Research Article

Comparative Microsatellite Typing of New World Leishmania infantum Reveals Low Heterogeneity among Populations and Its Recent Old World Origin

  • Katrin Kuhls mail,

    Affiliation: Institut für Mikrobiologie und Hygiene, Charité Universitätsmedizin Berlin, Berlin, Germany

  • Mohammad Zahangir Alam,

    Affiliation: Institut für Mikrobiologie und Hygiene, Charité Universitätsmedizin Berlin, Berlin, Germany

    Current address: Department of Parasitology, Bangladesh Agricultural University, Mymensingh, Bangladesh

  • Elisa Cupolillo,

    Affiliation: Laboratório de Pesquisa em Leishmaniose, Instituto Oswaldo Cruz - Fiocruz, Rio de Janeiro, Brazil

  • Gabriel Eduardo M. Ferreira,

    Affiliation: Laboratório de Biologia Molecular de Insetos, Instituto Oswaldo Cruz - Fiocruz, Rio de Janeiro, Brazil

  • Isabel L. Mauricio,

    Affiliation: Department of Pathogen Molecular Biology, Faculty of Infectious and Tropical Diseases, London School of Hygiene and Tropical Medicine, London, United Kingdom

    Current address: Instituto de Higiene e Medicina Tropical, Lisboa, Portugal

  • Rolando Oddone,

    Affiliation: Instituto de Investigaciones en Ciencias de la Salud, Universidad Nacional de Asuncion, Asuncion, Paraguay

  • M. Dora Feliciangeli,

    Affiliation: Universidad de Carabobo, BIOMED-Centro Nacional de Referencia de Flebotomos de Venezuela, UC-BIOMED-CNRFV, Maracay, Venezuela

  • Thierry Wirth,

    Affiliation: Département de Systématique et Évolution, Ecole Pratique des Hautes Etudes, Muséum National d'Histoire Naturelle, UMR-CNRS 5202, Paris, France

  • Michael A. Miles,

    Affiliation: Department of Pathogen Molecular Biology, Faculty of Infectious and Tropical Diseases, London School of Hygiene and Tropical Medicine, London, United Kingdom

  • Gabriele Schönian

    Affiliation: Institut für Mikrobiologie und Hygiene, Charité Universitätsmedizin Berlin, Berlin, Germany

  • Published: June 07, 2011
  • DOI: 10.1371/journal.pntd.0001155


Leishmania infantum (syn. L. chagasi) is the causative agent of visceral leishmaniasis (VL) in the New World (NW) with endemic regions extending from southern USA to northern Argentina. The two hypotheses about the origin of VL in the NW suggest (1) recent importation of L. infantum from the Old World (OW), or (2) an indigenous origin and a distinct taxonomic rank for the NW parasite. Multilocus microsatellite typing was applied in a survey of 98 L. infantum isolates from different NW foci. The microsatellite profiles obtained were compared to those of 308 L. infantum and 20 L. donovani strains from OW countries previously assigned to well-defined populations. Two main populations were identified for both NW and OW L. infantum. Most of the NW strains belonged to population 1, which corresponded to the OW MON-1 population. However, the NW population was much more homogeneous. A second, more heterogeneous, population comprised most Caribbean strains and corresponded to the OW non-MON-1 population. All Brazilian L. infantum strains belonged to population 1, although they represented 61% of the sample and originated from 9 states. Population analysis including the OW L. infantum populations indicated that the NW strains were more similar to MON-1 and non-MON-1 sub-populations of L. infantum from southwest Europe, than to any other OW sub-population. Moreover, similarity between NW and Southwest European L. infantum was higher than between OW L. infantum from distinct parts of the Mediterranean region, Middle East and Central Asia. No correlation was found between NW L. infantum genotypes and clinical picture or host background. This study represents the first continent-wide analysis of NW L. infantum population structure. It confirmed that the agent of VL in the NW is L. infantum and that the parasite has been recently imported multiple times to the NW from southwest Europe.

Author Summary

Leishmaniasis is a vector borne disease with a broad spectrum of clinical forms caused by protozoan parasites of the genus Leishmania. Visceral leishmaniasis is the most severe, systemic form of the disease. It is caused by parasites belonging to the Leishmania donovani complex, which includes L. infantum and L. donovani in the Old World (OW) and L. infantum (syn. L. chagasi) in the New World (NW). The identity and origin of the causative agent of VL in the Americas have been the subjects of much debate for decades. Different scientific approaches led to different conclusions, either favouring the hypothesis of indigenous origin of this parasite and its status as distinct species, or a recent importation of L. infantum by European colonists and synonymy of L. infantum and L. chagasi. We performed the first broad population study of these parasites from the NW using highly variable microsatellite markers. The level of heterogeneity and population structure was very low in contrast to the OW. Using a combined data analysis of NW and OW strains we have provided conclusive evidence of recent multiple introductions of L. infantum from Southwest Europe into the New World and for synonymy of L. infantum and L. chagasi.


In 1937 the causative agent of visceral leishmaniasis (VL) in the New World (also referred to as American visceral leishmaniasis – AVL) was designated as a distinct species, Leishmania (L.) chagasi Cunha & Chagas [1]. Many studies have subsequently concluded that the causative agent is indistinguishable from L. infantum, derived from Europe [2][4]. To explore the molecular epidemiology of AVL, we have applied a high resolution population genetic analysis to a vast collection of New World (NW) and Old World (OW) isolates.

Visceral leishmaniasis in the New World extends from the southern parts of the USA [5], [6] and Mexico to the North of Argentina, including countries such as Brazil, Paraguay, Bolivia, Venezuela, Suriname, Guyana, Colombia, Honduras, Panama, Costa Rica, El Salvador, Guadeloupe, Guatemala, and Nicaragua [7][11]. Brazil is the country that accounts for the highest number (~90%) of cases [12], [13]. The principal foci are located in drier, poorly forested areas, although there are several foci in the densely forested Amazon region and the Guianan Ecoregion Complex (GEC), which covers some States of Venezuela and all of Guyana, Suriname and French Guiana and the upper parts of the Brazilian states Amazonas, Roraima, Pará, and Amapá. The main foci here are in Pará, Roraima (Brazil), Bolivar (Venezuela) and parts of Guyana. There are few cases reported from Suriname and no cases from French Guiana except a recently imported canine case [14][17].

To a lesser extent, NW L. infantum also causes atypical cutaneous leishmaniasis (atypical CL). This clinical manifestation has been reported since the 1970s mainly from Caribbean countries such as Venezuela, Honduras, Costa Rica, Nicaragua, but sporadically also from Brazil [18][23]. Except in Brazil, atypical CL cases are characterised by non-ulcerative skin lesions that are often misidentified as nodular infantile tuberculoid leprosy. Host immuno-genetic factors and/or parasite factors in combination with socio-economical and environmental factors are likely to play a role in determining the varied clinical picture, as in the case of Mediterranean L. infantum infections.

In the NW, domestic dogs are primary reservoirs of infection for humans, but foxes (Cerdocyon thous), native marsupials (Didelphis marsupialis, D. albiventris) and rodents (e.g. domestic rats) have also been found infected not only in urban areas but also in the Amazonian region [11], [14], [15]. The sand fly Lutzomyia longipalpis is the primary vector of L. infantum in the NW [12], [15], however, differences in the sand fly populations [24][28] and perhaps also the involvement of other sand fly species (e.g. Lu. evansi) [11],[15],[29],[30] may contribute to the variable clinical manifestations of the disease seen in different geographic regions.

