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Article

Controlled Recirculating Wet Storage Purging V. parahaemolyticus in Oysters

by
Ruojun Mu
1,
Chengchu Liu
2,*,
Salina Parveen
3,
Donald Webster
4 and
Jie Pang
1,*
1
College of Food Science, Fujian Agriculture and Forestry University, Fuzhou 350002, China
2
Sea Grant College Extension Program, University of Maryland Extension and Maryland-Sea Grant Extension, Princess Anne, MD 21853, USA
3
Department of Agriculture, Food and Resource Sciences, University of Maryland Eastern Shore, Princess Anne, MD 21853, USA
4
Wye Research & Education Center, University of Maryland Extension, Queenstown, MD 21658, USA
*
Authors to whom correspondence should be addressed.
Pathogens 2022, 11(5), 553; https://doi.org/10.3390/pathogens11050553
Submission received: 2 March 2022 / Revised: 16 April 2022 / Accepted: 3 May 2022 / Published: 7 May 2022
(This article belongs to the Special Issue Relevant and Recurring Bacterial Pathogens in Aquaculture)
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Abstract

:
This work explored the effects of salinity and temperature on the efficacy of purging V. parahaemolyticus from eastern oysters (Crassostrea virginica). Oysters were inoculated with a 5-strain cocktail of V. parahaemolyticus to levels of 104 to 105 MPN (most probable number)/g and depurated in a controlled re-circulating wet-storage system with artificial seawater (ASW). Both salinity and temperature remarkably affected the efficacy for the depuration of V. parahaemolyticus from oysters during wet-storage. The wet-storage process at salinity 20 ppt at 7.5 °C or 10 °C could achieve a larger than 3 log (MPN/g) reduction of Vibrio at Day 7, which meets the FDA’s requirement as a post-harvest process for V. parahaemolyticus control. At the conditions of 10 °C and 20 ppt, a pre-chilled system could achieve a 3.54 log (MPN/g) reduction of Vibrio in oysters on Day 7. There was no significant difference in the shelf life between inoculated and untreated oysters before the depuration, with a same survival rate (stored in a 4 °C cooler for 15 days) of 93%.

1. Introduction

V. parahaemolyticus is a human pathogen that naturally exists in marine environments [1] and primarily causes seafood-associated gastroenteritis in the U.S., mostly from the consumption of raw oysters [2]. Based on CDC data, Vibrio infections follow a seasonal trend mainly from June to September at high temperatures [3]. Oysters can uptake and accumulate Vibrio from growth environments [4]. Vibrio can also replicate in oysters at favorable temperatures [5]. Therefore, a naturally higher abundance of V. parahaemolyticus (<10,000 [most probable number] MPN/g) can be detected in oysters [6]. It is reported that around 20 million Americans consume raw shellfish [7]. It has been documented that many outbreaks of V. parahaemolyticus infections were related to eating raw oysters in the U.S. since 1973 [8,9].
To increase shellfish safety, the seafood industry employs different strategies intended to reduce or control pathogen levels in oysters [10]. Liu et al. [11] revealed that frozen storage could achieve around 3.52 log (MPN/g) reductions of V. parahaemolyticus in half-shell Pacific oysters. Ma et al. [12] identified and validated a high hydrostatic pressure processing (HPP) method for commercial applications that achieved greater than 3.52-log reductions of V. parahaemolyticus in Pacific oysters. However, both methods lead to the death of the oysters; reducing the Vibrio levels in live oysters is still a challenge. Depuration in UV-sterilized water and electrolyzed oxidizing water was used to solve this problem [13,14]. Irradiations can also reduce the levels of Vibrio while keeping oysters alive [15]. One previous study reported that a wet-storage process (7–15 °C for 5–7 days) could reduce lab-inoculated V. parahaemolyticus in Pacific oysters (Crassostrea gigas) greater than 3.0 log units [16]. However, no information is available on the wet-storage process that is applied in reducing V. parahaemolyticus in eastern oysters (Crassostrea virginica).
In this work, we investigated the effects of salinity and temperature on the efficacy of purging V. parahaemolyticus from eastern oysters (Crassostrea virginica). We inoculated oysters with V. parahaemolyticus to levels of 104 to 105 MPN/g and depurated them in a controlled re-circulating wet-storage system with artificial seawater (ASW). We explored the effects of salinity, temperature, and the system design on the reduction of the Vibrio, as well as the shelf life of the oysters. In this study, we focused on the reduction of V. parahaemolyticus in eastern oysters and applied a new design of the wet-storage system. We hope those will give new insight into the depuration of Vibrio in seafood.

