Molecular characterization and classification of Trypanosoma spp. Venezuelan isolates based on microsatellite markers and kinetoplast maxicircle genes
- E. Sánchez1,
- T. Perrone^1,
- G. Recchimuzzi2,
- I. Cardozo1,
- N. Biteau3,
- PM Aso2,
- A. Mijares1,
- T. Baltz3,
- D. Berthier4,
- L. Balzano-Nogueira5 and
- MI Gonzatti2Email author
© Sánchez et al. 2015
Received: 6 July 2015
Accepted: 1 October 2015
Published: 15 October 2015
The Erratum to this article has been published in Parasites & Vectors 2015 8:566
Livestock trypanosomoses, caused by three species of the Trypanozoon subgenus, Trypanosoma brucei brucei, T. evansi and T. equiperdum is widely distributed throughout the world and constitutes an important limitation for the production of animal protein. T. evansi and T. equiperdum are morphologically indistinguishable parasites that evolved from a common ancestor but acquired important biological differences, including host range, mode of transmission, distribution, clinical symptoms and pathogenicity. At a molecular level, T. evansi is characterized by the complete loss of the maxicircles of the kinetoplastic DNA, while T. equiperdum has retained maxicircle fragments similar to those present in T. brucei. T. evansi causes the disease known as Surra, Derrengadera or "mal de cadeiras", while T. equiperdum is the etiological agent of dourine or "mal du coit", characterized by venereal transmission and white patches in the genitalia.
Nine Venezuelan Trypanosoma spp. isolates, from horse, donkey or capybara were genotyped and classified using microsatellite analyses and maxicircle genes. The variables from the microsatellite data and the Procyclin PE repeats matrices were combined using the Hill-Smith method and compared to a group of T. evansi, T. equiperdum and T. brucei reference strains from South America, Asia and Africa using Coinertia analysis. Four maxicircle genes (cytb, cox1, a6 and nd8) were amplified by PCRfrom TeAp-N/D1 and TeGu-N/D1, the two Venezuelan isolates that grouped with the T. equiperdum STIB841/OVI strain. These maxicircle sequences were analyzed by nucleotide BLAST and aligned toorthologous genes from the Trypanozoon subgenus by MUSCLE tools. Phylogenetic trees were constructed using Maximum Parsimony (MP) and Maximum Likelihood (ML) with the MEGA5.1® software.
We characterized microsatellite markers and Procyclin PE repeats of nine Venezuelan Trypanosoma spp. isolates with various degrees of virulence in a mouse model, and compared them to a panel of T. evansi and T. equiperdum reference strains. Coinertia analysis of the combined repeats and previously reported T. brucei brucei microsatellite genotypes revealed three distinct groups. Seven of the Venezuelan isolates grouped with globally distributed T. evansi strains, while TeAp-N/D1 and TeGu-N/D1 strains clustered in a separate group with the T. equiperdum STIB841/OVI strain isolated in South Africa. A third group included T. brucei brucei, two strains previously classified as T. evansi (GX and TC) and one as T. equiperdum (BoTat-1.1). Four maxicircle genes, Cytochrome b, Cythocrome Oxidase subunit 1, ATP synthase subunit 6 and NADH dehydrogenase subunit 8, were identified in the two Venezuelan strains clustering with the T. equiperdum STIB841/OVI strain. Phylogenetic analysis of the cox1 gene sequences further separated these two Venezuelan T. equiperdum strains: TeAp-N/D1 grouped with T. equiperdum strain STIB818 and T. brucei brucei, and TeGu-N/D1 with the T. equiperdum STIB841/OVI strain.
Based on the Coinertia analysis and maxicircle gene sequence phylogeny, TeAp-N/D1 and TeGu-N/D1 constitute the first confirmed T. equiperdum strains described from Latin America.
KeywordsTrypanosoma equiperdum Trypanosoma evansi Maxicircle Microsatellite genotyping Coinertia analysis
Trypanosomes are unicellular parasites that cause important diseases in humans and animals. They comprise a wide group of parasites of vertebrates usually transmitted by haematophagous arthropods . Livestock trypanosomoses caused by Trypanosoma brucei brucei, Trypanosoma equiperdum and Trypanosoma evansi, all belonging to the Trypanozoon subgenus, has a significant socio-economic impact and limits animal protein productivity throughout the world [2–4]. T. evansi, the first pathogenic trypanosome discovered, was found in the blood of horses and camels suffering an endemic disease known as Surra, derrengadera, murrina or “mal de cadeiras” . T. evansi was introduced to America in the XV century through the importation of horses from Africa by Spanish conquerors [5–7]. T. evansi is mechanically transmitted and it is now widely distributed throughout tropical and subtropical regions of Northern Africa, Southeast Asia, as well as Central and South America, where livestock and native wildlife are severely affected [2, 5, 8–10]. In Europe, the importation of dromedary camels from the Canary Islands was associated with T. evansi outbreaks in France and Spain [11, 12] and chronic T. evansi infection and death was reported in a dog that returned to Germany after international travel .
T. evansi is morphologically indistinguishable from the two other pathogenic species, T. brucei and T. equiperdum [5, 14–17]. T. equiperdum is the causative agent of dourine, a distinctive disease that only affects Equidae and is transmitted mainly via coitus [16, 18–22]. Because T. evansi, T. equiperdum and T. brucei species cannot be distinguished by sequences of their ribosomal RNA (rRNA) genes [1, 23–27], other probes, including isoenzymes and peptidase profiles [28–30], restriction fragment length polymorphisms , kinetoplast sequences [32, 33] and microsatellites markers  have been used to characterize and distinguish these trypanosome species. Simple sequence repeat (SSR) microsatellites are DNA loci with tandemly repeated short sequence motifs, whose copy number is hypervariable at each locus [35, 36]. The mutation rate of SSR microsatellites, and thus their variability, is higher than that observed for isoenzyme or RFLP markers [37–39], making them highly useful for studying the relationships between closely related species or within populations of the same species [40, 41].