Taxonomically NW L. infantum (syn. L. chagasi) belongs to the L. donovani species complex of the subgenus Leishmania Ross 1903, which in addition includes L. infantum and L. donovani from the OW [7]. There are two different hypotheses on the origin of NW L. infantum, of which the first one is now widely accepted: (1) L. infantum has been imported from Europe during the Spanish and Portuguese colonization carried by dogs or rats, and (2) L. chagasi is indigenous to the Americas [8], [31][36]. As summarized by Dantas-Torres [34], [35] these two hypotheses have led to much confusion regarding the nomenclature and at least 6 different nomenclatures are used in the literature. Until now, there have been no extensive studies of the population structure of NW L. infantum with a reasonable number of strains from different regions, environments, hosts and reservoirs and, therefore the taxonomic status of NW L. infantum is still not clear.

To detect structure of Leishmania populations it is essential to use a typing method with a high discriminatory potential. Many previously used methods were not adequate for discriminating at this taxonomic level. One of the most powerful and discriminative DNA-based methods for strain differentiation and population genetics is the analysis of highly variable, co-dominant microsatellite markers. Recently, multilocus microsatellite typing (MLMT) has been used successfully to differentiate L. infantum populations in the Mediterranean region of Europe and North Africa, the Middle East and Uzbekistan [4], [37][41] as well as L. donovani populations in the Indian subcontinent and East Africa [42], [43]. This method enabled differentiation even at the intra-zymodeme level, as shown for the predominant MON-1 zymodeme of L. infantum.

In the present study we have applied MLMT for an extensive population survey of NW L. infantum originating mainly from different endemic regions within Brazil, but also from other countries. To our knowledge this is the first comprehensive study of population structure of L. infantum in the NW. We show that NW L. infantum, indeed, was introduced on multiple occasions in recent times from European source populations of L. infantum and is inseparable from them. We also provide substantial new insight into the molecular epidemiology of AVL.

Materials and Methods

Parasite cultures and DNA extraction

Sources, designation, geographical origins, MLEE identification, if known, and clinical manifestation for the 426 studied strains, including NW L. infantum, OW L. infantum and L. donovani are listed in Table S1. NW L. infantum was represented by 98 strains from Brazil, Paraguay, Colombia, Venezuela, Honduras, Panama, and Costa Rica (Figure 1A, Table 1). Most NW L. infantum came from Brazil and Figure 1B shows the number of strains used from the respective Brazilian endemic regions. Figure 1C depicts the percentages of NW L. infantum strains causing different clinical pictures. The 308 L. infantum from seven European and two North African Mediterranean countries, four countries from the Middle East and Asia, as well as 20 L. donovani strains from East Africa and India were analysed in previous population genetic studies and have been incorporated here to elucidate the phylogenetic position of NW L. infantum in relation to OW L. donovani complex species. Table 1 summarises the number of strains per species according to geographical origin (continent and country), zymodeme and clinical picture. Most of the Brazilian strains were obtained from the Leishmania collection of the Oswaldo Cruz Institute (CLIOC, WDCM731, All strains from CLIOC were typed by MLEE as IOC/Z1 which corresponds to zymodeme MON-1 [44] (unpublished data) (Table S1). Strains from Paraguay were collected in 2000 (Programa Nacional de Leishmaniosis, SENEPA, Ministry of Public Health, Paraguay), and the strains from Venezuela were provided by the Universidad de Carabobo, Centro Nacional de Referencia de Flebotomos de Venezuela (CNRFV-BIOMED-UC). DNA of strains from Panama, Costa Rica and some from Brazil were obtained from the Royal Tropical Institute (KIT), Amsterdam, The Netherlands and from the WHO's Jerusalem Reference Centre for Leishmaniases, Hebrew University – Hadassah Medical School, Jerusalem. Strains from Honduras, which were previously typed by kDNA-RFLP [20] were given by the London School of Hygiene and Tropical Medicine, London, UK.


Figure 1. Distribution of the populations and subpopulations of NW L. infantum in the studied endemic regions.

The first number refers to the number of strains belonging to the indicated population (specified by the color), the second number gives the overall number of studied strains from the respective region. Additional endemic regions that were not studied are marked by grey color. (A): Colors of the respective population correlate with those in Fig. 2 (Pop1-INFNW - blue; Pop2-INFNW - red). In Honduras all but one strain belong to Population 1. In Colombia shared memberships in both populations could be recognized, with the predominant part of membership in Population 1. (B): Sub-populations found in Population 1. Colors correlate with those of the sub-populations in Fig. 2 (Sub-Pop1A-INFNW - dark blue, Sub-Pop1B-INFNW - light blue). In Pará one strain belongs to Sub-Pop1A-INFNW, and two strains have shared membership in both sub-populations 1A and 1B with predominating 1B traits, and two strains belong to sub-population 1B. Strains from Colombia belong to the 1B subpopulation (light blue), the Hondurian strains to 1A (dark blue) (not shown). (C): Distribution of clinical pictures among the 98 studied strains. VL – visceral leishmaniasis, CL – cutaneous leishmaniasis, CanL – canine leishmaniasis, nd – not determined.


Table 1. Numbers of strains per species, region, clinical picture and host of the studied sample set.


DNA was isolated using proteinase K- phenol/chloroform extraction [45] or the Wizard™ Genomic DNA Purification System (Promega, Madison, WI, USA) according the manufacturer's protocol, suspended in TE-buffer or distilled water and stored at 4°C until use.

PCR amplification assays and electrophoretic analysis of the microsatellite markers

The standard set of 14 primer pairs (Lm2TG, TubCA, Lm4TA, Li41-56, Li46-67, Li22-35, Li23-41, Li45-24, Li71-33, Li71-5/2, Li71-7, CS20, kLIST7031, LIST7039) that we have previously applied for the L. donovani complex was used for amplification of microsatellite containing fragments, as previously described [38], [43]. PCRs were performed with fluorescence-conjugated forward primers. Screening of length variations of the amplified markers was done by automated fragment analysis using capillary sequencers. PCR products from amplified microsatellites were analysed either with the fragment analysis tool of the CEQ 8000 automated genetic analysis system (Beckman Coulter, USA) or the ABI PRISM GeneMapper (Applied Biosystems, Foster City, CA).

Data analysis

Population structure was investigated by the STRUCTURE software [46], which applies a Bayesian model-based clustering approach. This algorithm identifies genetically distinct populations on the basis of allele frequencies. Genetic clusters are constructed from the genotypes identified, estimating for each strain the fraction of its genotype that belongs to each cluster. This clustering method proved superior to distance-based approaches for processing data sets of low variability like those presented by L. infantum. The following parameters were used: “burn-in” period of 20,000 iterations, probability estimates based on 200,000 Markov Chain Monte Carlo iterations. The most appropriate number of populations was determined by calculation of ΔK, which is based on the rate of change in the log probability of data between successive K values [47].

Phylogenetic analysis was based on microsatellite genetic distances, calculated with the program POPULATIONS 1.2.28 (​ations) for the numbers of repeats within each locus using the Chord-distance [48], which follows the infinite allele model (IAM). Neighbor-joining trees were constructed with the POPULATIONS software and visualized with MEGA [49]. Microsatellite markers as well as populations were analysed with respect to diversity of alleles (A), expected (gene diversity) and observed heterozygosity (He and Ho, respectively), and the inbreeding coefficient FIS applying GDA (​/plewis/software.php).

Genetic differentiation and gene flow was assessed by F-statistics [50] calculating the FST (theta) values (IAM) [51] with the corresponding p-values (confidence test) using the MSA software [52] (for details see Methods S1).