2. Results

2.1. Occurrence and Accumulation of V. parahaemolyticus in Oyster

The occurrence of V. parahaemolyticus levels in oysters was significantly different based on the date of harvest (Table 1). Winter- and early spring-harvested oysters had extremely low levels of V. parahaemolyticus levels (<1 log MPN/g), while summer-harvested oysters showed a significant increase in the occurrence of V. parahaemolyticus levels (about 3 log MPN/g). Based on the results, the inoculation procedure can accumulate V. parahaemolyticus levels to ~5 log MPN/g. Most importantly, this inoculation procedure is not dependent on the background level of V. parahaemolyticus in oysters.

2.2. Effects of Salinities on the Reduction of Vibrio

We firstly explored the effect of salinity on the reduction of Vibrio, controlling the temperature at 10 °C (Table 2). In all three salinity conditions, levels of V. parahaemolyticus were significantly different during the first 2 days, reduced up to 1 log MPN/g (salinity 15 ppt, Day 2). From Day 3, the reduction slowed down to around 0.3 log MPN/g per day. Those results revealed that our wet-storage system had a high deficiency during the first 2 days of the depuration. Depuration of oysters in ASW at 20 ppt resulted in 3.14 log MPN/g of reduction of V. parahaemolyticus in oysters after 7 days, while at 15 and 25 ppt ASW, the reduction only achieved 2.85 and 2.77, respectively.

2.3. Effects of Temperatures on the Reduction of Vibrio

We further explored the effect of temperature on the reduction of Vibrio in 20 ppt ASW, which we had already confirmed is the best salinity for depuration. We chose 3 temperatures to test the changes in the V. parahaemolyticus levels during the 7-day wet-storage process (Table 3). With the temperature decreased, the reduction of the V. parahaemolyticus levels significantly increased. At a temperature of 7.5 °C, the log reduction of the Vibrio achieved a 3.38 log MPN/g, which was the highest value among all trials. The significant increase in the depuration efficiency of the wet-storage was attributed to the low temperature. The levels of V. parahaemolyticus significantly decreased during the first 4 days, which was 2 days longer than all other trials. Detailed reductions (Log10 MPN/g) of V. parahaemolyticus at 7.5 °C, the salinity of 20 ppt is shown in Figure 1.

2.4. Effects of System Pre-Chilling on the Reduction of Vibrio

To get better efficiency of depuration for our wet-storage system, we pre-chilled the water tank before the wet-storage process. Figure 2 illustrates the temperature reduction rate of the wet-storage system. It took about 5 h for the system to decrease the temperature to 10 °C. Figure 3 shows the reductions of V. parahaemolyticus in inoculated oysters during the pre-chilled (black bar) and non-pre-chilled (grey bar) wet-storage processes. The temperature and salinity of the ASW were controlled at 10 °C and 20 ppt. The reduction of the V. parahaemolyticus levels in a pre-chilled wet-storage process significantly increased to 3.54 log MPN/g. This value is 0.82 log MPN/g higher than a non-pre-chilled depuration system. Furthermore, the pre-chill significantly increased the reduction of the V. parahaemolyticus levels on each day of depuration and the reduction rate.

2.5. Shelf Life of the Oyster

A total of three studies (100 oysters per study) were conducted to evaluate the survival rate of oysters in the walk-in cooler after the accumulated treatments (Figure 4). All oysters survived 3 days of refrigerated storage. For oysters after inoculation and without any treatment, only one oyster died on Day 5. All accumulated and non-treated oysters had similar survival rates during 15 days of storage at 4 °C. The survival rate of inoculated, and untreated oysters before depuration are both 93%. These results indicate that accumulated treatments do not affect the shelf life of oysters for depuration.