All Kinetoplastids, including the species within the Trypanozoon subgenus, contain kinetoplasts, a concatenated network of complex mitochondrial DNA comprising 5.000-10.000 minicircles of about 1000 bp , T. brucei minicircles sequences are highly heterogeneous  while the minicircles from T. evansi strains from Africa, Asia and South America, show extensive sequence conservation [44–47]. With the exception of Trypanosoma evansi, all species within the Trypanosoma genus contain 50-100 complete or partial maxicircles varying in size from 20 Kbp for T. brucei ssp. to 40 kbp for C. fasciculata . The maxicircles encode mitochondrial genes necessary for development and differentiation in the insect vector [48–51].
We previously showed that Venezuelan Trypanosoma spp. isolates separated into two groups, according to their RAPD profiles . Seven of the nine Venezuelan isolates clustered together, while two highly virulent horse isolates, TeAp-N/D1 and TeGu-N/D1, appeared to be genetically distinct [17, 52, 53]. By analyzing microsatellite loci and PE repeats, we found that the seven less virulent isolates clustered with T. evansi reference strains, while the more virulent TeAp-N/D1 and TeGu-N/D1 isolates closely matched a T. equiperdum reference strain, leading us to look for the presence of maxicircle genes.
Trypanosoma spp. field isolates and DNA extraction
Nine Venezuelan Trypanosoma spp. isolates were obtained from horse, donkey or capybara blood samples, as previously described : TeAp-Cedral05, TeAp-Cedral12, TeAp-ElFrío01, TeAp-Mantecal01, TeAp-N/D1, TeGu-N/D1, TeGu-Terecay01, TeGu-Terecay03 and TeGu-Terecay323. The trypanosomes were expanded in rats and purified by ion exchange chromatography (DEAE-Cellulose) . Parasites were quantified with a hemocitometer and genomic DNA was extracted using a commercial kit (BDtract™, Maxim Biotech, Inc). DNA concentration and purity were determined in a SmartSpect™ 3000 (BioRad). The DNA and PCR amplification products were analyzed by agarose gel electrophoresis under standard conditions.
The project was approved by the COBIANIM (IVIC-DIR-1073/12) an advisory body of IVIC with regard to the ethical use of animals in research, in accordance with national and international standards. This committee oversees all research activities at IVIC, requiring the use of animals and wildlife to meet with Venezuelan law and universal ethical values. The Commission assessed the methodological, bioethical and legal aspects of this project by resolution IVIC/No 1444 .
Microsatellite and Procyclin PE-typing
The PCR amplifications for microsatellite analysis were performed with an Eppendorf Mastercycler, as described . Five microsatellite markers were employed, four that were previously used to characterize trypanosome isolates , and a fifth new genetic marker MD2.349-CA amplified with primers MD2.349-CA-F (GCATGCGTGAGGAAGTGAG) and MD2.349-CA-R (GTCCTGTTGGCCGCATTAT) and also a sequence corresponding to the Procyclin PE repeats. The lengths of the PCR products were determined using the Genescan software (Applied Biosystems), and they were sequenced using an ABI 3130 XL (Applied Biosystems) at the C.G.F.B. (Functional Genomic Center of Bordeaux, France).
Two matrices were generated based on genotyping with microsatellite and Procyclin PE repeats (Additional file 1) and previously published data on T. brucei brucei . The categorical values matrix contains all the evaluated microsatellite data, classified from the lowest to the highest number of repeats. The binary values matrix was constructed with the Procyclin PE repeats data, where (0) was the absence and (1) the presence of a determined PE repeat. When each qualitative variable is represented by binary indicator variables for each category, specifying whether an object belongs to it (1) or not (0), multiple correspondence analysis (MCA) can be formulated as a principal component analysis (PCA) of the total set of these indicator variables with respect to some predefined metrics. Thus, just as in PCA, object coordinates can be seen as component scores determined up to a rotation only .
By applying this transformation it was possible to use the Hill-Smith  method to combine categorical and binary variables to compare all Trypanosoma spp. isolates and strains in a Coinertia analysis [58, 59]. This method is a combination of a multiple correspondence analysis (MCA) for categorical data matrix and MCA rotated to principal component analysis (PCA) for binary data matrix. It was implemented with functions of the ADE-4 package from the R software® [60–62].
PCR amplification of maxicircle genes
Four maxicircle sequences were amplified using either previously reported primers or novel primers designed for this study, based on the complete sequences of the following T. brucei genes: Cytochrome b (cytb-GenBank Accession N° M17998); Cytochrome oxidase Subunit 1 (cox1 -GenBank Accession N° M14820); ATP synthase subunit 6 (a6-GenBank Accession N° M14820); and NADH Dehydrogenase Subunit 8 (nd8 -GenBank Accession N° M63820.1). Primer sequences and PCR conditions are shown in Additional file 2: Table S1. The cytb and cox1 gene amplifications were performed with DNA from all nine Venezuelan isolates, while the a6 and nd8 amplifications were carried out only with DNA from TeAp-N/D1 and TeGu-N/D1.
The cytb, cox1, a6 and nd8 amplicons were purified prior to sequencing using the AccuPrep® PCR Purification Kit (BIONEER®) according to the manufacturer’s instructions. Sequencing of the TeAp-N/D1 genes: cytb [GenBank: KP729379), cox1 [GenBank: KP729381], a6 [GenBank: KP729385] and nd8 [GenBank: KP729383] and the corresponding TeGu-N/D1 genes: cytb [GenBank: KP729380], cox1 [GenBank: KP729386], a6 [GenBank: KP729382] and nd8 [GenBank: KP729384] was performed by Macrogen (Korea) and Unidad de Estudios Genéticos y Forenses (UEGF-Instituto Venezolano de Investigaciones Científicas, Venezuela).
