Research Article | Open Access
Nereida Parra-Gimenez, Armando Reyna-Bello, "Parasitological, Hematological, and Immunological Response of Experimentally Infected Sheep with Venezuelan Isolates of Trypanosoma evansi, Trypanosoma equiperdum, and Trypanosoma vivax", Journal of Parasitology Research, vol. 2019, Article ID 8528430, 9 pages, 2019. https://doi.org/10.1155/2019/8528430
Parasitological, Hematological, and Immunological Response of Experimentally Infected Sheep with Venezuelan Isolates of Trypanosoma evansi, Trypanosoma equiperdum, and Trypanosoma vivax
There are three trypanosoma species of veterinary importance in South America: (1) Trypanosoma evansi, the causative agent of derrengadera mechanically transmitted by bloodsucking insects such as tabanids, (2) Trypanosoma vivax, also mechanically transmitted by some dipteras hematophages as tabanids and/or Stomoxys, and (3) T. equiperdum, a tissue parasite adapted to sexual transmission and the causative agent of dourine, a distinctive disease that affects only Equidae. In order to evaluate the parasitological, hematological, and serological response of sheep infected with T. vivax, T. evansi, and T. equiperdum, four female sheep were experimentally infected with Venezuelan trypanosome field isolates: two T. evansi of differing virulences, one T. equiperdum; one T. vivax. Parasitemia and clinical parameters such as hematocrit, red blood cell count, hemoglobin, and body temperature were measured. T. evansi caused a chronic disease with undulant parasitemia alternating with some cryptic periods of at least 54 days, with no clinical signs. T. equiperdum, never described as infectious to ruminants, also caused a chronic disease with low undulant parasitemia. T. vivax caused an acute infection with severe anemia showing a drop of more than 70% of the hematocrit value, high fever, and rapid deterioration of physical condition, for 36 days of infection. Indirect ELISAs using crude extracts of the three species of trypanosomes as antigens were performed for detection of anti-trypanosome antibodies in sheep sera. Cross-reaction was observed between the three parasite species. These results show that sheep are susceptible to the three-trypanosome species and suggest they can act as a reservoir when sheep are raised and managed with other important livestock such as cattle, horses, buffalos, or goats. These findings are especially interesting for T. equiperdum, a species that has not been reported as infective to sheep.
Haemoparasitoses represent one of the main limitations for the development of the cattle industry in Africa, Asia, and Latin America. The economic losses caused by parasitic diseases are attributed mainly to reduced weight gain, lower milk production, high mortality, and high costs of veterinary care [1, 2]. Only two species of trypanosomes with veterinary implications in South America have been identified due to their pathogenicity in livestock: Trypanosoma vivax and T. evansi . However, Sanchez et al.  recently confirmed the first molecular report of T. equiperdum in Latin America.
Trypanosoma evansi is a mechanically transmitted extracellular blood parasite that causes equine trypanosomosis or surra, also known as Derrengadera in South America [4, 5]. Although it most notably affects horses and camels, it can also affect donkeys, dogs, cats, cattle, and buffalo . Other wild mammals, such as capybaras (Hydrochoerus hydrochaeris), act as reservoirs . Experimental T. evansi infections in sheep have shown a chronic and often cryptic disease, with low parasitemias and some cases of self-cure [8–11]. Desquesnes et al.  review a naturally infected sheep during outbreak in France due to T. evansi. In South America, specifically in Brazil, there are reports of vertical transmission using experimental infection in pregnant sheep . The clinical signs of T. evansi infection include anemia, recurrent fever, weight loss, emaciation, swelling of the hind limbs, and hemostatic abnormalities [6, 13].
Trypanosoma vivax is one of the most important pathogenic species of trypanosoma and is cyclically transmitted to domestic livestock by tsetse flies (Glossina spp,) as well as by mechanical means though other bloodsucking insects [1, 4, 14]. T. vivax cause a critical and often fatal disease in ruminants such as cattle, buffalos, sheep and goats, due to the high fever and induced anemia [1, 15]. In Brazil, the infection by T. vivax has also been described in horses . Clinical signs include fever, emaciation, anorexia, and immunosuppression. Thrombocytopenia, microthrombus formation, and hemorrhage suggestive of disseminated intravascular coagulation have also been demonstrated [14, 17, 18]. This haemoparasite was introduced to South America by cattle imported from Africa, as it can be transmitted by tabanids and stomoxes. Once this haemoflagelar arrived in Latin America, with the absence of Tsetse fly, T. vivax, it initiated an evolutionary differentiation by losing genes from its maxicircle . The parasite has spread in the continent where it is now endemic from Brazil to Costa Rica, including Colombia, Venezuela, Peru, Bolivia, Panama, Paraguay, and Ecuador [1, 14, 17, 20, 21].
