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Volume 10, Number 5—May 2004

Dispatch

Rift Valley Fever in Chad

David Ringot*Comments to Author , Jean-Paul Durand†, Hughes Tolou†, Jean-Paul Boutin†, and Bernard Davoust‡
Author affiliations: *Interarmy Veterinary Sector for Montpellier, Nîmes, France; †Tropical Medicine Institute of the French Defense Medical Service, Marseille, France; ‡Medical Service Directorate for Lyon, Lyon, France

Suggested citation for this article

Abstract

To evaluate the importance of human exposure to Rift Valley fever virus in Chad, investigations were carried out to determine specific antibody prevalence in domestic ruminants during the 2002 rainy season. Results highlighted recent, substantial, active transmission of this virus.

The virology laboratory of the unit of the Tropical Medicine Institute of the French Defense Medical Service (IMTSSA) investigated some cases of self-limiting nonmalarious febrile syndromes occurring among soldiers stationed in Chad. By using C6/36 and Vero cell lines, peripheral blood lymphocytes collected from two soldiers on duty in Chad during the 2001 rainy season were cocultured. Two strains of Rift Valley fever virus (RVFV) were isolated and identified by using indirect immunofluorescence, reverse transcriptase–polymerase chain reaction, and sequencing (1,2). To determine the potential for human exposure to RVFV, a seroprevalence investigation evaluated antibody prevalence in sheep, goats, and horned cattle among animals taken to slaughterhouses of N’Djamena and Abéché during the 2002 rainy season.

RVFV is a member of the genus Phlebovirus, family Bunyaviridae, and was first isolated in Kenya in 1930. Transmitted by a wide variety of mosquitoes from several genera, the virus may cause abortion in pregnant livestock and high death rate in young animals. RVFV has caused influenzalike disease in humans, and it occasionally leads to more serious complications, such as retinitis, meningoencephalitis, or severe hemorrhagic fever with a high death rate.

In Chad, RVFV has never been officially recognized by either the World Health Organization or by the International Office of Epizooties. Nevertheless, three facts suggest that the virus is present in Chad’s animal population. First, RVFV is generally thought to exist in the enzootic state in Central Africa in sheep and wild animals (3). Second, a study undertaken by the Pasteur Institute of Paris in collaboration with the EMVT (Département Elevage et Médecine Vétérinaire Tropicale du Centre de Coopération Internationale pour la Recherche en Agronomie pour le Développement) showed that 4% of sheep bred in Chad and Ethiopia had anti-RVFV neutralizing antibodies (4). Third, RVFV was identified in Sudan, Niger (5), and Nigeria, countries that border Chad.

The Study

During the 2002 rainy season (August through October), within the slaughterhouses of the cities of N’Djamena (southwestern Chad between the 10th and 15th parallels, a few kilometers from Cameroon) and Abéché (220 km east of N’Djamena), blood samples were collected from randomly selected sheep, goats, and horned cattle (Table 1). According to the veterinary services of Chad’s Ministry for Breeding, these animals were born and bred in Chad. Furthermore, they were gathered in parks a maximum of 3 days before slaughter. Sites were selected for their proximity to an area where French troops were deployed and also because the N’Djamena slaughterhouse, in particular, receives cattle from various parts of Chad.

Each sample was accompanied by information on the age of the animal (teeth examination), species, sex, and origin. Blood was centrifuged within 24 hours of collection. The serum was transferred into cryotubes and frozen at –80°C so that samples would arrive at IMTSSA for analysis still frozen (–20°C). Each sample was systematically tested for RVFV-specific immunoglobulin (Ig) G by using an enzyme-linked immunosorbent assay (ELISA). First, ELISA screening was done by using antigen capture (by mouse hyperimmune ascitic fluid) and detecting specific IgG in the diluted serum (1/500). The antigen used was a precipitate (polyethylene glycol 6000) of the supernatant of Vero cells infected with the RVFV clone 13. (This strain was isolated from a person in the Central African Republic [6] and is probably less dangerous than other strains for laboratory workers).