Sequence analysis and alignment
Maxicircle sequences from TeAp-N/D1 and TeGu-N/D1 isolates were compared to the corresponding sequences from T. equiperdum, T. brucei sp. and T. brucei brucei retrieved from the Genbank database. Sequence analysis was performed using nucleotide BLAST and the sequences were aligned by MUSCLE tools. Phylogenetic trees were constructed using Maximum Parsimony (MP) and Maximum Likelihood (ML) with the MEGA5.1® software  using T. cruzi as an outgroup. For the ML method, the evolution of the aligned sequences was analyzed.
We analyzed nine Trypanosoma spp. isolates obtained from two Venezuelan states (Apure and Guárico) and from three different hosts: horses, donkeys and capybara. We previously showed that the RAPDs profile of the TeAp-N/D1 and TeGu-N/D1 isolates (horse) were quite distinct from the other seven Venezuelan isolates . To further characterize these strains, all nine Trypanosoma spp. isolates were genotyped using microsatellites and Procyclin repeats followed by multivariate analysis, and the two that clustered with T. equiperdum (STIB841/OVI), TeAp-N/D1 and TeGu-N/D1, were analyzed for specific maxicircle gene sequences.
The results of the microsatellite and Procyclin PE repeats analysis of the nine Trypanosoma spp. Venezuelan isolates, along with the corresponding data from fifteen T. evansi, three T. equiperdum and eighteen T. b. brucei reference strains are presented in Additional file 1. The Trypanozoon reference strains used in this study originated from Latin America (Colombia and Brazil), Asia (China) and Africa (Chad, Kenya, Ethiopia, Gambia, Ivory Coast, Burkina Faso, Nigeria, Democratic Republic of Congo, Uganda, Tanzania and South Africa).
Five SSR microsatellites and the PE repeats of the PARP genes were used to analyze the nine Venezuelan isolates. The resulting genotypes were compared to reference T. evansi and T. equiperdum strains, as well as to eighteen previously reported T. brucei brucei strains , by coinertia analysis.
Amplification of maxicircle genes
Because the presence of maxicircles is a universally accepted marker to distinguish T. equiperdum from T. evansi, amplification of two maxicircle genes (cytb and cox1), was attempted in the nine Venezuelan Trypanosoma spp. isolates. In agreement with the microsatellite data, no amplification of cytb and cox1 was observed in the seven Venezuelan Trypanosoma spp. isolates that belong to the main T. evansi cluster: TeAp-Cedral05, TeAp-Cedral12, TeGu-Terecay03, TeAp-El Frío01, TeAp-Mantecal01, TeGu-Terecay323 and TeGu-Terecay01. However both cytb and cox1 could be amplified from DNA of the TeAp-N/D1 and TeGu-N/D1 isolates, as were, two additional maxicircle genes, ATP synthase subunit 6 (a6) and NADH dehydrogenase subunit 8 (nd8).
Phylogenetic analysis of four maxicircle genes
Analysis of the sequences of the cytb, cox1, a6 and nd8 genes amplified from the TeAp-N/D1 and TeGu-N/D1 isolates with BLASTn revealed maximum identities between 98 and 99 % to the orthologous genes from T. equiperdum strain STIB842 and BoTat1.1 (Additional file 2: Tables S2-S9). In addition, cox1 from TeAp-N/D1 was 99 % identical to the corresponding gene from T. brucei strain [GenBank: M14820] (Additional file 2: Table S4).
Summary of the Venezuelan T. evansi and T. equiperdum strains characterized in this study
Microsatellite Genotyping and Coinertia analysis
Closely related to T. evansi references strains from South America (Brazil and Colombia) and Asia (China).
Closely related to the T. equiperdum STIB841/ OVI strain
Positive for cytb, cox1, a6 and nd8
Closely related to the T. equiperdum STIB841/OVI strain.
Positive for cytb, cox1, a6 and nd8
The classification of trypanosomes within the Trypanozoon sub-genera was originally based on morphological and morphometrical criteria, as well as clinical manifestations, host range and geographical distribution. In the last several years, molecular markers such as microsatellite loci and sequence analysis of the rRNA and gGAPDH genes have been used to describe the evolutionary relationships among organisms. This has led to the re-evaluation of what constitutes a trypanosome species [5, 34, 64, 65]. The lack of maxicircle genes in T. evansi has been used to differentiate it from T. equiperdum , both being considered as petite mutants of T. brucei . Subtle genomic changes were found between the akinetoplastic strain T. evansi STIB805 and the T. b. brucei TREU 927/4 strain, supporting the view that T. evansi should be considered a subspecies of T. brucei . The species or subspecies status of both T. evansi and T. equiperdum has been debated by several authors and continues to be polemical [4, 16, 51, 66, 67].
Using RAPD analysis, we previously showed that nine Venezuelan Trypanosoma spp. isolates cluster into two separate groups, one with seven isolates that share a similar genetic pattern and a second, distinct group of two horse isolates, TeAp-N/D1 and TeGu-N/D1 that appeared identical except with one of the forty random primers . Since these nine Venezuelan Trypanosoma spp. isolates were presumed to belong to the Trypanozoon group, we used microsatellites markers and PARP-PE repeats to compare them to T. evansi and T. equiperdum reference strains. These loci exhibited limited polymorphism among seven of our isolates and the T. evansi reference strains from various hosts, horse, dog, coati, bovine, buffalo, mule and camels and geographical origins, South America, Asia and Africa. However, the microsatellite analysis clearly clustered two of the Venezuelan Trypanosoma spp. horse isolates with the T. equiperdum STIB841/OVI strain from South Africa.