3. Discussion

To prepare a unified level of Vibrio in original oysters for depuration, we scheduled the inoculation method for the accumulation of Vibrio in oysters. Even when we could detect naturally occurring V. parahaemolyticus in oysters harvested in summer, we still needed inoculation to increase the level to specific levels for our wet-storage depuration test. Our results are mostly consistent with findings from current studies [1,2,17]. Decreases in the level of V. parahaemolyticus were detected in all conditions during the 7-day wet-storage test (Table 2). Depuration of lab-inoculated oysters in ASW for 48 h resulted in a large log reduction of V. parahaemolyticus in oysters from 2 to 4 log MPN/g, based on the temperature and salinity. The results indicated that Vibrio purging rates are higher during the first 2 days. Depuration efficiency at a salinity of 20 ppt was significantly different from that of the other two conditions. The result suggests that appropriate salinity of the ASW during wet-storage is necessary for depuration of the oysters since ours were harvested from aquaculture with a salinity of the water of around 10 ppt based on a previous study [2], a small reduction of Vibrio with a salinity of 10 is likely due to little or no biological activity of oysters occurring in seawater. A higher salinity (20 ppt) of wet-storage may favor the depuration of the oysters. However, the behavior of the oysters may be affected when we increase salinity to 25 ppt. Under this condition, the activity of the oysters may be inhibited; hence, Vibrio may not be depurated effectively. Chae et al. [17] reported that increased reductions of V. parahaemolyticus were observed when oysters were depurated at 15 °C. At low temperatures, the oyster pumps water at the highest level, hence the uptake of Vibrio would be retarded. The temperatures we choose for depuration in our study are all below 15 °C. Based on the results, we found that an optimum wet-storage process could be achieved at a combination of 7.5 °C temperature and 20 ppt salinity, which produced a 3.38 log (MPN/g) reduction after 7 days of depuration (Figure 1). The wet-storage process at 10 °C and salinity 20 ppt could also achieve a larger than 3 log reduction, which meets the FDA’s requirement of larger than a 3.0 log (MPN/g) reduction as a post-harvest process for oyster V. parahaemolyticus control [18]. We also found that the pre-chilling treatment could improve the efficacy of the wet-storage process.
Depuration has been treated as a post-harvest process for decreasing sewage-associated bacteria (such as coliforms, Esherichia coli and Salmonella). It has been widely applied in many countries to remove sewage-associated bacterial contaminants in different shellfish species sold alive [19,20]. However, based on the little effect on reducing V. parahaemolyticus in shellfish, depuration has not yet been practiced in the shellfish industry as a post-harvest treatment for controlling the natural flora of shellfish [14,21,22,23]. Several studies reported the efficacy of depuration in reducing V. parahaemolyticus in Pacific oysters [16,17,18,19]. One study detailed the efficacy of V. parahaemolyticus depuration in oysters [19]. However, there are several differences between our results and this study, especially in the effects of salinity on the first two days. In this study, the log reduction of V. parahaemolyticus in oysters after 1 day reached up to 2.83. In another study [2], their results show a 1.71 and 1.76 log reduction of V. parahaemolyticus in oysters after storage of 1 day at salinities of 20 and 25 ppt, respectively. In a third study [1], the log reduction of V. parahaemolyticus in oysters also reach up to 2.57 at a salinity of 30 ppt. Those results show better efficiency of depuration than our system. The reasons may be as follows: (1) oyster species—the previous studies used Pacific oysters while we used Eastern oysters for the experiments; (2) original environment—there could be differences in the growing water temperature and salinity ranges for the oysters in different studies, which may affect the activation of oysters during wet-storage; (3) upwelling design of the depuration systems—we notice that downwelling system was applied in previous studies, while in our study, we used an upwelling system. In a downwelling system, the purified water was introduced to the system from the upside and may avoid the resuspension of detritus. This may increase the efficiency of the depuration of the system. Future work will investigate in detail the effects of the design of the systems on depuration. We found many factors that affect the efficiency of wet-storage systems, other than on-site salinity, temperature, etc. In this study, we notice a significant difference in depuration efficiency between pre-chilled and non-pre-chilled tank water for Vibrio in oysters. Furthermore, we assume the source of the oysters (farm-raised or wild-caught) and accumulation method (laboratory inoculation or natural accumulation through temperature abuse) may affect the reduction of the Vibrio during wet-storage procedures. In addition, the shelf life of the oysters during and after depuration is another concern of the wet-storage process. Further large-scale research is needed to confirm these findings.