Ethics statement

Research in this study was subject to ethical review by the European Commission and approved as part of contract negotiation for Project LeishEpiNetSA (contract 01547): the work conformed to all relevant European regulations. The research was also reviewed and approved by the ethics committee of the London School of Hygiene and Tropical Medicine (approval 5092). The Leishmania strains analysed in this consolidated microsatellite analysis were principally reference strains derived from international cryobanks as CLIOC (registered at the World Data Centre for Microorganisms under the number WDCM731 and recognized as depository authority by the Brazilian Ministry of the Environment, MMA/CGEN Deliberação CGEN 97 de 22/03/2005, Processo 02000.003672/2004-34), the cryobank of the London School of Hygiene and Tropical Medicine (LSHTM), the Centro Nacional de Referencia de Flebotomos de Venezuela (CNRFV-BIOMED-UC), the cryobank of the Royal Tropical Institute (KIT) in Amsterdam, Netherlands and the WHO's Jerusalem Reference Centre for Leishmaniases, Hebrew University, Jerusalem, Israel. They have already been object of many publications. Several other strains were from small prior studies also using other methods, such as the strains from Honduras that were isolated 16–23 years ago and deposited at the LSHTM cryobank [4], [20], [22]. In all cases Leishmania were isolated from patients as part of normal diagnosis and treatment with no unnecessary invasive procedures and with written and/or verbal consent recorded at the time of clinical examination. Data on isolates were coded and anonymised. Isolation of Leishmania during the course of this study and not obtained from historical reference collections, whether from patients or animals, was subject to a local ethical review and approval in Paraguay (human and animal samples) by the Ethical-Scientific Committee at the IICS-UNA, under Code P42/07. All L. infantum and L. donovani strains origin from different central cryobanks (Table S1) and were already the object of many publications [4], [37], [39][41], [43].


Genetic diversity and population structure of NW L. infantum

Ninety-eight strains of L. infantum from seven South and Central American countries with emphasis on Brazil have been studied by microsatellite analysis (Figure 1 and Table 1). Most of these strains were isolated in the drier, poorly forested regions and represented human or canine isolates, but several were isolated from wild animal reservoirs, foxes (Cerdocyon thous) and opossums (Didelphis marsupialis), in the Amazonian forest region (Pará, Colombia). Isolates from different clinical forms (human VL and ACL), as well as three strains from VL/HIV co-infections were included. Table 2 shows the variability measures for the 14 microsatellite loci in NW L. infantum. The number of alleles varied between 2–8, with a mean value of 5.1. The most variable markers were, as in a previous study on OW L. infantum [4], Lm2TG and Li 22–35. The observed heterozygosity was very low (mean Ho = 0.04) and always much lower than the expected (mean He = 0.216). Inbreeding coefficients varied between 0.489 and 1 (mean FIS = 0.818). This disparity between expected and observed heterozygosity and the high FIS values points to a considerable amount of inbreeding and/or population substructuring, reflecting possible Wahlund effect.


Table 2. Characterization of the 14 microsatellite markers used for population analysis of NW L. infantum.


STRUCTURE analysis indicated that the sample set of NW L. infantum comprised two main populations as inferred by ΔK calculation (Figure 2). This population structure has been confirmed by distance analysis and the inferred neighbor-joining tree (Figure 3). Population 1 (Pop1-INFNW) which includes 89 of the 98 strains consists of all strains from Brazil, Paraguay and Colombia, and all but one strain from Honduras, regardless of whether they were isolated from cases of VL, VL/HIV+ or CL, or from different animal reservoirs, such as dogs and foxes. It also included the single opossum isolate. Population 2 (Pop2-INFNW) comprises only 9 strains, mostly from the Caribbean region (all strains from Costa Rica, Panama, Venezuela and one strain from Honduras) isolated from VL, CL and canine leishmaniasis (CanL) cases (Table S1). The distribution of the respective populations 1 and 2 among the Central and South American countries is shown in Figure 1A. F-statistics showed significant genetic differentiation between these two populations: FST = 0.761 and p = 0.0001.


Figure 2. Estimated population structure and substructure of NW L. infantum as inferred by the STRUCTURE program.

Results are based on MLMT of 14 microsatellite markers obtained for the 98 strains of NW L. infantum studied. In the barplots each strain is represented by a single vertical line divided into K colors, where K is the number of populations assumed. Each color represents one population, and the length of the colors segment shows the strain's estimated proportion of membership in that population. Isolates are organized by membership coefficients. According to ΔK the most probable number of populations in the data set is two, corresponding to MON-1 (blue) and non-MON-1 (red) isolates. In each of these main populations ΔK calculations suggest two sub-populations. VL – visceral leishmaniasis, CL – cutaneous leishmaniasis, CanL – canine leishmaniasis.


Figure 3. Neighbor-joining tree inferred from the Chord-distance calculated for the MLMT profiles of NW L. infantum.

This unrooted tree was derived based on the MLMT profiles of 14 microsatellite markers for the studied sample set of 98 strains of NW L. infantum as used for Bayesian model-based analysis with the STRUCTURE program. The two populations inferred by STRUCTURE (K2) are found also by this distance –based method and are indicated on the tree. Strain origins are explained in the window beside. Marsupial and fox isolates are marked by triangles. VL – visceral leishmaniasis, CL – cutaneous leishmaniasis, CanL – canine leishmaniasis.


A very important observation was that Pop1-INFNW is very homogeneous with only 35 genotypes identified for the 89 strains (proportion of polymorphic strains in pop1 = 39%), whereas in Pop2-INFNW all strains had unique genotypes. Table 3 gives a detailed overview of the number of genotypes found in each country studied and Figure S1 shows a neighbor-joining tree, which is based only on distinct genotypes. Interestingly, 13 out of the 15 Honduran strains in Pop1-INFNW including all CL cases, shared an identical MLMT profile. Another cluster of identical MLMT profiles was found for eight strains of human and canine origin from Mato Grosso do Sul. A third big cluster of identical genotypes comprised 23 strains from Espírito Santo, Rio de Janeiro, Pernambuco, Ceará, and three from Paraguay. Also here an identical MLMT profile was shared by human VL, VL/HIV+ and canine isolates (Figure S1, Figure S2). The difference in the degree of polymorphism between Pop1-INFNW and Pop2-INFNW is also reflected by the mean number of alleles (MNA) of 3.1 for population 1 (N = 89) and of 2.9 for population 2 (N = 9) (Table 4). In both populations the observed heterozygosity was much lower than the expected, leading to high FIS values (Tables 2 and 4).


Table 3. Number of MLMT genotypes found for each country and the studied endemic regions of Brazil.


Table 4. Characterization of the two main populations found for the analysed 98 NW L. infantum strains.


Both main populations have been tested by STRUCTURE for sub-structures. Two sub-populations were found for each of the main populations (Figure 2). Sub-Pop1B-INFNW (34 strains) comprised 22 of the 24 strains from Mato Grosso do Sul, all fox isolates from Pará, all Colombian strains including the D. marsupialis isolate, and three canine strains from Paraguay. The other 55 strains were members of Sub-Pop1A-INFNW consisting of all strains from Honduras, seven strains from Paraguay and the strains from all other Brazilian foci. Both 1A and 1B sub-populations included strains isolated from all clinical forms of human disease as well as from dogs. Population 2 was divided into Sub-Pop2B-INFNW comprising all Venezuelan strains isolated from human cases of VL and CL and from dogs, and Sub-Pop2A-INFNW consisting of the CL strains from Panama and Costa Rica, and a single VL strain from Honduras. Distance analysis confirmed the inferred subpopulations (Figures S1 and S2). FST analysis however showed that genetic differentiation of the sub-populations was statistically not significant. The assignment of the strains to the respective populations and sub-populations is given in Table S1.