T. equiperdum is the causative agent of dourine in horses and donkeys. It differs from other mammalian trypanosomes since it is transmitted sexually and is primarily a tissue parasite, very difficult to find in blood [22–25]. Dourine has a worldwide distribution; it has been reported in Africa, Asia, Southern and Eastern Europe, Mexico, and Venezuela [3, 25].
The objective of this preliminary study was to evaluate the effect of experimental infections in sheep with three trypanosomes of veterinary interest in the region: T. evansi, T. vivax, and T. equiperdum.
2. Materials and Methods
One T. equiperdum isolate (TeAp-N/D1) and two T. evansi isolates (R38 and TeApMantecal01) from horse (Equus caballus) blood  and one T. vivax isolate (Tucacas) from cattle (Bos taurus) blood (kindly donated by Dr. Garcia) (Table 1) were used in this study.
2.2. Isolation of Trypanosomes
For T. evansi and T. equiperdum infections, the cryopreserved isolate were inoculated into the peritoneum of Sprague Dawley rats to obtain sufficient parasites for experimental sheep infections. When parasitemia reached 108 trypanosomes/ml, blood was obtained by cardiac puncture in the presence of heparin as anticoagulant under anesthesia with ether. Parasites were counted using a Neubauer chamber.
2.3. Experimental Animals
Four healthy, helminth-free crossbreed female sheep, between 3 and 6 months of age, were obtained locally and maintained for a month prior to experimental infection. For T. evansi and T. equiperdum, fresh 1 x106 parasites coming directly from infected rats were inoculated, while, for T. vivax, 1 x 106 cryopreserved ones were injected. After inoculation, the course of the infection was monitored for 65 days for T. evansi and T. equiperdum infections, but the T. vivax infected sheep was treated with 0.5 mg/kg isometamidium chloride (Hemoveex ®, Reveex, Venezuela) at 36 days postinfection to prevent animal death. The presence of parasites in the blood, rectal temperature, hematocrit, erythrocyte count, and hemoglobin concentration was monitored every other day during the experimental infection. A noninfected sheep was used as a control and the same clinical parameters were measured.
2.4. Detection of Trypanosomes in the Blood
For detection of parasitemia, 100 microscope fields of wet films were examined using a light microscope at 40 X magnification, as described by Brenner . The parasitemia was expressed as parasites/ml and the hematocrit centrifugation technique (HCT)  was used to observe parasites in case of very low levels of parasitaemia.
2.5. Body Temperature
Every other day at the same hour and using a rectal thermometer, temperature was measured and expressed in °C.
For determination of packed cell volume (PCV), blood (60 μl) was drawn into heparinized micro capillary tubes, which were centrifuged at 10.000 g per 5 min and the PCV was measured using a microhematocrit scale.
2.7. Red Blood Cell Count
To determine hematological data, a sample of sheep blood was drawn, using vacuum tubes containing EDTA as anticoagulant. The blood was diluted 1: 1000 in 3% trisodic Citrate and 1% formol. Red blood cells (RBC) were counted with an optical microscope using a Neubauer chamber.
The cyanmethemoglobin method was used to determine hemoglobin concentration. Blood was diluted in Drabking solution and the absorbance was assessed photometrically at 540 nm on a Milton Roy Spectronic1201.
2.9. Serum Sample
All blood samples were collected from the jugular vein in vacuum tubes without anticoagulant. The tubes were labeled and the blood was allowed to clot overnight at room temperature and the serum was separated by centrifugation. Samples were stored at -20°C until testing.