4. Materials and Methods

4.1. V. parahaemolyticus Cultures Preparation

Pathogenic (tlh+, tdh+, and trh+) and non-pathogenic (tlh+, tdh−, and trh−) V. parahaemolyticus strains isolated from clams and oysters were used in this study [24]. Each culture was individually grown in 10 mL tryptic soy broth (TSB, Difco, Becton) supplemented with 1% NaCl (TSB-Salt) at 37 °C for 18 to 24 h. The enriched cultures were streaked to individual tryptic soy agar (TSA, Difco, Becton Dickinson) supplemented with 1% NaCl (TSA-Salt) and incubated at 37 °C for 18 to 24 h. A single colony from a TSA-Salt plate was picked and enriched in 10 mL TSB-Salt at 37 °C for 4 h. The enriched cultures of V. parahaemolyticus were pooled into a 30 mL sterile centrifuge tube and centrifuged at 3000× g (To be checked) for 15 min. Pelleted cells were resuspended in 30 mL of sterile salt solution (1%) to produce a culture cocktail of approximately 4 × 108 CFU/mL.

4.2. Oyster Preparation

Oysters were natural diploid adult eastern oysters sourced from an oyster farm in the Choptank River, MD. Oysters were transported on ice in a cooler to the lab within about 2 h. The oysters, after a brief washing with tap water to remove the mud on the shell, were ready to be inoculated with Vibrio spp. The ASW was prepared by dissolving Instant Ocean Salt (Instant Ocean, United Pet Group, Inc., Cincinnati, OH 45455, USA) in deionized water according to the manufacturer’s instructions.

4.3. Accumulation of V. parahaemolyticus in Oysters

Accumulation of V. parahaemolyticus in oysters was conducted according to previous studies [16,17]. For each depuration study, 150 aquaculture oysters or 75 commercial oysters were transferred to an identical HDPE tank containing 30 L of freshly prepared ASW containing a V. parahaemolyticus culture cocktail at a level of approximately 104 to 105 CFU/mL. The oysters were held in the tank at room temperature overnight (18 h). The salinity during the inoculation was controlled the same as that in the depuration process. Air was pumped into the water to keep dissolved oxygen (DO) levels favorable for oyster pumping and uptake of Vibrio. Levels of aquaculture oysters were analyzed with a 3-tube most probable-number (MPN) method before and after inoculation.

4.4. Oyster Depuration

After inoculation, the oysters were transferred to a laboratory-scale recirculating tank with 150 L of ASW. The system was equipped with an ultraviolet (UV) Lite (Emperor Aquatic smarts, Aqua Logic, Inc, San Diego, CA, USA), a water chiller (Delta Star, Aqua Logic Inc., San Diego, CA, USA), a thermometer, and a flow rate meter (1500 L/h). The temperature of the process was set at 7.5, 10, and 12.5 °C, while salinity was fixed at 15, 20, and 25 ppt. The levels of V. parahaemolyticus in oysters were analyzed every day for 7 days during the depuration process. A total of three studies (100 oysters per study) were conducted to assess the ability of oysters to survive in the refrigerated walk-in cooler (4 °C) after the accumulated treatments.

4.5. Microbiological Analysis

Levels of V. parahaemolyticus in oysters were analyzed with a 3-tube MPN method described in the U.S. Food and Drug Administration’s BAM [25], using thiosulfatecitrate-bile salts-sucrose agar (TCBS) and Chrom-agar for V. parahaemolyticus isolation and confirmation. The accuracy of using CHROM to determine the MPN values was confirmed by BAX PCR. In a preliminary study, we applied BAX PCR in a few cases to confirm isolates recovered from CHROM agar plates. We did not observe any significant differences between the two methods (using Chrom-agar or BAX PCR to confirm presumptive isolates taken in TCBS plates). Therefore, Chrom-agar was used in all tests of V. parahaemolyticus levels.
For each test, 6 oysters were shucked using a sterile knife on a sterile cutting board and blended in a sterile blender jar with an equal weight of sterile phosphate-buffered saline (PBS) at high speed for 90 s to produce a 1:1 shellfish diluent homogenate. To prepare a 1:10 dilution, 1 g of oyster homogenate (1:1) was mixed with 9 mL of PBS. Additional 10-fold dilutions were prepared using PBS (i.e., 1 mL of 1:10 to 9.0 mL of PBS for a 1:100 dilution). One-milliliter portions of all dilutions were individually inoculated into 3 tubes of 10 mL Alkaline Peptone Water (APW). APW tubes were incubated at 37 °C for 16–18 h and the positive (turbid) tubes were recorded. A loopful of each positive APW tube was streaked onto Thiosulfate-Citrate Bile Salt-Sucrose (TCBS) plates and incubated at 37 °C for 18–24 h. All plates that had green colonies were considered presumptive positive for V. parahaemolyticus. Then, three different suspicious colonies in each plate were looped to strike on Chromagar plates [26] and incubated at 37 °C for 18–24 h. All plates that had purple colonies were considered to be Vp positive.