Coinertia analysis of the microsatellite and PE repeats revealed that seven of the nine Venezuelan isolates closely match eleven T. evansi reference strains from around the world, while TeAp-N/D1 and TeGu-N/D1 are identical to the South African T. equiperdum STIB841/OVI strain. Principal Component Analysis (PCA) of microsatellite markers showed that this T. equiperdum strain is closely related to the T. brucei brucei Kiboko group . In agreement with previous studies of Trypanozoon microsatellite loci , our coinertia analysis showed that BoTat-1.1 and BJ were highly heterogeneous T. equiperdum strains, genetically distant from the group that included the two Venezuelan T. equiperdum strains and STIB841/OVI. Four independent T. evansi/T. equiperdum genotypes have been recently described by Carnes et al . They classified two of the reference T. equiperdum strains included in this study, BoTat-1.1 (Teq21) and STIB841/OVI, within groups 2 and 3, respectively.
Since T. equiperdum is distinguished from T. evansi by the presence of partially deleted maxicircles [14, 51, 67], we amplified and sequenced maxicircle genes from the TeAp-N/D1 and TeGu-N/D1 isolates and analyzed the resulting phylogenetic relationships. In agreement with previous reports, the two Venezuelan T. equiperdum strains analyzed in this study, TeAp-N/D1 and TeGu-N/D1, have retained at least four maxicircle genes . ND8 and A6 constitute complexes I and V of the oxidative phosphorylation system, and their expression is essential in the T. brucei bloodstream form [68, 69], as is the expression of cytb . A6 is important for maintaining the mitochondrial membrane potential and several mutations that affect its function have been described in diskinetoplastic trypanosomes [71–73]. Mitochondrial genes have been proposed as excellent molecular markers for discriminating closely related species [74–76]. The four maxicircle genes from the TeAp-N/D1 and TeGu-N/D1 isolates revealed a close relationship to both T. brucei and T. equiperdum strains. The phylogenetic analysis of cox1 gene sequences is concordant with the four distinct groups of T. evansi and T. equiperdum strains that suggest four independent origins of these diskinetoplastic parasites . Interestingly, while the microsatellite loci and Procyclin PE repeats and coinertia analyses showed identical genotypes for TeAp-N/D1 and TeGu-N/D1, the cox1 and a6 mitochondrial markers separated them into different clusters. These results confirm the first molecular report of T. equiperdum strains (TeAp-N/D1 and TeGu-N/D1) isolated in Venezuela or in any part of Latin America.
Interestingly, T. equiperdum is not a typical American parasite but dourine, a sexually transmitted chronic disease in horses, mules and donkeys [5, 17], has been sporadically reported in the American continent from Canada (1921) to the USA (1934) and Mexico (1973) . In Venezuela, clinical dourine was first recorded by the presence of dourine plaques in a domestic male horse, but no parasites were observed . The actual geographical distribution of dourine is not known and trade restrictions appear to limit notification of the disease. The disease was widespread in the past but was eradicated from many countries of Europe after the 1940s [22, 79]. Currently, the disease is endemic in parts of Africa, Asia and Russia, and dourine outbreaks or incidents have been occasionally reported in the Middle East and Europe [16, 80–82]. However, dourine may exist in areas where diagnostic tests are not routinely performed [3, 17]. In 2011, seven dourine outbreaks were confirmed in various regions of Italy [18–21, 83], all linked to the movement of breeding animals showing the characteristic plaques and lesions. The presence of T. equiperdum was confirmed by RT-PCR.
T. equiperdum is morphologically indistinguishable from T. evansi and T. brucei, [5, 17]. T. evansi was initially proposed to have evolved from an ancestral T. brucei when infected camels were introduced to Glossina-free areas [5, 14] and is characterized by the absence of maxicircle structures [45, 84]. Several years ago, Claes et al  proposed that T. equiperdum does not exist as a separate species and that extant strains are either T.b. equiperdum, or misidentified T.b. brucei or T. evansi strains. Based on genetic analysis, other authors have also proposed that T. evansi and T. equiperdum should be considered sub-species of T. brucei [16, 17, 51, 65, 66]. In contrast, Desquesnes et al  recommend keeping the current species status for T. evansi and T. equiperdum, in agreement with the rules of the international code for zoological nomenclature and based on their significant biological differences. Further genomic analysis of the two Venezuelan T. equiperdum strains should shed new light on the evolution, origin and pathogenic effects of these trypanosomes.
The evolution of T. evansi and T. equiperdum has been revisited in recent years. Lun et al  proposed two sequential steps in the spreading of T. brucei out of Africa, the first involved the homogenization of minicircles in the T. b. brucei bloodstream form and the loss of the ability to differentiate within the insect vector, resulting in T. b. equiperdum. Over generations, the gradual loss of maxicircles occurred due to the lack of selective pressure to preserve them, giving rise to T. b. equiperdum and eventually T. b. evansi, which lacks all maxicircles. An alternative model proposed that an ancestral trypanosome lost maxicircle genes in three  or four independent occasions , to generate stable diskinetoplastic forms, a loss that is compensated by distinct mutations on the ATP synthase γ-subunit . A third, alternative hypothesis proposes that T. b. evansi and T. b. equiperdum underwent separate evolutionary processes from a T. b. brucei ancestor . Our results are quite consistent with the existence of partially distinct evolutionary lineages, with the two new Venezuelan T. equiperdum strains, TeAp-N/D1 and TeGu-N/D1 corresponding to the recently proposed T. equiperdum groups 1 and 3, respectively .