2.10. Preparation of Antigen for ELISA
Parasites for T. evansi and T. equiperdum antigen preparation were obtained from experimentally infected rats as describes previously. Parasites were purified by anion exchange chromatography using DEAE-Cellulose by described Lanham and Godfrey . The resultant parasites pellet was resuspended in 2 ml of PBS 20 mM, pH 7.2, and disrupted by thermal shock. The resulting homogenate was stored at -20°C with proteases inhibitors until used.
For T. vivax parasites purification, the protocol described by Gonzalez et al.  was used.
2.11. ELISA Procedure
For each trypanosome isolate, an ELISA plate was used, all under the same conditions, with each sample in duplicate. Negative serum samples were obtained from each sheep two weeks prior to infection and used as negative controls. During experimental infection, samples were taken at days -1, 2, 10, 18, 24, 30, 39, 47, and 61. Sensitized plates with 20 μg/well of antigen were washed five times with washing buffer (WB) (PBS-Tween 0.05 %, pH 7.2) and blocked with 200 μl/well of 5% skim milk in PBS for an hour at 37°C. Plates were washed five times with WB, and 100 μl/well of each sera diluted 1:200 in WB was added. Positive and negative reference sera were included in each ELISA plate. After incubation for an hour at 37°C, plates were washed five times with WB, and 100 μl of conjugate (Rabbit peroxidase conjugated anti-sheep IgG Pierce. Immunopure ® Antibody) diluted 1:5000 with WB was added and plates were incubated for 60 minutes at 37°C. After incubation, the plates were washed three times (PBS-Tween 0.05 %, pH 7.2) and 100 μl of substrate solution, ABTS 2% H2O2 was added and incubated at 37°C for 45 min. Absorbance was measured photometrically at 405 nm on an ELISA reader (BioRad 3550).
3.1. Disease Course
Infection profiles of the T. evansi, T. equiperdum, and T. vivax isolates are shown in Table 2. Animals infected with T. evansi and T. equiperdum were monitored for 65 days, while the sheep infected with T. vivax was monitored until day 36 when it was treated with a trypanocide drug. Animals infected with T. evansi and T. equiperdum developed chronic trypanosomosis with fluctuating parasitemias. T. evansi parasitemia reached a maximum value of about 7.9 x 104 tryp/ml blood (Figure 1). Parasites were detected by the Woo method  at 24, 43, and 54 days postinfection. In the T. vivax infection, parasitemia reached 3.4 x 106 tryp/ml blood at day 36. During infection, it showed an undulating parasitemia ranking between 1 x 102 and 5 x 104. The prepatent period for all infections was 2 days (Table 2)
3.1.2. Clinical Changes
The clinical changes were evaluated during 64 days postinfection. There were varying increases in the body temperature that coincide with parasitemia peaks in the T. evansi, T. vivax, and T. equiperdum infections (Figure 2(a)). Decreases in the hematocrit values in red cell count and hemoglobin were observed from the beginning of the infection until day 22 postinfection for the T. evansi and T. equiperdum infections, afterwards values returned to the normal range (Figures 2(b), 2(c), and 2(d)). In the T. vivax infection, significant decreases in these parameters were observed, as compared to the noninfected or infected with the other trypanosomes.
3.2. Parasite-Specific Antibody Responses (Antibody-ELISA)
The kinetics of anti-T. evansi, anti-T. vivax, and anti-T. equiperdum antibodies in the experimentally infected sheep are shown in Figure 3. The ELISA tests were either homologous, in which the sera reacted to antigens from the same isolate, or heterologous, whereby sera bound antigens from a different isolate. When the sera were examined against homologous and heterologous antigens of T. evansi, T. vivax, or T. equiperdum, homologues antigens showed a greater recognition. However, for the T. vivax antigen, recognition of the homologous sera is higher than the heterologous system. Note that the increase in the serologic response is continuous throughout the period of the infection when heterologous system is used; however, in homologous systems there is an increase in all antibody kinetics between days 24 and 39.
Experimental Infection with T. evansi, T. equiperdum, and T. vivax. In the present paper, experimental infection of sheep with T. evansi, T. equiperdum, and T. vivax was achieved. Data show a T. vivax acute infection with dramatic decrease of hematocrit and red blood cells counts. In contrast, T. evansi and T. equiperdum isolates caused a chronic disease with slight clinical manifestations.
