한국패류학회지 (The Korean Journal of Malacology)

한국패류학회 (The Malacological Society of Korea)
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급성 폐사 바지락 (Ruditapes philippinarum) 으로부터 Perkinsus olseni의 확산 기작

Dissemination of Perkinsus olseni is affected by the viability of Ruditapes philippinarum

  • 남기웅 (군산대학교 해양과학대학 해양생명응용과학부 수산생명의학전공) ;
  • 정희도 (국립수산과학원 갯벌연구소) ;
  • 송재희 (국립수산과학원 갯벌연구소) ;
  • 최광식 (제주대학교 해양과학대학 해양의생명과학부 해양생명과학전공) ;
  • 박경일 (군산대학교 해양과학대학 해양생명응용과학부 수산생명의학전공)
  • Nam, Ki-Woong (Department of Aquatic Life Medicine, College of Ocean Science and Technology, Kunsan National University) ;
  • Jeung, Hee-Do (Tidal Flat Research Institute, National Fisheries Research Institute) ;
  • Song, Jae-Hee (Tidal Flat Research Institute, National Fisheries Research Institute) ;
  • Choi, Kwang-Sik (Jeju National University) ;
  • Park, Kyung-Il (Department of Aquatic Life Medicine, College of Ocean Science and Technology, Kunsan National University)
  • 투고 : 2015.11.13
  • 심사 : 2015.12.30
  • 발행 : 2015.12.30
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초록

This study was conducted in order to elucidate the dissemination mechanism of P. olseni using field and laboratory experiments. For this purpose, we quantified the level of P. olseni infection in buried (healthy) and surfaced (gapped) R. philippinarum from a clam bed on Wi-do Island on the west coast of Korea. In addition, the levels of internal and released P. olseni cells from artificially infected (and later dead) R. philippinarum were monitored for 8 days using the RFTM-2 M NaOH lysis method. Our results indicate that P. olseni cells in buried R. philippinarum was $2,655,625{\pm}1,536,936cells/clam$; the level in gapped R. philippinarum was considerably lower, $28,203{\pm}24,889cells/clam$ (p < 0.05). In the laboratory experiment, the P. olseni cells remained in the host tissue 2 days after death was approximately 50% lower than the level of infection measured in living clams. The level dropped to 20% 4 days after death and to 1.5% 6 days after death; eight days after death, P. olseni cells were undetectable since the R. philippinarum flesh had completely decomposed. The level of released cells on the day of death was only 0.05% of the internal level in live R. philippinarum; however, the level increased to 2.3% 5 days after death then gradually decreased and no released cells were detected 8 days after death. Therefore, our laboratory experiment suggest that the low level of P. olseni infection observed in gapped R. philippinarum at Wi-do Island could be caused by lysis of the most of P. olseni cells during the decomposition of dead R. philippinarum tissues. Until the end of decomposition of R. philippinarum, 6.68% of the total amount of P. olseni was released within 8 days. Our study showed that the amount of P. olseni cells from dead host is a considerably higher level than naturally released from healthy R. philippinarum, suggesting that death of the host plays an important role in the dissemination of P. olseni.