FONACIT No 2004000400 RIDMOH, G-98003462, Misión Ciencia 2007001425, Ecos Nord PI-2008002104, TRYPADVAC2 No. 003716, GID21-USB, Instituto Venezolano de Investigaciones Científicas (IVIC) No 305. We thank Howard Takiff for critically reading and editing of the manuscript.
Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.
- Stevens JR, Brisse S. Systematics of Trypanosomes of medical and veterinary importance. In: Maudlin I, Holmes PH, Miles MA, editors. The Trypanosomiases. Oxfordshire: CABI Publishing; 2004. p. 1–23.View ArticleGoogle Scholar
- Luckins AG, Dwinger RH. Non-tsetse-transmitted Animal Trypanosomiasis. In: Maudlin I, Holmes PH, Miles MA, editors. The Trypanosomiases. Oxfordshire: CABI Publishing; 2004. p. 269–81.View ArticleGoogle Scholar
- Desquesnes M. Trypanosomes and Diagnosis. In: Livestock Trypanosomoses and their Vectors in Latin America. Paris, France: Office International des Epizooties; 2004. p. 15–21. 65-83.Google Scholar
- Desquesnes M, Holzmuller P, Lai DH, Dargantes A, Lun ZR, Jittaplapong S. Trypanosoma evansi and Surra: A Review and Perspectives on Origin, History, Distribution, Taxonomy, Morphology, Hosts, and Pathogenic Effects. BioMed Res Int. 2013;1–20.Google Scholar
- Hoare CA. The Trypanosomes of mammals. A zoological monograph. Oxford: Blackwell Scientific Publications; 1972.Google Scholar
- Canelón JL, Meléndez RD. Posible Origen del Trypanosoma evansi en Venezuela. Vet Tropica. 2003;28(2):155–67.Google Scholar
- Silva-Iturriza A, Nassar JM, Garcia-Rawlins AM, Rosales R, Mijares A. Trypanosoma evansi kDNA minicircle found in the Venezuelan nectar-feeding bat Leptonycteris curasoae (Glossophaginae), supports the hypothesis of multiple origins of that parasite in South America. Parasitol Int. 2013;62(2):95–9.View ArticlePubMedGoogle Scholar
- Levine ND. Tratado de Parasitología Veterinaria. Zaragoza: Editorial Acribia; 1983.Google Scholar
- Villareal MV, Mingala CN, Rivera WL. Molecular characterization of Trypanosoma evansi isolates from water buffaloes (Bubalus bubalis) in the Philippines. Acta Parasitol. 2013;58(1):6–12.View ArticlePubMedGoogle Scholar
- Desquesnes M, Dargantes A, Lai DH, Lun ZR, Holzmuller P, Jittapalapong S. Trypanosoma evansi and Surra: A Review and Perspectives on Transmission, Epidemiology and Control, Impact, and Zoonotic Aspects. BioMed Res Int. 2013;2013:321237.PubMed CentralPubMedGoogle Scholar
- Desquesnes M, Bossard G, Thevenon S, Patrel D, Ravel S, Pavlovic D, et al. Development and application of an antibody-ELISA to follow up a Trypanosoma evansi outbreak in a dromedary camel herd in France. Vet Parasitol. 2009;162(3-4):214–20.View ArticlePubMedGoogle Scholar
- Gutierrez C, Desquesnes M, Touratier L, Buscher P. Trypanosoma evansi: recent outbreaks in Europe. Vet Parasitol. 2010;174(1-2):26–9.View ArticlePubMedGoogle Scholar
- Defontis M, Richartz J, Engelmann N, Bauer C, Schwierk VM, Buscher P, et al. Canine Trypanosoma evansi infection introduced into Germany. Vet Clin Pathol. 2012;41(3):369–74.View ArticlePubMedGoogle Scholar
- Brun R, Hecker H, Lun ZR. Trypanosoma evansi and T. equiperdum: distribution, biology, treatment and phylogenetic relationship (a review). Vet. Parasitol. 1998;79(2):95–107.Google Scholar
- Gibson W, Miles M. Frontiers in research on parasitic protozoa. Trends Parasitol. 2002;18(12):521–2.View ArticlePubMedGoogle Scholar
- Claes F, Buscher P, Touratier L, Goddeeris BM. Trypanosoma equiperdum: master of disguise or historical mistake? Trends Parasitol. 2005;21(7):316–21.View ArticlePubMedGoogle Scholar
- Wei Y, Wen Y-Z., Desquesnes, M., Lun, Z-R. Molecular Epidemiology of Trypanosoma evansi and T. equiperdum and Atypical Human Infection by Animal Trypanosomes. In: The Molecular Epidemiology of Trypanosomes and Leishmania. NY, NY 10013, USA: Geoff Hide; 2011: p. 1-14Google Scholar
- Scacchia M, Camma C, Di Francesco G, Di Provvido A, Giunta R, Luciani M, et al. A clinical case of dourine in an outbreak in Italy. Vet Ital. 2011;47(4):473–5. 469-472.PubMedGoogle Scholar
- Calistri P, Narcisi V, Atzeni M, De Massis F, Tittarelli M, Mercante MT, et al. Dourine Reemergence in Italy. J Equine Vet Sci. 2013;33(2):83–9.View ArticleGoogle Scholar
- Pascucci I, Di Provvido A, Camma C, Di Francesco G, Calistri P, Tittarelli M, et al. Diagnosis of dourine in outbreaks in Italy. Vet Parasitol. 2013;193(1-3):30–8.View ArticlePubMedGoogle Scholar
- Vulpiani MP, Carvelli A, Giansante D, Iannino F, Paganico D, Ferri N. Reemergence of Dourine in Italy: Clinical Cases in Some Positive Horses. J Equine Vet Sci. 2013;33(6):468–74.View ArticleGoogle Scholar
- CFSPH and IICAB. http://www.cfsph.iastate.edu/Factsheets/pdfs/dourine.pdf (2009). Accessed 01 April 2015.