Interestingly, T. equiperdum is described as the only sexually transmitted trypanosome and not as a vector borne disease. Its host spectrum is very narrow, infecting almost exclusively equine and rabbits after experimental intratesticular inoculation [25, 30]. Once these strains have been adapted to the rabbit, other rodents such as rats and mice can be infected (OIE, 2016). A reference author on trypanosomiasis  also points out that T. equiperdum, a tissue parasite, rarely invades the blood. In ruminants, experimental infections could produce weak manifestations of Dourine and cryptic or low parasitemias [8, 11, 12]. In this experimental infection, we observed that T. equiperdum isolate was able to infect sheep and remained by 54 days of the experimental infection. Throughout the infection, the trypanosomes were observed in blood in undulating parasitaemia and the cutaneous edema characteristic of Dourine was never evident. In view of these results TeAp-N/D1 isolate obtained from a horse naturally infected in the Venezuelan savanna shows an unknown evolutionary form of T. equiperdum in the new world.
Trypanosoma evansi has a worldwide geographical distribution; Africa, Asia, and Central and South America are the main endemic areas. In natural infections of horses, various symptoms have been reported, including intermittent fever, severe anemia, limb edema, lethargy, loss of appetite, weight loss, and other symptoms [6, 31]. The virulence of a parasite depends on several factors: (a) susceptibility of the host, (b) host ability to control the parasitemia, and (c) intrinsic parasite factors, which could lead to a better adaptation to the host. Perrone et al., 2003, reported nine Venezuelan isolates of Trypanosoma spp. with marked differences in virulence in mice; two of them were used in the present study: TeApMantecal01 (T. evansi) and TeAp-N/D1 (T. equiperdum) . Even though both isolates showed a virulent behavior in mice and rats [32, 33], the T. equiperdum isolate appeared extremely virulent in both experimental models, causing an acute disease. These findings agree with observations reported by Onah et al.  and Audu et al.  in experimental sheep infections with T. evansi in Africa, where acute and chronic phases of the disease were observed. Campigotto et al., 2015, also reported experimental infections in sheep, with mild anemia and low parasitemia. However, fluctuating parasitemias were not observed.
Our biological data suggest that sheep are susceptible to both T. evansi and T. equiperdum isolates in Venezuela. The presence of the parasites in blood leads to great economic losses and increases the odds of the parasite transmission to other hosts.
The sheep experimentally infected with T. vivax showed an acute disease characterized by undulating parasitemia during the first 24 days after infection, and a rapid deterioration of the physical condition. The hematocrit values and RBC count showed a progressive reduction, until it reached a value of less of 18% at the day of the trypanocidal treatment. The clinical signs confirm the high pathogenicity and virulence of this T. vivax isolate in this ruminant model. This agrees with findings of naturally and experimentally infected sheep and goats reported for other T. vivax field isolates [17, 31, 34, 35].
In Africa and America, cattle and buffalo livestock share their habitats with herds of sheep and goats. Epidemiological data of field-infected herds showed the likelihood of T. vivax transmission between asymptomatic carriers such as buffalo and donkeys to susceptible hosts, in a same area . In Brazil, where sheep and goats are important livestock in the semiarid region, those animals may be severely affected by T. vivax infection, showing anemia, hyperthermia, enlarged lymph nodes, and progressive weight loss .
Even though we used a reduced number of experimental animals, the sheep susceptibility to T. evansi, T. equiperdum, and T. vivax was demonstrated and could open the possibilities of mixed infection in natural hosts of endemic areas due to the presence of the vector and the proximity of grazing areas.
Antigenic Cross-Reactivity by ELISA. The cross-reactivity between T. evansi and T. vivax is well documented (Reyna-Bello et al. , Desquesnes et al. , Uzcanga et al. , and Camargo et al. [39, 40]); our results show the same behavior with T. equiperdum. However, a reciprocal cross-reactivity does not occur when T. vivax is used as the antigen to detect antibodies against T. evansi or T. equiperdum. As this is a preliminary account of the infection of T. equiperdum in an ovine model, we can only speculate about the ability of the parasite to stimulate the immune response and more studies are needed to evaluate this phenomenon.