4.6. Statistical Analysis

Results of microbiological tests were analyzed by using SPSS 19.0 software (Chicago, IL, USA). Significant differences among means of each treatment over time were established at a level of p < 0.05. All statistical analyses were based on 3 trials. Samples of each trial were collected from six oysters.

5. Conclusions

The wet-storage process at a combination of 7.5 °C temperature and 20 ppt salinity can achieve a 3.38 log (MPN/g) reduction at Day 7. A pre-chilled system, at the conditions of 10 °C and 20 ppt, can achieve a 3.54 log (MPN/g) reduction of V. parahaemolyticus in oysters at Day 7. There was no significant difference in the shelf life between inoculated and untreated oysters before the depuration, with the same survival rate (stored in a 4 °C cooler for 15 days) of 93%.

Author Contributions

Conceptualization and methodology, C.L., S.P., J.P. and R.M.; software and formal analysis, R.M. and C.L.; investigation, R.M. and C.L.; data curation, S.P. and C.L.; writing—original draft preparation, R.M.; writing—review and editing, R.M., C.L., S.P. and D.W.; supervision, C.L. and J.P.; project administration, C.L., S.P. and J.P.; funding acquisition, C.L. and J.P. All authors have read and agreed to the published version of the manuscript.

Funding

This research was funded by Maryland Agricultural Experiment Station Competitive Grant [MAES2955340], US National Oceanic and Atmospheric Administration (NOAA)-Maryland Sea Grant-Aquaculture Extension Award [NA130ORA4170204], China Scholarship Council (CSC) [201608350088], Natural Science Foundation from Fujian Provincial Department of Science and Technology [2020J01556], and Scientific Research Foundation for Distinguished Young Scientists from Fujian Agriculture and Forestry University [xjq202006].

Institutional Review Board Statement

Not applicable.

Informed Consent Statement

Not applicable.

Data Availability Statement

Not applicable.