- Hide G, Cattand P, LeRay D, Barry JD, Tait A. The identification of Trypanosoma brucei subspecies using repetitive DNA sequences. Mol Biochem Parasitol. 1990;39(2):213–25.View ArticlePubMedGoogle Scholar
- Haag J, O'hUigin C, Overath P. The molecular phylogeny of trypanosomes: evidence for an early divergence of the Salivaria. Mol Biochem Parasitol. 1998;91(1):37–49.View ArticlePubMedGoogle Scholar
- Stevens JR, Gibson W. The molecular evolution of trypanosomes. Parasitol Today. 1999;15(11):432–7.View ArticlePubMedGoogle Scholar
- Stevens JR, Noyes HA, Schofield CJ, Gibson W. The molecular evolution of Trypanosomatidae. Adv Parasitol. 2001;48:1–56.View ArticlePubMedGoogle Scholar
- Hamilton PB, Adams ER, Malele, II, Gibson WC. A novel, high-throughput technique for species identification reveals a new species of tsetse-transmitted trypanosome related to the Trypanosoma brucei subgenus, Trypanozoon. Infect. Genet. Evol. 2008; doi:10.1016/j.meegid.2007.09.003
- Boid R. Isoenzyme characterisation of 15 stocks of Trypanosoma evansi isolated from camels in the Sudan. Trop Med Parasitol. 1988;39(1):45–50.PubMedGoogle Scholar
- Stevens JR, Nunes VL, Lanham SM, Oshiro ET. Isoenzyme characterization of Trypanosoma evansi isolated from capybaras and dogs in Brazil. Acta Trop. 1989;46(4):213–22.View ArticlePubMedGoogle Scholar
- Queiroz AO, Cabello PH, Jansen AM. Biological and biochemical characterization of isolates of Trypanosoma evansi from Pantanal of Matogrosso--Brazil. Vet Parasitol. 2000;92(2):107–18.View ArticlePubMedGoogle Scholar
- Paindavoine P, Pays E, Laurent M, Geltmeyer Y, Le Ray D, Mehlitz D, et al. The use of DNA hybridization and numerical taxonomy in determining relationships between Trypanosoma brucei stocks and subspecies. Parasitology. 1986;92(Pt 1):31–50.View ArticlePubMedGoogle Scholar
- Mathieu-Daude F, Bicart-See A, Bosseno MF, Breniere SF, Tibayrenc M. Identification of Trypanosoma brucei gambiense group I by a specific kinetoplast DNA probe. Am J Trop Med Hyg. 1994;50(1):13–9.PubMedGoogle Scholar
- Li FJ, Gasser RB, Lai DH, Claes F, Zhu XQ, Lun ZR. PCR approach for the detection of Trypanosoma brucei and T. equiperdum and their differentiation from T. evansi based on maxicircle kinetoplast DNA. Mol. Cell Probes. 2007; doi:10.1016/j.mcp.2006.03.009
- Biteau N, Bringaud F, Gibson W, Truc P, Baltz T. Characterization of Trypanozoon isolates using a repeated coding sequence and microsatellite markers. Mol Biochem Parasitol. 2000;105(2):187–202.View ArticlePubMedGoogle Scholar
- Weber JL. Informativeness of human (dC-dA)n. (dG-dT)n polymorphisms. Genomics. 1990;7(4):524–30.View ArticlePubMedGoogle Scholar
- Valadares HM, Pimenta JR, de Freitas JM, Duffy T, Bartholomeu DC, Oliveira Rde P et al. Genetic profiling of Trypanosoma cruzi directly in infected tissues using nested PCR of polymorphic microsatellites. Int. J. Parasitol. 2008; doi:10.1016/j.ijpara.2007.10.017
- Weber JL, Wong C. Mutation of Human Short Tandem Repeats. Hum. Mol. Genet. 1993; doi: 10.1093/Hmg/2.8.1123
- Hughes CR, Queller DC. Detection of highly polymorphic microsatellite loci in a species with little allozyme polymorphism. Mol Ecol. 1993;2(3):131–7.View ArticlePubMedGoogle Scholar
- Jenni L, Marti S, Schweizer J, Betschart B, Lepage RWF, Wells JM et al. Hybrid Formation between African Trypanosomes during Cyclical Transmission. Nature. 1986; doi: 10.1038/322173a0
- Capewell P, Cooper A, Duffy CW, Tait A, Turner CM, Gibson W et al. Human and animal Trypanosomes in Cote d'Ivoire form a single breeding population. PLoS One. 2013; doi:10.1371/journal.pone.0067852
- Simo G, Sobgwi PF, Njitchouang GR, Njiokou F, Kuiate JR, Cuny G et al. Identification and genetic characterization of Trypanosoma congolense in domestic animals of Fontem in the South-West region of Cameroon. Infect. Genet. Evol. 2013; doi:10.1016/j.meegid.2013.04.019
- Yurchenko V, Kolesnikov AA. Minicircular kinetoplast DNA from Trypanosomatidae. Mol Biol. 2001;35:3–13.View ArticleGoogle Scholar
- Pollard VW, Rohrer SP, Michelotti EF, Hancock K, Hajduk SL. Organization of minicircle genes for guide RNAs in Trypanosoma brucei. Cell. 1990;63(4):783–90.View ArticlePubMedGoogle Scholar
- Borst P, Fase-Fowler F, Gibson WC. Kinetoplast DNA of Trypanosoma evansi. Mol Biochem Parasitol. 1987;23(1):31–8.View ArticlePubMedGoogle Scholar
- Ou YC, Giroud C, Baltz T. Kinetoplast DNA analysis of four Trypanosoma evansi strains. Mol Biochem Parasitol. 1991;46(1):97–102.View ArticlePubMedGoogle Scholar
- Songa EB, Paindavoine P, Wittouck E, Viseshakul N, Muldermans S, Steinert M, et al. Evidence for kinetoplast and nuclear DNA homogeneity in Trypanosoma evansi isolates. Mol Biochem Parasitol. 1990;43(2):167–79.View ArticlePubMedGoogle Scholar