The experimental results of this study suggest the possibility of widespread infection by T. evansi, T. equiperdum, or T. vivax in Venezuela herds sheep. The existence of the disease should be suspected when clinical signs common to any of the three trypanosomes species appear. We state the possibility that sheep act as a reservoir for these three trypanosomes in areas where they live close to equines and cattle. In addition, it was observed in indirect ELISA that cross-reactivity between T. evansi and T. equiperdum versus T. vivax is curiously unidirectional.
Finally, we wish to point out that a sheep infected with a strain of T. equiperdum, described in previous studies, remained infected at least for 54 days, which represents an unusual finding.
The data used to support the findings of this study are available from the corresponding author upon request.
The authors declare that all the experiments in this paper were carried out in accordance with the legal and ethical standards of Venezuela.
Conflicts of Interest
The authors declare that they have no conflicts of interest.
Armando Reyna-Bello participated in the experimental design and analysis of the data. Nereida Parra-Gimenez participated in the development of the experimental design and contributed to the manuscript draft. All authors read and approved the final manuscript.
The authors thank Dr. Trina Perrone for her invaluable insights regarding the comparison of trypanosome isolates and for all their support during the realization of this experimental work. This research was supported by grants from FONACIT no. 2004000400 RIDMOH; Misión Ciencia 2007001425 from Instituto Venezolano de Investigaciones Científicas (IVIC). They thank Dr. Mary Isabel Gonzatti from Universidad Simón Bolivar, Dr. Alfredo Mijares, and Dr. Howard Takiff from Instituto Venezolano de Investigaciones Científicas, and Beatriz Cajade from Texas University for critically reading this manuscript.
- M. I. Gonzatti, B. González-Baradat, P. M. Aso, and A. Reyna-Bello, “Trypanosoma (duttonella) vivax and typanosomosis in latin America: Secadera/Huequera/Cacho Hueco,” in Trypanosomes and Trypanosomiasis, S. Magez and M. Radwanska, Eds., pp. 261–285, Springer, New York, NY, USA, 2014.
- A. A. Boada-Sucre, M. S. Rossi Spadafora, L. M. Tavares-Marques, H. J. Finol, and A. Reyna-Bello, “Trypanosoma vivax adhesion to red blood cells in experimentally infected sheep,” Pathology Research International, vol. 2016, Article ID 4503214, 9 pages, 2016.
- E. Sánchez, T. Perrone, G. Recchimuzzi et al., “Molecular characterization and classification of Trypanosoma spp. Venezuelan isolates based on microsatellite markers and kinetoplast maxicircle genes,” Parasites & Vectors, vol. 8, no. 1, Article ID 536, 2015.
- A. L. A. R. Osório, C. R. Madruga, M. Desquesnes, C. O. Soares, L. R. R. Ribeiro, and S. C. G. Da Costa, “Trypanosoma (Duttonella) vivax: Its biology, epidemiology, pathogenesis, and introduction in the New World - A review,” Memórias do Instituto Oswaldo Cruz, vol. 103, no. 1, pp. 1–13, 2008.
- M. Desquesnes, A. Dargantes, D.-H. Lai, Z.-R. Lun, P. Holzmuller, and S. Jittapalapong, “Trypanosoma evansi and surra: a review and perspectives on transmission, epidemiology and control, impact, and zoonotic aspects,” BioMed Research International, vol. 2013, Article ID 321237, 20 pages, 2013.
- M. Desquesnes, P. Holzmuller, D.-H. Lai, A. Dargantes, Z.-R. Lun, and S. Jittaplapong, “Trypanosoma evansi and surra: a review and perspectives on origin, history, distribution, taxonomy, morphology, hosts, and pathogenic effects,” BioMed Research International, vol. 2013, Article ID 194176, 22 pages, 2013.
- T. M. Perrone, M. I. Gonzatti, G. Villamizar, A. Escalante, and P. M. Aso, “Molecular profiles of Venezuelan isolates of Trypanosoma sp. by random amplified polymorphic DNA method,” Veterinary Parasitology, vol. 161, no. 3-4, pp. 194–200, 2009.
- D. N. Onah, J. Hopkins, and A. G. Luckins, “Haematological changes in sheep experimentally infected with Trypanosoma evansi,” Parasitology Research, vol. 82, no. 8, pp. 659–663, 1996.
- D. N. Onah, J. Hopkins, and A. G. Luckins, “Proliferative responses of peripheral blood leucocytes of sheep infected with Trypanosoma evansi,” Scandinavian Journal of Immunology, vol. 48, no. 2, pp. 170–176, 1998.