Acknowledgments

The authors thank Shannon Hood (University of Maryland Center for Environmental Science and Maryland Sea Grant Extension, respectively) and Andy Lazur (University of Maryland Extension) for providing the and lab supplies and helping review the manuscript. We would also like to thank Joan Meredith (University of Maryland Eastern Shore) for technical assistance.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Su, Y.C.; Yang, Q.; Häse, C. Refrigerated seawater depuration for reducing Vibrio parahaemolyticus contamination in pacific oyster (Crassostrea gigas). J. Food Prot. 2010, 73, 1111–1115. [Google Scholar] [CrossRef] [PubMed]
  2. Phuvasate, S.; Su, Y.C. Impact of water salinity and types of oysters on depuration for reducing Vibrio parahaemolyticus in pacific oysters (Crassostrea gigas). Food Control 2013, 32, 569–573. [Google Scholar] [CrossRef]
  3. Center for Disease Control and Prevention (CDC). 2006. Available online: http://www.cdc.gov/mmwr/preview/mmwrhtml/mm55d807a1.htm (accessed on 18 September 2018).
  4. Jones, J.L.; Lydon, K.A.; Kinsey, T.P.; Friedman, B.; Curtis, M.; Schuster, R. Effects of ambient exposure, refrigeration, and icing on, Vibrio vulnificus, and, Vibrio parahaemolyticus, abundances in oysters. Inter. J. Food Microbiol. 2017, 253, 54–58. [Google Scholar] [CrossRef] [PubMed]
  5. Taylor, M.A.; Yu, J.W.; Howell, T.L.; Jones, S.H. Varying success of relaying to reduce Vibrio parahaemolyticus levels in oysters (Crassostrea virginica). J. Food Prot. 2018, 81, 659–669. [Google Scholar] [CrossRef] [PubMed]
  6. Gooch, J.A.; Depaola, A.; Bowers, J.; Marshall, D.L. Growth and survival of Vibrio parahaemolyticus in postharvest American oysters. J. Food Prot. 2002, 65, 970–974. [Google Scholar] [CrossRef] [PubMed]
  7. Gulnihal, O.; Chintapenta, L.K.; Amy, C.; Kenneth, H. Effects of microbial and heavy metal contaminants on environmental/ecological health and revitalization of coastal ecosystems in Delaware bay. Front. Environ. Sci. 2017, 5, 26. [Google Scholar]
  8. Sonja, O.; Antje, W.; Thomas, M.; Markus, K.; Sarah, R.; Gunnar, G. A polyphasic approach for the differentiation of environmental vibrio isolates from temperate waters. FEMS Microbiol. Ecol. 2015, 1, 145–162. [Google Scholar]
  9. Public Health Agency of Canada. 2015. Available online: http://www.phac-aspc.gc.ca/phn-asp/2015/vibrioparahaemolyticus-eng.php (accessed on 18 September 2018).
  10. Wang, W.; Li, M.; Li, Y. Intervention strategies for reducing Vibrio parahaemolyticus in seafood: A review. J. Food Sci. 2015, 80, 10–19. [Google Scholar] [CrossRef]
  11. Liu, C.; Lu, J.; Su, Y.-C. Effects of flash freezing, followed by frozen storage, on reducing Vibrio parahaemolyticus in pacific raw oysters (Crassostrea gigas). J. Food Prot. 2009, 72, 174–177. [Google Scholar] [CrossRef]
  12. Ma, L.; Su, Y.C. Validation of high pressure processing for inactivating Vibrio parahaemolyticus in pacific oysters (Crassostrea gigas). Int. J. Food Microbiol. 2011, 144, 469–474. [Google Scholar] [CrossRef]
  13. Ramos, R.J.; Miotto, M.; Squella, F.J.L.; Cirolini, A.; Ferreira, J.F.; Vieira, C.R.W. Depuration of oysters (Crassostrea gigas) contaminated with Vibrio parahaemolyticus and Vibrio vulnificus with UV light and chlorinated seawater. J. Food Prot. 2012, 75, 1501. [Google Scholar] [CrossRef] [PubMed]
  14. Ren, T.; Su, Y.C. Effects of electrolyzed oxidizing water treatment on reducing Vibrio parahaemolyticus and Vibrio vulnificus in raw oysters. J. Food Prot. 2006, 69, 1829–1834. [Google Scholar] [CrossRef]
  15. Park, S.Y.; Chung, M.S.; Ha, S.D. Combined effect of sodium hypochlorite and gamma-irradiation for the control of Vibrio vulnificus in fresh oyster and clam. LWT 2018, 91, 568–572. [Google Scholar] [CrossRef]
