AJTMH ASTMH Job Mart
HOME HELP FEEDBACK SUBSCRIPTIONS ARCHIVE SEARCH TABLE OF CONTENTS
QUICK SEARCH:   [advanced]


     

Am. J. Trop. Med. Hyg., 69(3), 2003, pp. 260-262
Copyright © 2003 by The American Society of Tropical Medicine and Hygiene

This Article
Right arrow Abstract Freely available
Right arrow Full Text (PDF)
Right arrow Alert me when this article is cited
Right arrow Alert me if a correction is posted
Right arrow Citation Map
Services
Right arrow Similar articles in this journal
Right arrow Similar articles in Web of Science
Right arrow Similar articles in PubMed
Right arrow Alert me to new issues of the journal
Right arrow Download to citation manager
Right arrow reprints & permissions
Citing Articles
Right arrow Citing Articles via HighWire
Right arrow Citing Articles via Web of Science (14)
Right arrow Citing Articles via Google Scholar
Google Scholar
Right arrow Articles by KLENK, K.
Right arrow Articles by KOMAR, N.
Right arrow Search for Related Content
PubMed
Right arrow PubMed Citation
Right arrow Articles by KLENK, K.
Right arrow Articles by KOMAR, N.

POOR REPLICATION OF WEST NILE VIRUS (NEW YORK 1999 STRAIN) IN THREE REPTILIAN AND ONE AMPHIBIAN SPECIES

KACI KLENK AND NICHOLAS KOMAR
Centers for Disease Control and Prevention, Fort Collins, Colorado


ABSTRACT
TOP
 ABSTRACT
INTRODUCTION
 MATERIALS AND METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 
Because West Nile (WN) virus primarily cycles between mosquitoes and birds, North American reptiles and amphibians have not been evaluated as reservoir hosts of this virus. We infected three species of reptiles and one species of amphibian: Iguana iguana (green iguana), Thamnophis sirtalis sirtalis (Florida garter snake), Trachymes scripta elegans (red-ear slider), and Rana catesbeiana (North American bullfrog). After inoculation with WN virus, some of the green iguanas, bullfrogs, and garter snakes showed low but detectable viral loads in the blood, oral or cloacal swabs, and/or organs.


INTRODUCTION
TOP
 ABSTRACT
 INTRODUCTION
MATERIALS AND METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 
West Nile (WN) virus primarily cycles between adult ornithophilic mosquitoes and birds.1,2 This virus was first documented in North America in 1999,3 but involvement of nearctic amphibians and reptiles in the ecology of WN virus is presently unknown. In Russia, WN virus was isolated from a lake frog (Rana ridibunda), and subsequent experiments demonstrated that these frogs develop high-titered viremia capable of infecting biting mosquitoes, suggesting that frogs could be important reservoir hosts for WN virus in Europe.4 However, WN virus studies with North American herpetefauna are lacking.

North American reptiles and amphibians may be competent amplification hosts for WN virus, and play important roles in WN virus transmission. To test this hypothesis, we infected four species of herpetefauna found in North America: Iguana iguana (green iguana), Thamnophis sirtalis sirtalis (Florida garter snake), Trachymes scripta elegans (red-ear slider), and Rana catesbeiana (North American bullfrog). We report on viremia profiles and tissue tropisms for these four species after infection by subcutaneous inoculation, and for green iguanas after mosquito-borne infection.


MATERIALS AND METHODS
TOP
 ABSTRACT
 INTRODUCTION
 MATERIALS AND METHODS
RESULTS
 DISCUSSION
 REFERENCES
 
Virus strains. We used the NY99-4132 strain of WN virus, passaged 3–4 times in Vero cells, that was isolated from crow brain provided by W. Stone (New York State Department of Environmental Conservation, Albany, NY).