Combined population analysis of NW and OW L. infantum

To address questions about the nomenclature and the origin of NW L.infantum we have included in the analysis previously identified MLMT profiles of 308 L. infantum strains from different countries of southern Europe, North Africa, the Middle East and Asia and, as an outgroup, 20 L. donovani strains from East Africa and India [4], [37], [39][41], [43] (Table S1, Table 1). Most of the L. infantum strains belong to the zymodeme MON-1, the most ubiquitous in the Old World, however several non-MON-1 strains have been also included. All these strains represented different clinical pictures in humans, namely VL, CL, VL/HIV+, PKDL, as well as canine, fox and sand fly isolates (Table 1).

STRUCTURE analysis of the combined NW and OW L. infantum strains revealed 3 main populations, as deduced from ΔK calculation (Figure 4), which showed significant genetic differentiation (Table 5). The largest population (Pop1-INFNW+OW) was formed by 224 strains from Spain, Portugal, France, Italy (all identified as MON-1) as well as from Brazil, Paraguay, Honduras (all but one strain) and Colombia. The second population (Pop2-INFOW) comprised 121 MON-1 strains from Algeria, Tunisia, Greece, Turkey, Israel, Palestine, Uzbekistan, China, and few from France and Italy. Strains from the New World were not found in this population. The third population (Pop3-INFNW+OW) consisted of 59 strains from southwestern Europe and North Africa (all identified as non-MON-1) as well as from Venezuela, Panama, Costa Rica and a single strain from Honduras. Consequently, population 1 of NW L. infantum (Pop1-INFNW) is part of the southwestern European L. infantum MON-1 population, and population 2 of NW L. infantum (Pop2-INFNW) of the Mediterranean non-MON-1 L. infantum population. The non-MON-1 population was the most variable one, as shown by the highest values for the MNA (9.6), Ho (0.27) and He (0.777), although the sample size was much smaller than that of the other two populations. This is in agreement with previous observations for Mediterranean L. infantum [4]. All three populations showed high FIS values, especially the two MON-1 populations (Table 6).


Figure 4. Estimated population structure and substructure of the combined New World and Old World sample set.

MLMT profiles based on 14 microsatellite markers for 308 OW strains and 98 NW strains of L. infantum were analysed by Bayesian statistics implemented in the STRUCTURE software. In the barplots each strain is represented by a single vertical line divided into K colors, where K is the number of populations assumed. Each color represents one population, and the length of the colors segment shows the strain's estimated proportion of membership in that population. Isolates are organized by membership coefficients. According to ΔK the most probable number of populations in the data set is three, corresponding to MON-1 isolates from Southwest Europe and the New World (blue), MON-1 isolates from North Africa, Southeast Europe and Asia (green), and non-MON-1 islates from the Old and New World (red). ΔK calculations suggest two sub-populations in the main populations Pop1 and Pop3.


Table 5. FST values and corresponding p-values for the main three populations.


Table 6. Characterization of the main populations found by STRUCTURE analysis for the 406 L. infantum strains.


The two main populations which included the NW L. infantum strains were tested for sub-structures. Population 1 (Pop1-INFNW+OW) was clearly divided into two sub-populations, as inferred by ΔK (Figure 4), with significant genetic differentiation between them (FST = 0.223, p = 0.0001). Sub-Pop1A-INFNW+OW (N = 149 strains) comprised the majority of strains and included strains from the Iberian mainland, Italy, and France as well as the NW strains. Sub-Pop1B-INFOW (N = 75 strains) contained all Balearic strains, strains from Sicily and Campania (Italy) and from the Provence region of France. The sub-structures of the non-MON-1 population 3 (Pop3-INFNW+OW) were not very clear, however a first split led to Sub-Pop3A-INFOW formed by 28 strains from North Africa and Malta. Sub-Pop3B-INFNW+OW comprised 31 strains from Europe and the NW (Figure 4). There is significant genetic differentiation between these sub-populations (FST = 0.25, p = 0.0001). Table 7 presents the variability measures for each of the detected sub-populations. The most homogeneous population was Sub-Pop1A-INFNW+OW, which comprised L. infantum MON-1 (MNA = 3.3), even though its sample size was the largest. High FIS values were detected for each of these sub-populations.


Table 7. Characterization of sub-populations of populations 1 and 3 of combined NW and OW L. infantum.


The same clustering and population structure was found by distance analysis of the MS data. Figure 5 shows the neighbor-joining tree inferred from the combined sample set of 426 strains from the Old and New World with L. donovani as outgroup. NW strains of L. infantum are intermingled among the European L. infantum MON-1 and non-MON-1 strains. Identical genotypes were found multiple times for strains of NW and OW L. infantum in population 1 (Pop1-INFNW+OW), e.g. between strains from Mato Grosso do Sul (Brazil) and a strain from Portugal, between strains from eastern Brazil, Paraguay, and from France and Spain. Furthermore, one of the Honduran VL strains was identical to strains from Portugal and France (data not shown). NW strains of L. infantum were concentrated in few major clusters that also contained strains from the Iberian peninsula and France, indicating an expansion of single clones (Figure S3, Figure 5).


Figure 5. Neighbor-joining tree derived for the combined New World and Old World data set.

This unrooted tree was inferred from the Chord-distance calculated for the MLMT profiles of 14 microsatellite markers for the studied sample set of 98 NW strains of L. infantum (marked by blue squares), 308 OW strains of L. infantum (marked by dots of different colors, depending on their origin) and 20 strains of L. donovani (marked by grey triangles). The three populations inferred by Bayesian model-based analysis with the STRUCTURE program (K3) and shown in Fig. 4 are indicated. MON-1 strains are marked by blue branches, non-MON-2 strains by red branches, and L. donovani by black branches. NW strains of L. infantum are present in population 1 and 3. Strains isolated from Didelphis marsupialis and Cerdocyon thous are interspersed among population1 that included the majority of NW strains (human and canine) together with strains of L. infantum from the Iberian mainland (Spain, Portugal), France and Italy. Strain origins are listed in the legend beside.



Population structure of NW L. infantum and comparison with OW L. infantum population structure

Knowledge of the population structure of NW L. infantum was so far very restricted and essentially based on clinical observations and the population structure of the vector. With the development of MLMT an adequate and powerful tool based on highly polymorphic genetic markers that differentiate at intra-species level became available for analysing population structure of the parasite. The present paper shows that there are two main populations of NW L. infantum, that correlate with the separation of L. infantum into MON-1 and non-MON-1 strains [4], [43]. Ninety-one per cent of the 98 NW strains analysed fell into the MON-1 population (Pop1-INFNW), which extends over a huge geographical and ecological range, including strains from all Brazilian, Paraguayan and some Colombian foci, and from Honduras. This situation is very similar to that in the OW, where ~70% of L. infantum strains isolated in foci in southern Europe, Middle East, Central Asia and North Africa belong to zymodeme MON-1 [53]. The remaining 9% of the NW L. infantum strains belong to the non-MON-1 population 2 (Pop2-INFNW) and, interestingly, all these strains come from the Caribbean region, from Panama, Costa Rica and Venezuela, and a single strain from Honduras. Whether the non-MON-1 strains are generally present exclusively in the Caribbean region needs to be further elucidated.

The focal point of our sampling was Brazil, including most of the known foci. Although Brazil is an ecologically diverse country and different reservoirs and vector populations have been reported, all the 64 Brazilian strains from different VL foci belonged to the MON-1 population 1. The same was true for the neighboring country Paraguay.