  16. Phuvasate, S.; Chen, M.H.; Su, Y.C. Reductions of vibrio parahaemolyticus in pacific oysters (Crassostrea gigas) by depuration at various temperatures. Food Microbiol. 2012, 31, 51–56. [Google Scholar] [CrossRef] [Green Version]
  17. Chae, M.J.; Cheney, D.; Su, Y.-C. Temperature Effects on the Depuration of Vibrio parahaemolyticus and Vibrio vulnificus from the American Oyster (Crassostrea virginica). J. Food Sci. 2009, 74, 62–66. [Google Scholar] [CrossRef] [PubMed]
  18. United States Food and Drug Administration. National Shellfish Sanitation Program (NSSP) Guide for the Control of Molluscan Shellfish (2019 Revision). Available online: https://www.fda.gov/media/143238/download (accessed on 10 April 2022).
  19. Su, Y.C.; Liu, C. Vibrio parahaemolyticus: A concern of seafood safety. Food Microbiol. 2007, 24, 549–558. [Google Scholar] [CrossRef] [PubMed]
  20. Shen, X.; Su, Y.C.; Liu, C.; Oscar, T.; Depola, A. Efficacy of Vibrio parahaemolyticus depuration in oysters (Crassostrea gigas). Food Microbiol. 2019, 79, 35–40. [Google Scholar] [CrossRef] [PubMed]
  21. Son, N.T.; Fleet, G.H. Behavior of pathogenic bacteria in the oyster, Crassostrea commercialis, during depuration, re-laying and storage. Appl. Environ. Microbiol. 1980, 40, 994–1002. [Google Scholar] [CrossRef] [Green Version]
  22. Eyles, M.J.; Davey, G.R. Microbiology of commercial depuration of Sydney rock oyster, Crassostrea commercialis. J. Food Prot. 1984, 47, 703–706. [Google Scholar] [CrossRef]
  23. Timoney, J.F.; Abston, A. Accumulation and elimination of Escherichia coli and Salmonella typhimurium by hard clams in an in vitro system. Appl. Environ. Microbiol. 1984, 47, 986–988. [Google Scholar] [CrossRef] [Green Version]
  24. Parveen, S.; Hettiarachchi, K.A.; Bowers, J.C.; Jones, J.L.; Tamplin, M.L.; Mckay, R.; Beatty, W.; Brohawn, K.; Dasilva, L.V.; Depaola, A. Seasonal distribution of total and pathogenic Vibrio parahaemolyticus in chesapeake bay oysters and waters. Int. J. Food Microbiol. 2008, 128, 354–361. [Google Scholar] [CrossRef] [PubMed]
  25. Kaysner, C.A.; De Paola, A., Jr. Vibrio . In FDA Bacteriological Analytical Manual (BAM); 2004. Available online: https://www.fda.gov/Food/FoodScienceResearch/LaboratoryMethods/ucm070830.htm (accessed on 1 December 2021).
  26. Duan, J.; Su, Y.C. Comparison of a chromogenic medium with thiosulfate-citrate-bile salts-sucrose agar for detecting vibrio parahaemolyticus. J. Food Sci. 2005, 70, 125–128. [Google Scholar] [CrossRef]
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Figure 1. Reductions (Log10 MPN/g) of V. parahaemolyticus in lab-inoculated oysters during controlled re-circulating wet-storage process at 7.5 °C, salinity of 20 ppt. Data were collected as mean values of reductions from three trails (sample of each trail from six oysters).
Figure 1. Reductions (Log10 MPN/g) of V. parahaemolyticus in lab-inoculated oysters during controlled re-circulating wet-storage process at 7.5 °C, salinity of 20 ppt. Data were collected as mean values of reductions from three trails (sample of each trail from six oysters).
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Figure 2. Temperature reduction curve of wet-storage system from room temperature to 10 °C.
Figure 2. Temperature reduction curve of wet-storage system from room temperature to 10 °C.
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Figure 3. Reductions (Log10 MPN/g) of V. parahaemolyticus in lab-inoculated oysters during pre-chilled (black bar) and non-pre-chilled (grey bar) wet-storage processes at 10 °C, salinity of 20 ppt. Data were collected as mean values of reductions from three trails (sample of each trail from six oysters).