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참고문헌

  1. Auzoux-Bordenave, S., Vigario, A.M., Ruano, F., Domart-Coulon, I. and Doumenc, D. (1995) In vitro sporulation of the clam pathogen Perkinsus atlanticus (Apicomplexa, Perkinsea) under various environmental conditions. Journal of Shellfish Research, 14: 469-475.
  2. Bushek, D., Ford S.E. and Chintala, M.M. (2002) Comparison of in vitro-cultured and wild-type Perkinsus marinus. III. Fecal elimination and its role in transmission. Diseases of Aquatic Organisms, 51: 217-225. https://doi.org/10.3354/dao051217
  3. Chu, F.-L., La Peyre, J.F. and Burrenson, C.S. (1993) Perkinsus marinus infection and potential defense related activities in eastern oysters C. virginica: salinity effects. Journal of Invertebrate Pathology, 62: 225-232.
  4. Chung, E.Y., Hur, S.B., Hur, Y.B. and Lee, J.S. (2001) Gonadal maturation and artificial spawning of the Manila clam Ruditapes philippinarum (Bivalvia: Veneridae), in Komso Bay, Korea. Journal of Fisheries Science and Technology, 4: 208-218.
  5. Donaghy, L., Lambert, C., Choi, K.S. and Soudant. P. (2009) Hemocytes of the carpet shell clam (Ruditapes decussatus) and the Manila clam (Ruditapes philippinarum): Current knowledge and future prospects. Aquaculture, 297: 10-24. https://doi.org/10.1016/j.aquaculture.2009.09.003
  6. Eaton, C.D. (2008) Co-evolution. in; Encyclopedia of ecology. (ed. by Sven Erik Jorgensen and Brian D. Fath, 1st Edition). pp. 659-663, Elsevier B.V., Oxford.
  7. Eugenia, R., Pazo, J.P., Garcia, A. and Fernandez Cortes, F. (1992) Reproductive cycle of Manila clam, Ruditapes philippinarum (Adams & Reeve 1850) in ria of Vigo (NW Spain). Scientia Marina, 56(1): 61-67.
  8. Hamaguchi, M.N., Suzuki, N., Usuki, H. and Ishioka, H. (1998) Perkinsus protozoan infection in short-necked clam Tapes (= Ruditapes) philippinarum in Japan. Journal of Fish Pathology, 33: 473-480. https://doi.org/10.3147/jsfp.33.473
  9. Lee, Y.H., Chang, Y.J., Lim, H.K. and Chung, G.S. (1996) Comparison of growth and survival rate in Shortnected clams, Ruditapes philippinarum from different seeding production area. Aquaculture, 9: 223-232.
  10. Mandal, F.B. (2011) Human parasitology. PHI Learning Private Limited, New Delhi.
  11. Moodie, E. (2005) Microsporidia (microsporans). In: Marine parasitology. (ed. by L. Rohde). pp 30-46, CSIRO, Australia.
  12. OIE. (2006) Infection with Perkinsus olseni. In: Manual of diagnostic test for aquatic animals 2006. pp 335-342. OIE. Paris.
  13. Park, K.I. and Choi, K.S. (2001) Spatial distribution of the protozoan parasite Perkinsus sp. found in the Manila clams, Ruditapes philippinarum, in Korea. Aquaculture, 203: 9-22. https://doi.org/10.1016/S0044-8486(01)00619-6
  14. Park, K.-I., Figueras, A. and Choi, K.-S. (2006) Application of enzyme-linked immunosorbent assay(ELISA) for the study of reproduction in the Manila clam, Ruditapes philippinarum: (Mollusca: Bivalvia): II. Impacts of Perkinsus olseni on clam reproduction. Aquaculture, 251: 182-191. https://doi.org/10.1016/j.aquaculture.2005.06.003
  15. Park, K.I, Park, J.K. Lee, J. and Choi, K.S. (2005) Use of molecular markers for species identification of Korean Perkinsus sp. isolated from Manila clam Ruditapes philippinarum. Diseases of Aquatic Organisms, 66: 255-263. https://doi.org/10.3354/dao066255
  16. Park, K.-I., Yang, H.-S., Kang, H.-S., Cho, M., Park, K.-J. and Choi, K.-S. (2010) Isolation and identification of Perkinsus olseni from feces and marine sediment using immunological and molecular techniques. Journal of Invertebrate Pathology, 105: 261-269. https://doi.org/10.1016/j.jip.2010.07.006
  17. Perkins, F.O. (1996) The structure of Perkinsus marinus. (Mackin, Owen, and Collier, 1950) Levine, 1978, with comments on the taxonomy and phylogency of Perkinsus sp. Journal of Shellfish Research, 15: 67-87.
  18. Ragone-Calvo, L.M., Dungan, C.F., Roberson, B.S. and Burreson, E.M. (2003) Systematic evaluation of factors controlling Perkinsus marinus transmission dynamics in lower Chesapeake Bay. Diseases of Aquatic Organisms, 56: 75-86. https://doi.org/10.3354/dao056075
  19. Ray, S.M. (1954) Studies of pathogenesis of Dermocystidium marinum. Proceedings of the National Shellfisheries Association, 45: 164-167.
  20. Song, J.H. (2015) Strategy for the sustainable development of Manila clam farming industry. Aqua Culture, 9: 70-74.
  21. Waki, T., Shimokawa, J., Watanabe, S., Yoshinaga, T. and Ogawa, K. (2012) Experimental challenges of wild Manila clams with Perkinsus species isolated from naturally infected wild Manila clams. Journal of Invertebrate Pathology, 111: 50-55. https://doi.org/10.1016/j.jip.2012.05.009

피인용 문헌

  1. 고창 갯벌에서 중국산 및 충남산 바지락의 성장, 비만도 및 폐사 특성 비교 vol.32, pp.3, 2015, https://doi.org/10.9710/kjm.2016.32.3.175