- Lun ZR, Brun R, Gibson W. Kinetoplast DNA and molecular karyotypes of Trypanosoma evansi and Trypanosoma equiperdum from China. Mol Biochem Parasitol. 1992;50(2):189–96.View ArticlePubMedGoogle Scholar
- Myler PJ. Molecular variation in trypanosomes. Acta Trop. 1993;53(3-4):205–25.View ArticlePubMedGoogle Scholar
- Borst P, Fase-Fowler F. The maxi-circle of Trypanosoma brucei kinetoplast DNA. Biochim Biophys Acta. 1979;565(1):1–12.View ArticlePubMedGoogle Scholar
- Clayton CE, Michels P. Metabolic compartmentation in African trypanosomes. Parasitol Today. 1996;12(12):465–71.View ArticlePubMedGoogle Scholar
- Lai DH, Hashimi H, Lun ZR, Ayala FJ, Lukes J. Adaptations of Trypanosoma brucei to gradual loss of kinetoplast DNA: Trypanosoma equiperdum and Trypanosoma evansi are petite mutants of T. brucei. Proc. Natl. Acad. Sci. U. S. A. 2008; doi:10.1073/pnas.0711799105
- Perrone TM, Gonzatti MI, Villamizar G, Escalante A, Aso PM. Molecular profiles of Venezuelan isolates of Trypanosoma sp. by random amplified polymorphic DNA method. Vet. Parasitol. 2009; doi:10.1016/j.vetpar.2009.01.034
- Holzmuller P, Grebaut P, Peltier JB, Brizard JP, Perrone T, Gonzatti M et al. Secretome of animal trypanosomes. Ann. N. Y. Acad. Sci. 2008; doi:10.1196/annals.1428.097
- Lanham SM, Godfrey DG. Isolation of salivarian trypanosomes from man and other mammals using DEAE-cellulose. Exp Parasitol. 1970;28(3):521–34.View ArticlePubMedGoogle Scholar
- COBIANIM: The COBIANIM register. http://www.ivic.gob.ve/cobianim/. Accessed 30 May 2015.
- Kiers HAL. Simple Structure in Component Analysis Techniques for Mixtures of Qualitative and Quantitative Variables. Psychometrika. 1991;56(2):197–212. doi:10.1007/Bf02294458.View ArticleGoogle Scholar
- Hill MO, Smith AJE. Principal Component Analysis of Taxonomic Data with Multistate Discrete Characters. Taxon. 1976; doi:10.2307/1219449
- Doledec S, Chessel D. Coinertia Analysis - an Alternative Method for Studying Species Environment Relationships. Freshwater Biol. 1994; doi:10.1111/j.1365-2427.1994.tb01741.x
- Dray S, Chessel D, Thioulouse J. Coinertia analysis and the linking of ecological data tables. Ecology. 2003; doi:10.1890/03-0178
- Chessel D, Dufour AB, Thioulouse J. The ade4 package-I- One-table methods. R News. 2004;4:5–10.Google Scholar
- Dray S, Dufour AB. The ade4 package: Implementing the duality diagram for ecologists. J Stat Softw. 2007;22(4):1–20.View ArticleGoogle Scholar
- Dray S, Dufour AB, Chessel D. The ade4 package-II: Two-table and K-table methods. R News. 2007;7(2):47–52.Google Scholar
- Tamura K, Peterson D, Peterson N, Stecher G, Nei M, Kumar S. MEGA5: molecular evolutionary genetics analysis using maximum likelihood, evolutionary distance, and maximum parsimony methods. Mol. Biol. Evol. 2011; doi:10.1093/molbev/msr121
- Gibson W. Resolution of the species problem in African trypanosomes. Int. J. Parasitol. 2007; doi:10.1016/j.ijpara.2007.03.002
- Hamilton PB, Gibson WC, Stevens JR. Patterns of co-evolution between trypanosomes and their hosts deduced from ribosomal RNA and protein-coding gene phylogenies. Mol. Phylogenet. Evol. 2007; doi:10.1016/j.ympev.2007.03.023
- Carnes J, Anupama A, Balmer O, Jackson A, Lewis M, Brown R et al. Genome and phylogenetic analyses of trypanosoma evansi reveal extensive similarity to T. brucei and multiple independent origins for dyskinetoplasty. PLoS Negl. Trop. Dis. 2015; doi:10.1371/journal.pntd.0003404
- Lun ZR, Lai DH, Li FJ, Lukes J, Ayala FJ. Trypanosoma brucei: two steps to spread out from Africa. Trends. Parasitol. 2010; doi:10.1016/j.pt.2010.05.007
- Bhat GJ, Koslowsky DJ, Feagin JE, Smiley BL, Stuart K. An extensively edited mitochondrial transcript in kinetoplastids encodes a protein homologous to ATPase subunit 6. Cell. 1990;61(5):885–94.View ArticlePubMedGoogle Scholar
- Souza AE, Myler PJ, Stuart K. Maxicircle CR1 transcripts of Trypanosoma brucei are edited and developmentally regulated and encode a putative iron-sulfur protein homologous to an NADH dehydrogenase subunit. Mol Cell Biol. 1992;12(5):2100–7.PubMed CentralView ArticlePubMedGoogle Scholar
- Feagin JE, Jasmer DP, Stuart K. Developmentally regulated addition of nucleotides within apocytochrome b transcripts in Trypanosoma brucei. Cell. 1987;49(3):337–45.View ArticlePubMedGoogle Scholar
- Schnaufer A, Domingo GJ, Stuart K. Natural and induced dyskinetoplastic trypanosomatids: how to live without mitochondrial DNA. Int J Parasitol. 2002;32(9):1071–84.View ArticlePubMedGoogle Scholar
- Jensen RE, Simpson L, Englund PT. What happens when Trypanosoma brucei leaves Africa. Trends. Parasitol. 2008; 24(10): doi:10.1016/j.pt.2008.06.007.