The degree of polymorphism in NW L. infantum is much lower than among OW L. infantum. Only 39% of the NW MON-1 strains had individual MLMT profiles compared to about 75% of the OW MON-1 strains analysed in this and in a previous study [4]. The lower variability of NW L.infantum is also reflected by lower MNA and He values for both the MON-1 and non-MON-1 populations (Table 4 and Table S2). Moreover, in contrast to the NW genetically clearly separated geographically determined sub-populations were observed in the OW MON-1 cluster. The lower diversity of NW L. infantum supports the hypothesis of a recent import of selected strains of L. infantum from the Old to the New World [54]. In the case of indigenous parasites we would expect a much higher diversity and more complex population structures.

Despite the low diversity of NW L.infantum we found indications for population sub-structures. The MON-1 sub-populations are mostly geographically determined. Two sub-populations were recognized in Brazil and Paraguay, Sub-Pop1B-INFNW comprised three strains from central Paraguay, all but two strains from the Mato Grosso do Sul focus and those from rural foci in Pará. All other strains were members of the Sub-Pop1A-INFNW. Strains from Colombia and Honduras belonged to the sub-populations 1B and 1A, respectively. There is some hint that the Colombian strains may form a separate population, but this has to be proven with more strains from that country.

Three big clusters were detected that contain genetically identical strains. The first two included strains from the same focus, eight strains from Mato Grosso do Sul and 13 from Honduras, respectively. The third comprised 26 strains from seven states of Brazil, mostly from the eastern part of the country and some from Paraguay. This is evidence for the spread of several single clones in the New World. The homogeneity of strains in Honduras where only three genotypes were identified for 15 strains collected between 1987 and 1994 was surprising and needs further investigation.

The strong heterozygote deficiency and high inbreeding coefficients found for NW and OW L. infantum could result from population subdivision (Wahlund effect), presence of null alleles, natural selection, gene conversion, and inbreeding. Since similar FIS patterns were obtained across all 14 microsatellite loci in this study, null alleles, selection and gene conversion are unlikely to be responsible for the heterozygote deficiency found. Recent studies [55], [56] have demonstrated the existence of Wahlund effect in Leishmania populations which did however account only partially for the high inbreeding and suggested the “existence of population foci at a microgeographic scale, where clonality alternates with sexuality of an endogamic nature”. The strains of NW L. infantum analysed herein were sampled over large areas and further geographic subdivision of the subpopulations identified seems to be quite likely. For clarifying whether the high inbreeding is exclusively due to population subdivision or also to the presence of sexual recombination, mainly among identical or similar organisms, sampling at finer geographical scale would be essential.

Clinical picture, reservoirs and vectors versus NW L. infantum populations and sub-populations

There was no strict correlation between clinical pictures and population assignment. Strains isolated from human VL and CL cases, including the atypical CL cases collected exclusively in the Caribbean, were assigned to both the MON-1 and non-MON-1 populations. VL/HIV+ coinfections were found only in the MON-1 population, but due to the small number of these samples so far analysed we cannot draw conclusions. In Pop1-INFNW strains from CL cases from Honduras formed a single cluster of identical genotypes and one of the two VL strains from Honduras was similar to this CL cluster. This confirms previous reports showing by kDNA RFLP and RAPD that the two clinical forms in Honduras and Nicaragua were caused by genetically similar parasites [20], [21]. In addition, we found that at least two different parasite populations circulate in Honduras. Disease susceptibility and clinical manifestation is, however not only affected by parasite factors but also by host conditions, such as malnutrition and the age of the patient (status of the host immune system). In Honduras VL patients were much younger than CL patients. The vector may also play a role, as two species, Lu. longipalpis and Lu. evansi, are present in the Honduran endemic foci.

Obviously, we cannot link the restricted occurrence of CL cases in the Caribbean region with the general population assignment to MON-1 and non-MON-1 strains. From the Old World it is known, that only 20% of the CL cases are due to MON-1 strains and that the majority of CL cases is caused by strains of zymodeme MON-24, besides other dermotropic zymodemes, some of which were represented by several strains in this study. Ninety percent of all VL cases of immunocompetent individuals are caused by MON-1 strains, but there are also several other viscerotropic zymodemes [57], [58]. The tropism of many zymodemes is not clear cut, they are known to cause both VL and CL and the reasons leading to the respective clinical picture seem to be very complex.

The dog is the main reservoir host for NW L. infantum [59] and this was confirmed by the detection of identical MLMT profiles for human and canine strains from different VL foci, such as Mato Grosso do Sul, Ceará, Espírito Santo, Rio de Janeiro (Brazil) and Paraguay. All canine strains were found in the MON-1 population except one from Venezuela which was linked to the non-MON-1 population. This is in agreement with the situation in the OW where the majority of canine leishmaniasis is due to strains of zymodeme MON-1 [58], [60], [61]. Only very few other zymodemes, MON-98, 77, and 108, which are closely related to MON-1, and MON-253 and MON-24 have occasionally been found in dogs.

It has been suggested that natural foci of sylvatic zoonotic transmission may exist beside the main transmission cycle via the domestic dog [62][64]. Foxes are considered to be a natural reservoir of VL in different states of Brazil, such as Pará [65], Mato Grosso do Sul [66], Ceará and Piauí [63], Minas Gerais [67], [68], and Amazonas [69]. Didelphis marsupialis has been incriminated as an important reservoir host of NW L. infantum only in Colombia [70][72]. Opossums infected by NW L. infantum have, however also been reported from Bahia and Minas Gerais [73], [74]. The role of these animals in natural infection cycles remains however, questionable [73], [75]. MLMT analysis did not reveal separate genotypes for strains from wild animals. The four isolates from foxes and the one from a marsupial were all assigned to the MON-1 Sub-Pop1B-INFNW and interspersed with the human and canine strains (Figure 2, Figure 3 and Figures S1, S2, S33).

The transmission of NW L. infantum, its virulence and clinical picture are likely influenced by coevolutionary interactions between specific parasite and sand fly genotypes, as suggested recently [26], and different sand fly species or subspecies might be involved in the transmission of different L. infantum genotypes in the NW. Lu. longipalpis, the major vector of NW L. infantum, is distributed from Southern Mexico to Northern Argentina and it is considered to be a complex of sibling species [15], [24][26], [28]. Arrivillaga et al. (2002) have concluded from mitochondrial sequence (COI) data that Lu. longipalpis in Central and South America consists of at least four clades, which constitute species [27]. These clades may correlate in part with some of the populations or subpopulations of NW L. infantum identified in this study.

The Caribbean non-MON-1 population might possibly be linked to Lu. evansi which was reported as an alternative vector for NW L. infantum in Latin America [15], but was not found in Brazil. Interestingly, most strains from Mato Grosso do Sul and three from Paraguay were found in Sub-Pop1B-INFNW whereas the strains from all other Brazilian and Paraguyan foci were assigned to Sub-Pop1A-INFNW. This could be attributed to the fact that in some foci of Mato Grosso do Sul Lu. cruzi (a species within the Lu. longipalpis complex) has been established as the vector for NW L. infantum and it has been found to be sympatric with Lu. longipalpis in many areas [76][82]. It is perhaps also present in bordering areas of Paraguay and Bolivia [77], [79], [80], [83]. Whether different geographically determined L. infantum genotypes correlate with the occurrence of specific sand fly species in those areas should be further investigated.