On the same ELISA plate as negative antigen, the serum was tested with Dugbe, a non-cross-reactive Nairovirus. All IgG-positive serum samples were retested for IgG (with a negative, noninfected Vero antigen) and IgM by using the M-antibody capture method. The most frequently used techniques for detecting anti-RVFV antibodies are immunofluorescence, plaque reduction neutralization assay, and immunoenzymatic assays (7). Because RVFV cross-reacts with many other phleboviruses (5), the choice of techniques used for this study was influenced by their sensitivity and specificity. Seroneutralization is described as the reference method for specificity (no cross-reaction with other phleboviruses) (7), but the need for cell culture makes it unsuitable for screening large numbers of serum samples (8). ELISA was preferred, since it is considered an efficient alternative in terms of sensitivity, specificity, and ease of use (7,8).

Serum samples were considered positive when the ratio between optical density associated with RVFV antigen and that associated with the Dugbe antigen was >3.5. Serum specimens demonstrating anti-RVFV IgG were validated in parallel by immunotransfer (Western blot) with a high threshold of positivity. Only serum samples containing both specific antibodies against the envelope glycoproteins (G1 and G2) and the nucleocapsid (NC) protein were considered positive. Comparative results between the two techniques confirm high specificity of ELISA (97% of the serum samples positive by ELISA were confirmed by Western blot). This high specificity has been described previously by crosschecking results with those of virus neutralization assay (8).

Conclusions

The relatively high prevalence of RVFV (Table 2) combined with the fact that 41% of IgG-positive animals are also IgM-positive (in cattle, these antibodies appear on the fourth day (9) after natural infection and persist for 2–6 months (10) underscore the seriousness of the situation in Chad. Indeed, many articles describe how domestic ruminants are an early and sensitive indicator of human epidemics (7) and how outbreaks of human infection are preceded by amplification cycles among animals (7).

The 1987 epizootic-epidemic in Mauritania was predicted by the Pasteur Institute of Dakar; by using a seroepidemiologic study among domestic animals, researchers showed that the virus had been circulating for at least 6 months in animal hosts and that an amplification cycle of the disease was in progress (11). We fear that, as occurred in Burkina Faso in 1987 (1), ecologic changes or climatic conditions favorable to vector proficiency (e.g., periods of intense rain associated with epizootic appearance in Kenya [12] and South Africa [13]) can increase, in areas where the virus circulates, antibody prevalence in animals and can lead to human cases (4). This risk appears even more important since human outbreaks are specifically preceded by an increase of antibody prevalence among animal populations. A study by the Pasteur institute of Paris showed that 4% of sheep bred in Chad and Ethiopia had anti RVFV antibodies (14), and these figures were repeatedly confirmed (4).

Data regarding origin (source and path) could not be collected for animals led to the N’Djamena slaughterhouse (all that was known was that they were born and bred in Chad) and are imprecise for those received at the Abéché slaughterhouse (local source not specified). Thus, charting the distribution of RVFV-positive animals and the geographic distribution of the virus is not possible. Nevertheless, the weak antibody prevalence in animals killed in the Abéché slaughterhouse should be noted, which allows us to conclude that this particular area is still isolated from RVFV.

Dr. Ringot is departmental manager of the interarmy veterinary sector for Montpellier for the French Defense Medical Service. One of the service’s missions is protecting French military personnel against zoonoses and biologic diseases.

Acknowledgment

We thank veterinary services of the Ministry for Breeding of Chad for their collaboration, the personnel of the medicosurgical center of the Kosseï base in N’Djamena who took part in this investigation, and J. Mosnier for his technical assistance.