- D. N. Onah, J. Hopkins, and A. G. Luckins, “Changes in peripheral blood lymphocyte subpopulations and parasite- specific antibody responses in Trypanosoma evansi infection of sheep,” Parasitology Research, vol. 85, no. 4, pp. 263–269, 1999.
- P. A. Audu, K. A. N. Esievo, G. Mohammed, and O. J. Ajanusi, “Studies of infectivity and pathogenicity of an isolate of Trypanosoma evansi in Yankasa sheep,” Veterinary Parasitology, vol. 86, no. 3, pp. 185–190, 1999.
- G. Campigotto, A. S. Da Silva, A. Volpato et al., “Experimental infection by Trypanosoma evansi in sheep: Occurrence of transplacental transmission and mice infection by parasite present in the colostrum and milk of infected ewes,” Veterinary Parasitology, vol. 212, no. 3-4, pp. 123–129, 2015.
- H. Mekata, S. Konnai, C. N. Mingala et al., “Isolation, cloning, and pathologic analysis of Trypanosoma evansi field isolates,” Parasitology Research, vol. 112, no. 4, pp. 1513–1521, 2013.
- M. Desquesnes, Livestock Trypanosomoses and Their Vectors in Latin America, CIRAD-EMVT Publication, OIE, Paris, France, 2004.
- H. A. Garcia, O. J. Ramírez, C. M. F. Rodrigues et al., “Trypanosoma vivax in water buffalo of the Venezuelan Llanos: An unusual outbreak of wasting disease in an endemic area of typically asymptomatic infections,” Veterinary Parasitology, vol. 230, pp. 49–55, 2016.
- A. S. Da Silva, H. A. Garcia Perez, M. M. Costa et al., “Horses naturally infected by Trypanosoma vivax in southern Brazil,” Parasitology Research, vol. 108, no. 1, pp. 23–30, 2011.
- J. S. Batista, A. F. Oliveira, C. M. F. Rodrigues et al., “Infection by Trypanosoma vivax in goats and sheep in the Brazilian semiarid region: From acute disease outbreak to chronic cryptic infection,” Veterinary Parasitology, vol. 165, no. 1-2, pp. 131–135, 2009.
- C. Gutierrez, J. A. Corbera, M. Morales, and P. Büscher, “Trypanosomosis in goats: Current status,” Annals of the New York Academy of Sciences, vol. 1081, pp. 300–310, 2006.
- G. Greif, M. Rodriguez, A. Reyna-Bello, C. Robello, and F. Alvarez-Valin, “Kinetoplast adaptations in American strains from Trypanosoma vivax,” Mutation Research - Fundamental and Molecular Mechanisms of Mutagenesis, vol. 773, pp. 69–82, 2015.
- T. W. Jones and A. M. R. Dávila, “Trypanosoma vivax - Out of Africa,” Trends in Parasitology, vol. 17, no. 2, pp. 99–101, 2001.
- H. Garcia, M. Garcia, H. Perez, and A. Mendoza-Leon, “The detection and PCR-based characterization of the parasites causing trypanosomiasis in water-buffalo herds in Venezuela,” Annals of Tropical Medicine & Parasitology, vol. 99, no. 4, pp. 359–370, 2013.
- Y. Wei, Y-Z. Wen, M. Desquesnes, and Z-R. Lun, “Molecular epidemiology of Trypanosoma evansi and T. equiperdum and atypical human infection by animal trypanosomes,” in The Molecular Epidemiology of Trypanosomes and Leishmania, pp. 1–14, Geoff Hide, 2011.
- I. Pascucci, A. Di Provvido, C. Cammà et al., “Diagnosis of dourine in outbreaks in Italy,” Veterinary Parasitology, vol. 193, no. 1-3, pp. 30–38, 2013.
- M. P. Vulpiani, A. Carvelli, D. Giansante, F. Iannino, D. Paganico, and N. Ferri, “Reemergence of dourine in Italy: Clinical cases in some positive horses,” Journal of Equine Veterinary Science, vol. 33, no. 6, pp. 468–474, 2013.
- Y. Gizaw, M. Megersa, and T. Fayera, “Dourine: a neglected disease of equids,” Tropical Animal Health and Production, vol. 49, no. 5, pp. 887–897, 2017.