Origin of NW L. infantum

Our results indicate that L. infantum was introduced from Southwest Europe to the New World several times and at several points along this continent (Figure 6). The genotypes found in specific regions in South and Central America were also found in Europe, especially among the Spanish, Portuguese, French and Italian strains of L. infantum. When analysed together the MON-1 population of NW L. infantum was intermingled with MON-1 strains from the Western European Mediterranean countries and the non-MON-1 population comprised strains from both New and Old Worlds.


Figure 6. Map showing the presumable origin of NW L. infantum.

The respective populations of L. infantum in the Old and New Worlds are indicated by the respective colors used in Fig. 2 and 5. NW L. infantum has been introduced from Southwest Europe to the New World multiple times.


There were several waves of immigration of Europeans into the New World especially from Leishmania endemic countries such as Portugal and Spain starting with the arrival of the Conquistadores up to the immigration of settlers during last century. Brought to South America with European immigrants, perhaps many times, the parasites spread rapidly due to migration, urbanization and trade. There is e.g. some indication of expansion of single genotypes (clones) among the Northeast of Brazil and Mato Grosso do Sul, respectively. This introduction of L. infantum is still ongoing as recently shown for an infected dog which was brought from France to French Guiana [17].

This study further confirmed that the agent of VL in the New World is L. infantum and not a separate indigenous species, L. chagasi. This is also supported by i) the identity of the isoenzyme profiles [44], [54], [84][88], ii) the identical genotypes obtained by analysing different genomic targets with different molecular techniques [2][4], [38], [43], [89][92], iii) the fact that L. infantum can be transmitted by several OW sand fly species and infect, develop in and adapt to Lu. longipalpis [32], and (iv) by the fact that New World foxes are phylogenetically closer to Old World wolf-like canids than to Old World foxes and therefore have a high potential to be a reservoir [93]. It still remains unclear, whether neotropical wild animals found to be infected with L. infantum are accidental hosts or real reservoirs. We could show, that parasites isolated from four foxes and one marsupial did not constitute a separate population in the NW and are, thus, not part of separate transmission cycles.

Multiple introductions of the parasite help to explain the immense spread of L. infantum in the NW Furthermore, Lu. longipalpis has been proven to be a permissive vector and fast adaptation is facilitated by modification of the parasite's surface molecules [94], [95]. Thus L. infantum brought to the NW could have easily adapted to the respective local sand fly populations.

Recent, and likely continious migrations to and possibly even from, the NW are further supported by FST values calculated between NW and OW L. infantum, which indicate only little genetic differentiation (data not shown). In contrast, we observed that the populations of L. infantum from southern Europe are more closely related to NW L. infantum than to other populations of OW L. infantum, e.g. from North Africa, Central Asia, the Middle East and even South Eastern Europe. Moreover, parasites indigenous in the NW should be more diverse, but we observed them to be much less diverse than L. infantum or L. donovani from the Old World. This is consistent with a founder effect, i.e. recent introduction of a restricted part of the original L. infantum population, with possible genetic drift or clonal expansion of only some genotypes. As a consequence there is no justification for a taxonomic separation of L. chagasi and L. infantum at species or subspecies level .

The present paper represents to our knowledge the first comprehensive population study of NW L .infantum, in which we have applied a high resolution typing method sensitive enough to detect population structures at intra-species level. We found a very homogenous population structure in Brazil and Paraguay consisting exclusively of MON-1 strains and a mixed population structure including MON-1 and non-MON-1 strains in the Caribbean region. Further studies with refined sampling strategies based on the populations and sub-populations detected in this study will enable more intensive microepidemiological analyses of NW L. infantum genotypes, and their association with reservoirs, vectors, clinical presentation, host immunological status, ecology, geography, and socioeconomic or demographic factors. We have provided conclusive evidence of recent multiple introductions of L. infantum from the Old into the New World including both MON-1 and non-MON-1 genotypes and for the synonymy of L. infantum and L. chagasi.

Supporting Information

Figure S1.

Neighbor-joining tree of NW L. infantum genotypes. This midpoint-rooted tree was derived from the Chord-distance calculated for the MLMT profiles of 14 microsatellite markers. Only different genotypes are scored. Clinical pictures, reservoir, origin and number of strains sharing the same genotype are indicated, as well as population and sub-population assignements according to Bayesian model-based analysis with the STRUCTURE program (see Fig. 2). MS - Mato Grosso do Sul, PA - Pará, RJ - Rio de Janeiro, ES - Espírito Santo, BA - Bahia, RN - Rio Grande do Norte, PI - Piauí, PE - Pernambuco, nd - not defined. VL - visceral leishmaniasis, CL - cutaneous leishmaniasis, CanL - canine leishmaniasis.



Figure S2.

Midpoint-rooted neighbor-joining tree showing all individual NW L. infantum strains. Phylogenetic tree derived from the Chord-distance calculated for the MLMT profiles of 14 microsatellite markers for the 98 NW strains of L.infantum studied. Clinical pictures and reservoir for each strain are indicated. The origin of the Brazilian strains (state) is given as abbreviation: MS - Mato Grosso do Sul, PA - Pará, RJ - Rio de Janeiro, ES - Espírito Santo, BA - Bahia, RN - Rio Grande do Norte, PI - Piauí, PE - Pernambuco. Populations and sub-populations according to STRUCTURE analysis (see Fig. 2) are shown. T -WHO reference strain of NW L. infantum (PP75). VL – visceral leishmaniasis, CL – cutaneous leishmaniasis, CanL – canine leishmaniasis, nd – not determined.



Figure S3.

Neighbor-joining tree showing only population 1 of the combined NW and OW strains of L. infantum. This unrooted tree is based on the Chord-distance of the MLMT profiles of 14 microsatellite markers and it includes only strains belonging to population1 (MON-1) of the combined OW (dots) and NW (squares) L. infantum data set (see Fig. 5 and 6). Isolates of wild animal reservoirs are indicated by arrows. NW L. infantum strains (all marked by blue squares) are concentrated in few clusters marked in grey, that also contain L. infantum from Portugal (pink dots), Spain (red dots) and France (green dots). Origins of the strains are indicated in the legend beside.



Table S1.

bT – Reference strain of the species; 1 – zymdemes according to the Montpellier system – MON [86] or the CLIOC system – IOC/Z [44], MON-1 and Z1 are corresponding zymodemes; 2 – Population assignment according to STRUCTURE analysis of the combined dataset of 409 strains of NW and OW L. infantum; 3 – Population assignment according to STRUCTURE analysis of the dataset of 98 NW L. infantum strains; - VL – visceral leishmaniasis; CL – cutaneous leishmaniasis; PKDL – post Kala-Azar dermal leishmaniasis; CanL – canine leishmaniasis; cIL – central Israel, nIL – north Israel; nd – not defined; na – not applicable; CNRFV - BIOMED-Centro Nacional de Referencia de Flebotomos de Venezuela; SENEPA - Programa Nacional de Leishmaniosis, SENEPA, Ministry of Public Health, Paraguay; CLIOC - Coleção de Leishmania do Instituto Oswaldo Cruz, Brazil; LSHTM - London School of Hygiene and Tropical Medicine, UK; KIT - Royal Tropical Institute, Amsterdam, Netherlands; CNRLM - Centre National de Référence des Leishmania, Université Montpellier, France; ISCM - WHO Collaborating Centre for Leishmaniasis, Servicio de Parasitología, Instituto de Salud Carlos III, Mahadahonda (Madrid), Spain; ISS - Instituto Superiore di Sanità, Italy;.HPI - Hellenic Pasteur Institute, Athens, Greece; IHMT - Instituto de Higiene e Medicina Tropical, Universidade Nova de Lisboa, Portugal; JRCL - WHO's Jerusalem Reference Centre for Leishmaniases, Hebrew University, Hadassah Medical School, Jerusalem, Israel; AQNHI - Al-Quds Nutrition and Health Research Institute, Faculty of Medicine, Al-Quds University, Abu-Deis, Palestine; IPA - Institut Pasteur d'Algérie, Algiers, Algeria; LPMM - Laboratoire de Parasitologie_Mycologie à la Faculté de Pharmacie, Monastir, Tunisia; BHU - Kala-azar Medical Research Centre, Banaras Hindu University, Varanasi, India.