Sources of animals and animal care. All animals were acquired through commercial sources, were housed as cohorts of two or three in plastic 58-quart containers with screen lids and had benefit of full-spectrum lighting and heat lamps 12 hours per day. Food and water was provided ad libitum. Species-specific diets were determined following suppliers recommendations or published guidelines.5,6

Mosquitoes and mosquito inoculation. Colonized 7–14-day-old Aedes aegypti DQ (DeQuincey, LA) mosquitoes were inoculated intrathoracically with approximately 0.35 µL of WN virus (containing approximately104.6 plaque-forming units [pfu]). Infected mosquitoes were placed in groups of five inside screened half-pint paper cartons and incubated in a 16:8 hour light:dark photoperiod at 28°C and a relative humidity of 80% for 8–11 days before blood feeding.

West Nile virus infection. We injected study animals with approximately 2,000 pfu of WN virus subcutaneously using a volume of 0.1 mL delivered via 1 mL syringe attached to a 27-gauge subcutaneous needle. Some iguanas were infected by mosquito bite by holding each iguana against a carton containing infected mosquitoes. Each iguana was considered infected when at least one mosquito became engorged.

Specimen collection. Because the animals were small, blood samples were taken from anesthetized animals via cardiocentesis. Sampling individual animals for blood frequently (e.g., daily) was not practical due to the long anesthetic recovery time of ectothermic vertebrates.7 Instead of daily blood sampling, two or three individuals of each species were humanely killed with Beuthanasia-D (Schering-Plough Animal Health, Kenilworth, NJ) (0.1 mL/0.1 kg given intramuscularly) for collection of blood samples each day post-infection (pi) for seven days. Blood (0.2 mL) was sampled via cardiocentesis using a 27-gauge 0.5-inch needle and added to 0.9 mL of BA-1 diluent (Hanks’ M-199 salts, 1% bovine serum albumin, 350 mg/L of sodium bicarbonate, 100 units/mL of penicillin, 100 mg/L of streptomycin, 1 mg/L of Fungizone in 0.05 M Tris, pH 7.6), producing an approximate 1:10 serum dilution. Blood samples were centrifuged at 3,750 rpm for 10 minutes to separate serum from clotted blood, and stored at -70°C.

To obtain oral and cloacal swabs, cotton-tipped applicators were inserted into either the oral cavity or the cloaca of living animals and then placed in 0.5 mL of BA-1 diluent to release any virus. Samples were stored at -70°C.

Two or three individuals of each species were also killed 12–15 days pi. In addition, a group of five needle-inoculated iguanas and one uninfected cage-mate were killed at 28 days pi. Blood samples were obtained from these animals for detection of neutralizing antibodies and organ samples were removed from the carcasses. Six to 10 organ samples (approximately 0.5 cm3 in size) were harvested from each animal. These included heart, kidney, lung, liver, small intestine, gonad, eye, skin, brain, and spleen. Organ samples were ground in 2 mL of BA-1 diluent containing 20% fetal bovine serum, using TenBroeck glass tissue grinders (Bellco Glass, Inc., Vineland, NJ). Each resulting homogenate was transferred to a 1.7-mL Eppendorf (Brinkman Instruments, Westbury, NY) microcentrifuge tube and clarified by microcentrifugation at 7,500 rpm for 2 minutes. Each supernatant was transferred to a cryovial and stored at -70°C. Whole blood sampled postmortem was centrifuged at 3,750 rpm for 10 minutes or separation of serum.

Plaque assay. One hundred microliters of each sample (for samples taken through day 7 pi) were added in duplicate to Vero cell monolayers in six-well plates (Costar, Cambridge, MA). Samples were allowed to incubate on the cells for one hour at 37°C. The cells were then overlaid with 3 mL per well of 0.5% agarose in M-199 medium supplemented with 350 mg/L of sodium bicarbonate, 29.2 mg/L of L-glutamine and antibiotics as in BA-1 diluent. After 48 hours of additional incubation, a second 3-mL 0.5% agarose overlay containing 0.004% neutral red was added for plaque visualization. Plaques were counted on days 3 and 4 after infection of the Vero cells. BA-1 diluent was used as a cell viability control. Plaques from swabs and organ samples were harvested and confirmed as WN virus with a neutralization assay using a known source of antibody to WN virus.