References

  1. Durand JP, Richecoeur L, Peyrefitte C, Boutin JP, Davoust B, Zeller H, La fièvre de la vallée du Rift: infections sporadiques de militaires français hors des zones d’épidémies actuellement connues. Med Trop. 2002;62:2914.
  2. Durand JP, Bouloy M, Richecoeur L, Peyrefitte CN, Tolou H. Rift Valley fever virus infection among French troops in Chad. Emerg Infect Dis [serial online] 2003 Jun. Available from: http://www.cdc.gov/ncidod/EID/vol9no6/02-0647.htm
  3. Maurice Y. Premières constatations sérologiques sur l’incidence de la maladie de Wesselsbronn et de la fièvre de la vallée du Rift chez les ovins et les ruminants sauvages du Tchad et du Cameroun. Rev Elev Med Vet Pays Trop. 1967;20:395405.PubMed
  4. Lefevre PC. Actualités de la fièvre de la vallée du Rift. Quels enseignements tirer des épidémies de 1977 et 1987. Med Trop. 1997;57:614.
  5. Mariner JC, Morrill J, Ksiazek TG. Antibodies to hemorrhagic fever viruses in domestic livestock in Niger: Rift Valley fever and Crimean-Congo hemorrhagic fever. Am J Trop Med Hyg. 1995;53:21721.PubMed
  6. Muller R, Saluzzo JF, Lopez N, Dreier T, Turell M, Smith J, Characterization of clone 13, a naturally attenuated avirulent isolate of Rift Valley fever virus, which is altered in the small segment. Am J Trop Med Hyg. 1995;53:40511.PubMed
  7. Food and Agricultural Organization of the United Nations—Actes du séminaire sur la surveillance épidémiologique et le contrôle de la fièvre de la vallée du Rift en Afrique de l’Ouest (Mali – Mauritanie – Sénégal). Dakar, Sénégal, 2001 Apr 9–12. TCP/RAF/8931.
  8. Pretorius A, Oelofsen MJ, Smith MS, Van Der Ryst E. Rift Valley fever virus: a seroepidemiologic study of small terrestrial vertebrates in South Africa. Am J Trop Med Hyg. 1997;57:6938.PubMed
  9. Peters CJ, Ennis WH, Turell MJ, Niklasson B. Rapid detection of Rift Valley fever antigen in the serum of infected lambs. Res Virol. 1989;140:436. DOIPubMed
  10. Morvan J, Rollin PE, Laventure S, Roux J. Duration of immunoglobulin M antibodies against Rift Valley fever virus in cattle after natural infection. Trans R Soc Trop Med Hyg. 1992;86:675. DOIPubMed
  11. Lefevre PC. Impact des arboviroses d’intérêt vétérinaire. Le cas de la fièvre de la vallée du Rift. Med Trop. 2000;60:2730.
  12. Davies FG, Linthicum KJ, James AD. Rainfall and epizootic Rift Valley fever. Bull World Health Organ. 1985;63:9413.PubMed
  13. McIntosh BM, Jupp PG, Dos Santos I, Barnard BJ. Vector studies on Rift Valley fever virus in South Africa. S Afr Med J. 1980;58:12732.PubMed
  14. L’Hostis B. La fièvre de la vallée du Rift: étude bibliographique et enquête sérologique chez les petits ruminants dans cinq pays d’Afrique [dissertation]. Nantes, France: Université de Nantes/Ecole Nationale Vétérinaire de Nantes; 1987.

Tables

Suggested citation for this article: Ringot D, Durand J-P, Tolou H, Boutin J-P, Davoust B. Rift Valley fever in Chad. Emerg Infect Dis [serial on the Internet] 2004 May [date cited];10. Available from: http://wwwnc.cdc.gov/eid/article/10/5/03-0621.htm

DOI: 10.3201/eid1005.030621

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Table of Contents – Volume 10, Number 5—May 2004

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David Ringot, Secteur Vétérinaire Interarmées de Montpellier, BP 40 Nîmes Armées, France; fax: 33-4-67-16-55-54





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