Table S2.

N, number of strains; P, proportion of polymorphic loci; MNA, mean number of alleles; Ho, observed heterozygosity; He, expected heterozygosity; FIS, inbreeding coefficient; FR – France; IT – Italy.



Methods S1.

Additional information about the methods of MLMT data analyses.




We thank Andrés Canese and Cynthia Céspedes (Programa Nacional de Leishmaniosis, SENEPA, Ministry of Public Health, Paraguay), Christophe Ravel (Centre National de Référence des Leishmania, Montpellier, France), Marina Gramiccia (Instituto Superiore di Sanità, Rome, Italy), Wendy van der Meide and Henk Schallig (Royal Tropical Institute, Amsterdam, The Netherlands), Lee Schnur (Kuvin Centre for the Study of Tropical and Infectious Diseases, Hadassah Medical School, Jerusalem, Israel), Harry Noyes (Liverpool School of Tropical Medicine, Liverpool, UK), Lenea Campino and Sofia Cortes (Instituto de Higiene e Medicina Tropical, Universidade Nova de Lisboa, Portugal), Carmen Cañavate (WHO Collaborating Centre for Leishmaniasis, Instituto de Salud Carlos III, Mahadahonda (Madrid), Spain), Ketty Soteriadou and Christos Haralambous (Helenic Pasteur Insitute, Athens, Greece), Nabila Seridi (Laboratoire de Génétique, Faculté des Sciences Biologiques USTHB, Algiers, Algeria), Najla Chargui (Laboratoire de Parasitologie, Mycologie, Faculté de Pharmacie, Monastir, Tunisia) and Ahmad Amro (Palestine) for supplying DNA of OW and NW L. infantum strains. We are grateful to Carola Schweynoch for technical assistance.

Author Contributions

Conceived and designed the experiments: KK GS EC MAM. Performed the experiments: KK MZA RO GEMF. Analyzed the data: KK TW MZA. Contributed reagents/materials/analysis tools: GS EC ILM RO MDF GEMF. Wrote the paper: KK GS EC ILM GEMF MAM.