Neutralization assays. For virus identification, 75 µL of the virus suspension (containing approximately 200 pfu/0.1 mL) were mixed in a polypropylene 96-well plate with 75 µL of WN hyperimmune mouse ascitic fluid (diluted 1:100 in BA-1 diluent) to produce a final WN virus antibody concentration of 1:200 and a final virus concentration of 100 pfu/0.1 mL. The virus-antibody mixtures were incubated at 37°C for one hour to allow virus neutralization, and then tested by plaque assay. As a negative antibody control, 75 µL of BA-1 diluent was also mixed with 75 µL of the virus suspension. A 90% reduction in the number of plaques in the test well compared with the negative control indicated a positive identification for WN virus.

For detection of neutralizing antibodies, 15 µL of postmortem serum samples was mixed with 60 µL of BA-1 diluent and 75 µL of a WN virus preparation (200 pfu/0.1 mL) in a polypropylene 96-well plate. The virus-serum mixtures were incubated at 37°C for one hour to allow for virus neutralization. These mixtures were then tested by plaque assay. Controls used only BA-1 diluent (cell viability control), a serum-free virus mixture with BA-1 (to enumerate the number of pfu in the challenge dose of virus), and a WN hyperimmune mouse ascitic fluid (diluted 1:200) mixture with virus (to verify challenge virus identity).


RESULTS
TOP
 ABSTRACT
 INTRODUCTION
 MATERIALS AND METHODS
 RESULTS
DISCUSSION
 REFERENCES
 
Detection of viremia. Forty-four green iguanas, 24 North American bullfrogs, 19 Florida garter snakes, and 22 red-ear sliders were experimentally infected with WN virus. By sampling three animals each day, we detected viremia in 10 green iguanas and 2 bullfrogs (Figure 1Go). Four green iguanas inoculated via needle and six inoculated via infected mosquito showed low viremias 1–4 days pi (maximum = 103.2 pfu/mL of serum). Only two bullfrogs had detectable viremias: one killed at one day pi (101.9 pfu/mL of serum) and one at three days pi (102.2 pfu/mL of serum). No garter snakes or red-ear sliders developed viremia above the detection threshold of our plaque assay, which was 101.7 pfu/mL of serum.



View larger version (23K):
[in this window]
[in a new window]
  		    FIGURE 1. Maximum viremias presented by day postinfection for green iguanas and North American bullfrogs experimentally infected with West Nile virus via needle or infectious mosquito. No viremia was detected after four days postinfection. The threshold of detection was 101.7pfu/mL of serum. pfu = plaque-forming units.

 
Virus isolation from swabs. West Nile virus was isolated from swabs of four needle-inoculated green iguanas, one mosquito-infected green iguana, and two bullfrogs (Table 1Go). The viral loads were very low (approximately 5 pfu/swab). All swabs from the garter snakes and red-ear sliders were negative.


View this table:
[in this window]
[in a new window]
 
TABLE 1
Isolation of West Nile virus from three reptiles and one amphibian*
 
Virus detection in organs. One needle-inoculated green iguana, one bullfrog, and three garter snakes killed on day 12 pi harbored detectable WN virus in one or more organs (Table 1Go). No patterns were discernable, except in the garter snakes. Each of the three snakes tested had a WN virus-positive spleen. The maximum viral load in organs was 400 pfu/0.5 cm3 of tissue (found in a garter snake spleen).

Detection of antibody to WN virus. Two of five needle-inoculated green iguanas tested on day 28 pi had detectable WN virus-neutralizing antibodies (87% and 88% neutralization at a serum dilution of 1:10). One cage-mate iguana failed to seroconvert.