- Dean S, Gould MK, Dewar CE, Schnaufer AC. Single point mutations in ATP synthase compensate for mitochondrial genome loss in trypanosomes. Proc. Natl. Acad. Sci. U. S. A. 2013; doi:10.1073/pnas.1305404110.80
- Blair D, Agatsuma T, Watanobe T, Okamoto M, Ito A. Geographical genetic structure within the human lung fluke, Paragonimus westermani, detected from DNA sequences. Parasitology. 1997;115(Pt 4):411–7.View ArticlePubMedGoogle Scholar
- Morgan JA, Blair D. Relative merits of nuclear ribosomal internal transcribed spacers and mitochondrial CO1 and ND1 genes for distinguishing among Echinostoma species (Trematoda). Parasitology. 1998;116(Pt 3):289–97.View ArticlePubMedGoogle Scholar
- Mas-Coma S, Bargues MD. Populations, hybrids and the systematic concepts of species and subspecies in Chagas disease triatomine vectors inferred from nuclear ribosomal and mitochondrial DNA. Acta Trop. 2009;110(2-3):112–36.View ArticlePubMedGoogle Scholar
- OIE: The OIE register. http://web.oie.int/hs2/sit_mald_cont.asp?c_mald=60&c_cont=2. Accessed 10 April 2015.
- Rivas-Larralde G. Un caso de durina en Venezuela. Revista de Medicina Veterinaria y Parasitología. 1939;1:192.Google Scholar
- Caporale VP, Battelli G, Semproni G. Epidemiology of dourine in the equine population of the Abruzzi Region. Zentralbl Veterinarmed B. 1980;27(6):489–98.View ArticlePubMedGoogle Scholar
- Zablotskij VT, Georgiu C, de Waal T, Clausen PH, Claes F, Touratier L. The current challenges of dourine: difficulties in differentiating Trypanosoma equiperdum within the subgenus Trypanozoon. Rev Sci Tech. 2003;22(3):1087–96.PubMedGoogle Scholar
- Gari FR, Ashenafi H, Tola A, Goddeeris BM, Claes F. Comparative diagnosis of parasitological, serological, and molecular tests in dourine-suspected horses. Trop. Anim. Health Prod. 2010; doi:10.1007/s11250-010-9615-1
- Hagos A, Degefa G, Yacob H, Fikru R, Alemu T, Feseha G, et al. Seroepidemiological survey of trypanozoon infection in horses in the suspected dourine-infected Bale highlands of the Oromia region, Ethiopia. Rev Sci Tech. 2010;29(3):649–54.PubMedGoogle Scholar
- OIE: The OIE register. http://www.oie.int/fileadmin/Home/fr/Health_standards/tahm/2.05.03_DOURINE.pdf. Accessed 01 April 2015.
- Lun ZR, Desser SS. Is the broad range of hosts and geographical distribution of Trypanosoma evansi attributable to the loss of maxicircle kinetoplast DNA? Parasitol. Today. 1995; doi:10.1016/0169-4758(95)80129-4
- Schnaufer A. Evolution of dyskinetoplastic trypanosomes: how, and how often? Trends Parasitol. 2010; doi:10.1016/j.pt.2010.08.001
- Gibson WC, de C Marshall TF, Godfrey DG. Numerical analysis of enzyme polymorphism: a new approach to the epidemiology and taxonomy of trypanosomes of the subgenus Trypanozoon. Adv Parasitol. 1980;18:175–246.View ArticlePubMedGoogle Scholar
- Zhang ZQ, Baltz T. Identification of Trypanosoma evansi, Trypanosoma equiperdum and Trypanosoma brucei brucei using repetitive DNA probes. Vet Parasitol. 1994;53(3-4):197–208.View ArticlePubMedGoogle Scholar
- Gibson WC, Wilson AJ, Moloo SK. Characterisation of Trypanosoma (Trypanozoon) evansi from camels in Kenya using isoenzyme electrophoresis. Res Vet Sci. 1983;34(1):114–8.PubMedGoogle Scholar
- Stevens JR, Lanham SM, Allingham R, Gashumba JK. A simplified method for identifying subspecies and strain groups in Trypanozoon by isoenzymes. Ann Trop Med Parasitol. 1992;86(1):9–28.PubMedGoogle Scholar
- Gillingwater K, Buscher P, Brun R. Establishment of a panel of reference Trypanosoma evansi and Trypanosoma equiperdum strains for drug screening. Vet. Parasitol. 2007; doi:10.1016/j.vetpar.2007.05.020
- Baltz T, Baltz D, Giroud C, Crockett J. Cultivation in a semi-defined medium of animal infective forms of Trypanosoma brucei, T. equiperdum, T. evansi, T. rhodesiense and T. gambiense. EMBO J. 1985;4(5):1273–7.PubMed CentralPubMedGoogle Scholar