- Z. Brener, “The behaviour of slender and stout forms of trypanosoma cruzi in the blood-stream of normal and immune mice,” Annals of Tropical Medicine and Parasitology, vol. 63, no. 2, pp. 215–220, 1969.
- P. T. Woo, “The haematocrit centrifuge for the detection of trypanosomes in blood.,” Canadian Journal of Zoology, vol. 47, no. 5, pp. 921–923, 1969.
- S. M. Lanham and D. G. Godfrey, “Isolation of salivarian trypanosomes from man and other mammals using DEAE-cellulose,” Experimental Parasitology emphasizes, vol. 28, no. 3, pp. 521–534, 1970.
- L. E. González, J. A. García, C. Núñez et al., “Trypanosoma vivax: a novel method for purification from experimentally infected sheep blood,” Experimental Parasitology emphasizes, vol. 111, no. 2, pp. 126–129, 2005.
- C. Hoare, “The Trypanosomes of Mammals. Blackwell Scientific Publications,” Oxford and Edinburgh, p. 749, 1972.
- C. M. F. Rodrigues, R. G. Olinda, T. M. F. Silva et al., “Follicular degeneration in the ovaries of goats experimentally infected with Trypanosoma vivax from the Brazilian semi-arid region,” Veterinary Parasitology, vol. 191, no. 1-2, pp. 146–153, 2013.
- T. M. Perrone, Tipificación de Aislados Venezolanos de Trypanosoma evansi.[Doctoral, thesis], Universidad Simón Bolívar, 2003.
- P. Holzmuller, P. Grébaut, J.-B. Peltier et al., “Secretome of animal trypanosomes: From a standard method toward new diagnostic and therapeutic targets,” Annals of the New York Academy of Sciences, vol. 1149, pp. 337–342, 2008.
- G. J. N. Galiza, H. A. García, A. C. O. Assis et al., “High mortality and lesions of the central nervous system in trypanosomosis by Trypanosoma vivax in Brazilian hair sheep,” Veterinary Parasitology, vol. 182, no. 2–4, pp. 359–363, 2011.
- A. A. Boada-Sucre, M. S. Rossi, E. Gómez, R. González, J. P. Rodríguez, and A. Reyna-Bello, “Sheep experimental infection with isolate LIEM-176 of Trypanosoma vivax: changes in body temperature, hematocrit, hemoglobin and plasma proteins,” Revista Ibero-Latinoamericana de Parasitología, vol. 72, no. 2, pp. 132–141, 2013.
- A. Reyna-Bello, F. A. García, M. Rivera, B. Sansó, and P. M. Aso, “Enzyme-linked immunosorbent assay (ELISA) for detection of anti-Trypanosoma evansi equine antibodies,” Veterinary Parasitology, vol. 80, no. 2, pp. 149–157, 1998.
- M. Desquesnes, Z. Bengaly, L. Millogo, Y. Meme, and H. Sakande, “The analysis of the cross-reactions occurring in antibody-ELISA for the detection of trypanosomes can improve identification of the parasite species involved,” Annals of Tropical Medicine and Parasitology, vol. 95, no. 2, pp. 141–155, 2001.
- G. L. Uzcanga, T. Perrone, J. A. Noda et al., “Variant surface glycoprotein from Trypanosoma evansi Is partially responsible for the cross-reaction between Trypanosoma evansi and Trypanosoma vivax,” Biochemistry, vol. 43, no. 3, pp. 595–606, 2004.
- R. E. Camargo, G. L. Uzcanga, and J. Bubis, “Isolation of two antigens from Trypanosoma evansi that are partially responsible for its cross-reactivity with Trypanosoma vivax,” Veterinary Parasitology, vol. 123, no. 1-2, pp. 67–81, 2004.
- R. Camargo, A. Izquier, G. L. Uzcanga et al., “Variant surface glycoproteins from Venezuelan trypanosome isolates are recognized by sera from animals infected with either Trypanosoma evansi or Trypanosoma vivax,” Veterinary Parasitology, vol. 207, no. 1-2, pp. 17–33, 2015.
Copyright © 2019 Nereida Parra-Gimenez and Armando Reyna-Bello. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.