DISCUSSION
TOP
 ABSTRACT
 INTRODUCTION
 MATERIALS AND METHODS
 RESULTS
 DISCUSSION
REFERENCES
 
Ectothermic animals have been hypothesized to play some role in the transmission of arboviruses. Asian field studies have found antibodies to Japanese encephalitis (JE) virus, a close relative of WN virus, in cobra snakes (Naja naja) and in many species of turtles.8–10 Asian laboratory studies have demonstrated JE virus replication in lizards11–13 and snakes.14,15 Laboratory experiments in the United States have confirmed reservoir competence of North American garter snakes for western equine encephalitis virus,16–19 and in one New York survey, one painted turtle (Chrysemys picta picta) and one leopard frog (Rana pipiens pipiens) circulated neutralizing antibodies to Saint Louis encephalitis virus.20

Due to the recent emergence of WN virus in North America, we investigated WN virus competence in North American reptilian and amphibian species by experimentally infecting three reptile species and one amphibian species. Although infectious virus particles were detected in the blood of some individuals, the viral titers were quite low. The threshold viremia for infecting Culex pipiens mosquitoes with the NY99 strain of WN virus is approximately 105pfu/mL of serum.21 The maximum viremia that we detected was 103.2 pfu/ mL of serum, approximately 60-fold lower than necessary for transmission to C. pipiens. These relatively low titers may be infectious to other species. Threshold viremias are unknown for mosquitoes that feed on reptiles and amphibians.

We detected WN virus-neutralizing antibodies in the serum of two of five green iguanas sampled 28 days pi. Cold-blooded vertebrates have relatively slow humoral response times, which may explain the low seroconversion rate. Some individual antibody levels may not peak for several weeks pi and may take months to decrease back to baseline levels.22,23

Although WN virus blood titers were low, infectious virus particles were also isolated from organs and oral or cloacal swabs of some animals. Thus, some reptilian or amphibian species may contribute to the infection of a predator through oral transmission. Oral transmission of WN virus has been documented in mice24 and birds.25,26 However, the minimum dose required for oral infection of crows or other potential predators is unknown.

In summary, we present experimental infection data for WN virus in green iguanas, North American bullfrogs, Florida garter snakes, and red-ear sliders. Iguanas, bullfrogs, and snakes became infected, but their contribution to the WN virus transmission cycle in nature is yet to be proven.

Received April 1, 2003. Accepted for publication May 23, 2003.

Financial support: This research was supported by an Emerging Infectious Disease fellowship sponsored by the Association of Public Health Laboratories and the National Center for Infectious Diseases (Centers for Disease Control and Prevention).

Authors’ address: Kaci Klenk and Nicholas Komar, Centers for Disease Control and Prevention, PO Box 2087, Fort Collins, CO 80522, Telephone: 970-266-3561, Fax: 970-266-3599, E-mail: knk4{at}cdc.gov.


