11] and 102 cell/mL in the seawater column in the Adriatic sea. Interestingly, V. aestuarianus can be found associated with plankton where up to 106 bacteria/g were quantified . However, detection protocols  did not allow the discrimination of virulent and non-virulent strains, and thus the importance of the plankton compartment in the effective concentration of virulent V. aestuarianus, and/or its transmission to oysters is still unknown.
Finally, our study demonstrates that virulence classification determined only through injection protocols with high doses of bacteria can be source of debates, leading some authors to consider some strains as pathogens . The V. aestuarianus 07/115 strain, induces high levels of mortality when injected at 5 × 108 bacteria/animal, but does not affect oysters when injected at very low doses (102 bacteria/animal ) or when present in high concentrations in the surrounding water. Future efforts on animal models and infection protocols are certainly needed to clearly define mollusk pathogens.
In conclusion, this study provides new experimentally acquired data on the V. aestuarianus–C. gigas interaction by estimating bacterial shedding and bacterial infective doses. However, more integrative population-based studies are now needed to try to link these first parameter estimations to natural occurring epidemics.
The authors declare that they have no competing interests.
Conception and design: MAT, CL, DT; Acquisition of data: MAT, DT, LP, PH, AKD, MA, LD, MK, or analysis and interpretation of data: MAT, DT, LP, PH, AKD, MK, Manuscript: MAT, MK, LD, CL. All authors read and approved the final manuscript.
Firstly, we acknowledge the anonymous reviewers for their careful reading of our manuscript and constructive comments. We wish to acknowledge Bruno Petton (IFREMER, Lemar) for SPF oyster production. Moreover, the oysters used in this work were produced and maintained in controlled conditions at the IFREMER hatchery in La Tremblade and at the IFREMER nursery in Bouin. We are very grateful to the hatchery and nursery teams for their assistance in oyster production.
This study was supported by the GIGASSAT project funded by ANR-AGROBIOSPHERE (ANR-12-AGRO-0001-01) and by the French Ministries of Ecology and Agriculture through the research program “AESTU” (Convention DPMA 2014-Ifremer).
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