Figure 3. Reductions (Log10 MPN/g) of V. parahaemolyticus in lab-inoculated oysters during pre-chilled (black bar) and non-pre-chilled (grey bar) wet-storage processes at 10 °C, salinity of 20 ppt. Data were collected as mean values of reductions from three trails (sample of each trail from six oysters).
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Figure 4. Survival of oysters after treatments for controlled re-circulating wet-storage process for 15 days.
Figure 4. Survival of oysters after treatments for controlled re-circulating wet-storage process for 15 days.
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Table
Table 1. V. parahaemolyticus levels (log10 MPN/g) in oysters at different dates of harvest.
Table 1. V. parahaemolyticus levels (log10 MPN/g) in oysters at different dates of harvest.
Vibrio LevelsDate
28 November 201712 December 201710 April 20184 June 20182 July 201831 July 2018
Before inoculation0.54 ± 0.160.45 ± 0.160.36 ± 0.002.44 ± 0.203.04 ± 0.153.31 ± 0.31
After inoculation5.92 ± 0.225.41 ± 0.245.50 ± 0.285.79 ± 0.225.17 ± 0.215.79 ± 0.22
Table
Table 2. Changes of V. parahaemolyticus levels (log10 MPN/g) in lab-inoculated oysters during depuration at salinity of 15, 20, and 25 ppt. (Temperature was controlled at 10 °C).
Table 2. Changes of V. parahaemolyticus levels (log10 MPN/g) in lab-inoculated oysters during depuration at salinity of 15, 20, and 25 ppt. (Temperature was controlled at 10 °C).
Time (Day)Salinity (ppt)
152025
05.18 ± 0.00 A5.50 ± 0.28 A5.41 ± 0.24 A
14.86 ± 0.19 B4.86 ± 0.19 B4.79 ± 0.22 B
23.86 ± 0.19 C3.99 ± 0.37 C4.24 ± 0.12 C
33.65 ± 0.30 CD3.75 ± 0.19 CD3.97 ± 0.00 CD
43.30 ± 0.11 D3.30 ± 0.11 DE3.66 ± 0.00 DE
52.97 ± 0.00 E2.97 ± 0.00 EF3.24 ± 0.24 EF
62.53 ± 0.18 E2.63 ± 0.00 FG2.86 ± 0.19 FG
72.32 ± 0.00 F2.36 ± 0.00 G2.63 ± 0.00 G
Total log reduction2.85 ± 0.00 a3.14 ± 0.00 b2.77 ± 0.12 a
FDA Requirement Achieved (3 log reduction) NoYesYes
Data with the same letter in the same column are not significantly different (p > 0.05).
Table
Table 3. Changes of V. parahaemolyticus levels (log10 MPN/g) in laboratory-inoculated oysters during depuration at 7.5, 10, and 12.5 °C (Salinity was controlled at 20 ppt).
Table 3. Changes of V. parahaemolyticus levels (log10 MPN/g) in laboratory-inoculated oysters during depuration at 7.5, 10, and 12.5 °C (Salinity was controlled at 20 ppt).
Time (Day)Temperature (°C)
7.51012.5
05.79 ± 0.22 A5.50 ± 0.28 A5.47 ± 0.16 A
15.31 ± 0.12 B4.86 ± 0.19 B4.72 ± 0.29 B
24.29 ± 0.11 C3.99 ± 0.37 C4.38 ± 0.00 BC
33.86 ± 0.19 D3.75 ± 0.19 CD3.86 ± 0.28 CD
43.01 ± 0.06 EF3.30 ± 0.11 DE3.65 ± 0.19 DE
52.77 ± 0.12 F2.97 ± 0.00 EF3.57 ± 0.30 DEF
62.57 ± 0.16 F2.63 ± 0.00 FG3.24 ± 0.16 EF
72.41 ± 0.05 F2.36 ± 0.00 G3.04 ± 0.12 F
Total log reduction3.38 ± 0.05 a3.14 ± 0.00 b2.44 ± 0.12 c
FDA Requirement Achieved (3 log reduction) YesYesNo
Data with the same letter in the same column are not significantly different (p > 0.05).
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MDPI and ACS Style

Mu, R.; Liu, C.; Parveen, S.; Webster, D.; Pang, J. Controlled Recirculating Wet Storage Purging V. parahaemolyticus in Oysters. Pathogens 2022, 11, 553. https://doi.org/10.3390/pathogens11050553

AMA Style

Mu R, Liu C, Parveen S, Webster D, Pang J. Controlled Recirculating Wet Storage Purging V. parahaemolyticus in Oysters. Pathogens. 2022; 11(5):553. https://doi.org/10.3390/pathogens11050553

Chicago/Turabian Style

Mu, Ruojun, Chengchu Liu, Salina Parveen, Donald Webster, and Jie Pang. 2022. "Controlled Recirculating Wet Storage Purging V. parahaemolyticus in Oysters" Pathogens 11, no. 5: 553. https://doi.org/10.3390/pathogens11050553

APA Style

Mu, R., Liu, C., Parveen, S., Webster, D., & Pang, J. (2022). Controlled Recirculating Wet Storage Purging V. parahaemolyticus in Oysters. Pathogens, 11(5), 553. https://doi.org/10.3390/pathogens11050553

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