REFERENCES
TOP
 ABSTRACT
 INTRODUCTION
 MATERIALS AND METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 

  1. Hayes CG, 1989. West Nile fever. Monath TP, ed. The Arboviruses: Epidemiology and Ecology. Volume V. Boca Raton, FL: CRC Press, 59–88.
  2. Taylor RM, Work HH, Hurlbut HS, Rizk F, 1956. A study of the ecology of West Nile virus in Egypt. Am J Trop Med Hyg 5: 579–620.
  3. Lanciotti RS, Roehrig JT, Deubel V, Smith J, Parker M, Steele K, Crise B, Volpe KE, Crabtree MB, Scherret JH, Hall A, MacKenzie JS, Cropp CB, Panigrahy B, Ostlund E, Schmitt B, Malkinson M, Banet C, Weissman J, Komar N, Savage HM, Stone W, McNamara T, Gubler DJ, 1999. Origin of the West Nile virus responsible for an outbreak of encephalitis in the Northeastern United States. Science 286: 2333–2337.[Abstract/Free Full Text]
  4. Kostyukov MA, Alekseev AN, Bul’chev VP, Gordeeva ZE, 1986. Experimentally proven infection of Culex pipiens L. mosquitoes with West Nile fever virus via the Lake Pallas Rana ridibunda frog and its transmission via bites. Med Parazitol (Mosk) 6: 76–78.
  5. Kreger MD, 1997. Laboratory housing for reptiles and amphibians. Reinhardt V, ed. Comfortable Quarters for Laboratory Animals. Washington, DC: Animal Welfare Institute, 32–40.
  6. Pough HF, 1991. Recommendations for the care of amphibians and reptiles in academic institutions. Inst Lab Anim Resources News 33: S1–S21.
  7. Mader DR, 1996. Reptile Medicine and Surgery. Philadelphia: W. B. Saunders.
  8. Shortridge KF, Ng MH, Oya A, Kobayashi M, Munro R, Wong F, Lance V, 1974. Arbovirus infections in reptiles: immunological evidence for a high incidence of Japanese encephalitis virus in the cobra, Naja naja. Trans R Soc Trop Med Hyg 68: 454–460.[Medline]
  9. Shortridge KF, Oya A, Kobayashi M, Yip DY, 1975. Arbovirus infections in reptiles: Studies on the presence of Japanese encephalitis virus antibody in the plasma of the turtle, Trionyx sinensis. Southeast Asian J Trop Med Public Health 6: 161–169.[Medline]
  10. Shortridge KF, Oya A, Kobayashi M, Duggan R, 1977. Japanese encephalitis virus antibody in cold-blooded animals. Trans R Soc Trop Med Hyg 71: 261–262.[Medline]
  11. Doi R, Oya A, Telford SR Jr, 1968. A preliminary report on infection of the lizard, Takydromus tachydromoides, with Japanese encephalitis virus. Jpn J Med Sci Biol 21: 205–207.[Medline]
  12. Oya A, Doi R, Shirasaka A, Yabe S, Sasa M, 1983. Studies on Japanese encephalitis virus infection of reptiles. I. Experimental infection of snakes and lizards. Jpn J Exp Med 53: 117–123.[Medline]
  13. Doi R, Oya A, Shirasaka A, Yabe S, Sasa M, 1983. Studies on Japanese encephalitis virus infection of reptiles. II. Roles of lizards on hibernation of Japanese encephalitis virus. Jpn J Exp Med 53: 125–134.[Medline]
  14. Mifune K, Shichijo A, Ueda Y, Suenaga O, Miyagi L, 1969. Low susceptibility of common snakes in Japan to Japanese encephalitis virus. Trop Med 11: 27–32.
  15. Lee HW, 1968. Multiplication and antibody formation of Japanese encephalitis virus in snakes. II. Proliferation of the virus. Seoul J Med 9: 157–161.
  16. Thomas LA, Eklund CM, Rush WA, 1958. Susceptibility of garter snakes (Thamnophis spp.) to western equine encephalomyelitis virus. Proc Soc Exp Biol Med 99: 698–700.
  17. Thomas LA, Eklund CM, 1960. Over-wintering of western equine encephalomyelitis virus in experimentally infected garter snakes and transmission to mosquitoes. Proc Soc Exp Biol Med 105: 52–55.
  18. Thomas LA, Eklund CM, 1962. Over-wintering of western equine encephalomyelitis virus in garter snakes experimentally infected by Culex tarsalis. Proc Soc Exp Biol Med 109: 421–424.
  19. Thomas L, Patzer E, Cory J, Coe J, 1980. Antibody development in garter snakes (Thamnophis spp.) experimentally infected with western equine encephalitis. Am J Trop Med Hyg 29: 112–117.
  20. Whitney E, Jamnback H, Means RG, Watthews TH, 1968. Arthropod-borne-virus survey in St. Lawrence County, New York. Am J Trop Med Hyg 17: 645–650.
  21. Turell MJ, O’Buinn M, Oliver J, 2000. Potential for New York mosquitoes to transmit West Nile virus. Am J Trop Med Hyg 62: 413–414.[Abstract]
  22. Hsu E, 1998. Mutation, selection, and memory in B lymphocytes of exothermic vertebrates. Immunol Rev 162: 25–36.[Web of Science][Medline]
  23. Du Pasquier L, Haimovich J, 1976. The antibody response during amphibian ontogeny. Immunogenetics 3: 381–391.
  24. Odelola HA, Oduye OO, 1977. West Nile virus infection of adult mice by oral route. Arch Virol 54: 251–253.[Web of Science][Medline]
  25. McLean RG, Ubico SR, Bourne D, Komar N, 2002. West Nile virus in livestock and wildlife. Curr Top Microbiol Immunol 267: 271–308.[Web of Science][Medline]
  26. Komar N, Langevin S, Hinten S, Nemeth N, Edwards E, Hettler D, Davis B, Bowen R, Bunning M, 2003. Experimental infection of Northern American birds with the New York 1999 strain of West Nile virus. Emerg Infect Dis 9: 311–322.[Web of Science][Medline]



This article has been cited by other articles:


Home page
 Am J Trop Med HygHome page
J. A. FARFAN-ALE, B. J. BLITVICH, N. L. MARLENEE, M. A. LORONO-PINO, F. PUERTO-MANZANO, J. E. GARCIA-REJON, E. P. ROSADO-PAREDES, L. F. FLORES-FLORES, A. ORTEGA-SALAZAR, J. CHAVEZ-MEDINA, et al.
ANTIBODIES TO WEST NILE VIRUS IN ASYMPTOMATIC MAMMALS, BIRDS, AND REPTILES IN THE YUCATAN PENINSULA OF MEXICO.
Am J Trop Med Hyg, May 1, 2006; 74(5): 908 - 914.
[Abstract] [Full Text] [PDF]

Home page
 J Wildl DisHome page
M. C. Allender, M. A. Mitchell, C. A. Phillips, K. Gruszynski, and V. R. Beasley
Hematology, plasma biochemistry, and antibodies to select viruses in wild-caught eastern massasauga rattlesnakes (sistrurus catenatus catenatus) from illinois.
J. Wildl. Dis., January 1, 2006; 42(1): 107 - 114.
[Abstract] [Full Text] [PDF]

Home page
 J Wildl DisHome page
E. R. Jacobson, P. E. Ginn, J. M. Troutman, L. Farina, L. Stark, K. Klenk, K. L. Burkhalter, and N. Komar
WEST NILE VIRUS INFECTION IN FARMED AMERICAN ALLIGATORS (ALLIGATOR MISSISSIPPIENSIS) IN FLORIDA
J. Wildl. Dis., January 1, 2005; 41(1): 96 - 106.
[Abstract] [Full Text] [PDF]

This Article
Right arrow Abstract Freely available
Right arrow Full Text (PDF)
Right arrow Alert me when this article is cited
Right arrow Alert me if a correction is posted
Right arrow Citation Map
Services
Right arrow Similar articles in this journal
Right arrow Similar articles in Web of Science
Right arrow Similar articles in PubMed
Right arrow Alert me to new issues of the journal
Right arrow Download to citation manager
Right arrow reprints & permissions
Citing Articles
Right arrow Citing Articles via HighWire
Right arrow Citing Articles via Web of Science (14)
Right arrow Citing Articles via Google Scholar
Google Scholar
Right arrow Articles by KLENK, K.
Right arrow Articles by KOMAR, N.
Right arrow Search for Related Content
PubMed
Right arrow PubMed Citation
Right arrow Articles by KLENK, K.
Right arrow Articles by KOMAR, N.

HOME HELP FEEDBACK SUBSCRIPTIONS ARCHIVE SEARCH TABLE OF CONTENTS