  1. 1. Cunha AM, Chagas E (1937) Nova espécie de protozoário do genero Leishmania pathogenico para o homem. Leishmania chagasi, n. sp. . Nota Prévia Hospital (Rio de Janeiro) 11: 3–9.
  2. 2. Mauricio IL, Stothard JR, Miles MA (2000) The strange case of Leishmania chagasi. Parasitol Today 16: 188–189.
  3. 3. Mauricio IL, Howard MK, Stothard JR, Miles MA (1999) Genomic diversity in the Leishmania donovani complex. Parasitology 119(Pt 3): 237–246.
  4. 4. Kuhls K, Chicharro C, Cañavate C, Cortes S, Campino L, et al. (2008) Differentiation and Gene Flow among European Populations of Leishmania infantum MON-1. PLoS Negl Trop Dis 2: e261.
  5. 5. Rosypal AC, Troy GC, Zajac AM, Duncan RB Jr, Waki K, et al. (2003) Emergence of zoonotic canine leishmaniasis in the United States: isolation and immunohistochemical detection of Leishmania infantum from foxhounds from Virginia. J Eukaryot Microbiol 50: Suppl691–693.
  6. 6. Rosypal AC, Zajac AM, Lindsay DS (2003) Canine visceral leishmaniasis and its emergence in the United States. Vet Clin North Am Small Anim Pract 33: 921–937, viii.
  7. 7. Lainson R, Shaw JJ (1987) Evolution, classification and geographical distribution. In: Peters W, Killick-Kendrick R, editors. The leishmaniases in biology and medicine. London: Academic Press. pp. 1–120.
  8. 8. Momen H, Grimaldi G Jr, Deane LM (1987) Leishmania infantum, the aetiological agent of American visceral leishmaniasis (AVL)? Mem Inst Oswaldo Cruz 82: 447–448.
  9. 9. Shaw JJ, Lainson R (1987) Ecology and epidemiology, New World. In: Peters W, Killick-Kendrick R, editors. The leishmaniases in biology and medicine. London: Academic Press. pp. 291–363.
  10. 10. Grimaldi G Jr, Tesh RB, McMahon-Pratt D (1989) A review of the geographic distribution and epidemiology of leishmaniasis in the New World. Am J Trop Med Hyg 41: 687–725.
  11. 11. Lainson R, Shaw JJ (2005) New World Leishmaniasis. In: Cox FEG, Wakelin D, Gillespie SH, Despommier DD, editors. Topley & Wilson's Microbiology and Microbial Infections, 10th ed. London: Wiley & Blackwell. pp. 313–349.
  12. 12. Deane LM, Grimaldi G (1985) Leishmaniasis in Brazil. In: Chang KP, editor. Leishmaniasis. Amsterdam: Elsevier. pp. 247–281.
  13. 13. Romero GA, Boelaert M (2010) Control of visceral leishmaniasis in Latin America-a systematic review. PLoS Negl Trop Dis 4: e584.
  14. 14. Rotureau B (2006) Ecology of the Leishmania species in the Guianan ecoregion complex. Am J Trop Med Hyg 74: 81–96.
  15. 15. Lainson R, Rangel EF (2005) Lutzomyia longipalpis and the eco-epidemiology of American visceral leishmaniasis, with particular reference to Brazil: a review. Mem Inst Oswaldo Cruz 100: 811–827.
  16. 16. Desjeux P (1991) Information sur l'Épidémiologie des Leishmanioses et la Lutte Contre ces Maladies par Pays ou Territoire. Geneva: World Health Organization.
  17. 17. Rotureau B, Ravel C, Aznar C, Carme B, Dedet JP (2006) First report of Leishmania infantum in French Guiana: canine visceral leishmaniasis imported from the Old World. J Clin Microbiol 44: 1120–1122.
  18. 18. Oliveira Neto MP, Grimaldi G Jr, Momen H, Pacheco RS, Marzochi MC, et al. (1986) Active cutaneous leishmaniasis in Brazil, induced by Leishmania donovani chagasi. Mem Inst Oswaldo Cruz 81: 303–309.
  19. 19. Ponce C, Ponce E, Morrison A, Cruz A, Kreutzer R, et al. (1991) Leishmania donovani chagasi: new clinical variant of cutaneous leishmaniasis in Honduras. Lancet 337: 67–70.
  20. 20. Noyes H, Chance M, Ponce C, Ponce E, Maingon R (1997) Leishmania chagasi: genotypically similar parasites from Honduras cause both visceral and cutaneous leishmaniasis in humans. Exp Parasitol 85: 264–273.
  21. 21. Belli A, Garcia D, Palacios X, Rodriguez B, Valle S, et al. (1999) Widespread atypical cutaneous Leishmaniasis caused by Leishmania (L.) chagasi in Nicaragua. Am J Trop Med Hyg 61: 380–385.
  22. 22. De Lima H, Rodriguez N, Feliciangeli MD, Barrios MA, Sosa A, et al. (2009) Cutaneous leishmaniasis due to Leishmania chagasi/Le. infantum in an endemic area of Guarico State, Venezuela. Trans R Soc Trop Med Hyg 103: 721–726.
  23. 23. Zeledon R, Hidalgo H, Viquez A, Urbina A (1989) Atypical cutaneous leishmaniasis in a semiarid region of north-west Costa Rica. Trans R Soc Trop Med Hyg 83: 786.
  24. 24. Lanzaro GC, Ostrovska K, Herrero MV, Lawyer PG, Warburg A (1993) Lutzomyia longipalpis is a species complex: genetic divergence and interspecific hybrid sterility among three populations. Am J Trop Med Hyg 48: 839–847.
  25. 25. Bauzer LG, Souza NA, Maingon RD, Peixoto AA (2007) Lutzomyia longipalpis in Brazil: a complex or a single species? A mini-review. Mem Inst Oswaldo Cruz 102: 1–12.
  26. 26. Maingon RD, Ward RD, Hamilton JG, Bauzer LG, Peixoto AA (2008) The Lutzomyia longipalpis species complex: does population sub-structure matter to Leishmania transmission? Trends Parasitol 24: 12–17.
  27. 27. Arrivillaga JC, Norris DE, Feliciangeli MD, Lanzaro GC (2002) Phylogeography of the neotropical sand fly Lutzomyia longipalpis inferred from mitochondrial DNA sequences. Infect Genet Evol 2: 83–95.
  28. 28. Araki AS, Vigoder FM, Bauzer LG, Ferreira GE, Souza NA, et al. (2009) Molecular and behavioral differentiation among Brazilian populations of Lutzomyia longipalpis (Diptera: Psychodidae: Phlebotominae). PLoS Negl Trop Dis 3: e365.
  29. 29. Travi BL, Velez ID, Brutus L, Segura I, Jaramillo C, et al. (1990) Lutzomyia evansi, an alternate vector of Leishmania chagasi in a Colombian focus of visceral leishmaniasis. Trans R Soc Trop Med Hyg 84: 676–677.
  30. 30. Feliciangeli MD, Rodriguez N, De Guglielmo Z, Rodriguez A (1999) The re-emergence of American visceral leishmaniasis in an old focus in Venezuela. II. Vectors and parasites. Parasite 6: 113–120.
  31. 31. Shaw JJ (1994) Taxonomy of the genus Leishmania: present and future trends and their implications. Mem Inst Oswaldo Cruz 89: 471–478.
  32. 32. Killick-Kendrick R, Molyneux DH, Rioux JA, Lanotte G, Leaney AJ (1980) Possible origins of Leishmania chagasi. Ann Trop Med Parasitol 74: 563–565.
  33. 33. Shaw JJ (2006) Further thoughts on the use of the name Leishmania (Leishmania) infantum chagasi for the aetiological agent of American visceral leishmaniasis. Mem Inst Oswaldo Cruz 101: 577–579.
  34. 34. Dantas-Torres F (2006a) Leishmania infantum versus Leishmania chagasi: do not forget the law of priority. Mem Inst Oswaldo Cruz 101: 117–118; discussion 118.
  35. 35. Dantas-Torres F (2006b) Final comments on an interesting taxonomic dilemma: Leishmania infantum versus Leishmania infantum chagasi. Mem Inst Oswaldo Cruz 101: 929–930.
  36. 36. Shaw JJ (2002) New World leishmaniasis: the ecology of leishmaniasis and the diversity of leishmanial species in Central and South America. In: Farrell J, editor. World Class Parasites: Leishmania. Boston, Dordrecht, London: Kluwer Academic Publishers. pp. 11–31.
  37. 37. Chargui N, Amro A, Haouas N, Schonian G, Babba H, et al. (2009) Population structure of Tunisian Leishmania infantum and evidence for the existence of hybrids and gene flow between genetically different populations. Int J Parasitol 39: 801–811.
  38. 38. Ochsenreither S, Kuhls K, Schaar M, Presber W, Schonian G (2006) Multilocus microsatellite typing as a new tool for discrimination of Leishmania infantum MON-1 strains. J Clin Microbiol 44: 495–503.
  39. 39. Seridi N, Amro A, Kuhls K, Belkaid M, Zidane C, et al. (2008) Genetic polymorphism of Algerian Leishmania infantum strains revealed by multilocus microsatellite analysis. Microbes Infect 10: 1309–1315.
  40. 40. Alam MZ, Kovalenko DA, Kuhls K, Nasyrova RM, Ponomareva VI, et al. (2009) Identification of the agent causing visceral leishmaniasis in Uzbeki and Tajiki foci by analysing parasite DNA extracted from patients' Giemsa-stained tissue preparations. Parasitology 136: 981–986.
  41. 41. Amro A, Schonian G, Al-Sharabati MB, Azmi K, Nasereddin A, et al. (2009) Population genetics of Leishmania infantum in Israel and the Palestinian Authority through microsatellite analysis. Microbes Infect 11: 484–492.
  42. 42. Alam MZ, Kuhls K, Schweynoch C, Sundar S, Rijal S, et al. (2009) Multilocus microsatellite typing (MLMT) reveals genetic homogeneity of Leishmania donovani strains in the Indian subcontinent. Infect Genet Evol 9: 24–31.
  43. 43. Kuhls K, Keilonat L, Ochsenreither S, Schaar M, Schweynoch C, et al. (2007) Multilocus microsatellite typing (MLMT) reveals genetically isolated populations between and within the main endemic regions of visceral leishmaniasis. Microbes Infect 9: 334–343.
  44. 44. Cupolillo E, Grimaldi G Jr, Momen H (1994) A general classification of New World Leishmania using numerical zymotaxonomy. Am J Trop Med Hyg 50: 296–311.
  45. 45. Schonian G, Schweynoch C, Zlateva K, Oskam L, Kroon N, et al. (1996) Identification and determination of the relationships of species and strains within the genus Leishmania using single primers in the polymerase chain reaction. Mol Biochem Parasitol 77: 19–29.
  46. 46. Pritchard JK, Stephens M, Donnelly P (2000) Inference of population structure using multilocus genotype data. Genetics 155: 945–959.
  47. 47. Evanno G, Regnaut S, Goudet J (2005) Detecting the number of clusters of individuals using the software STRUCTURE: a simulation study. Mol Ecol 14: 2611–2620.
  48. 48. Cavalli-Sforza LL, Edwards AW (1967) Phylogenetic analysis. Models and estimation procedures. Am J Hum Genet 19: 233–257.
  49. 49. Tamura K, Dudley J, Nei M, Kumar S (2007) MEGA4: Molecular Evolutionary Genetics Analysis (MEGA) software version 4.0. Mol Biol Evol 24: 1596–1599.
  50. 50. Wright S (1951) The genetical structure of populations. Ann Eugenics 15: 323–354.
  51. 51. Weir BS, Cockerham CC (1984) Estimating F statistics for the analysis of population structure. Evolution 38: 1358–1370.
  52. 52. Dieringer D, Schlotterer C (2002) Microsatellite analizer (MSA): a platform independent analysis tool for large microsatellite sets. Molec Ecol Notes 3: 167–169.
  53. 53. Gallego M, Pratlong F, Fisa R, Riera C, Rioux JA, et al. (2001) The life-cycle of Leishmania infantum MON-77 in the Priorat (Catalonia, Spain) involves humans, dogs and sandflies; also literature review of distribution and hosts of L. infantum zymodemes in the Old World. Trans R Soc Trop Med Hyg 95: 269–271.
  54. 54. Momen H, Pacheco RS, Cupolillo E, Grimaldi Junior G (1993) Molecular evidence for the importation of Old World Leishmania into the Americas. Biol Res 26: 249–255.
  55. 55. Gelanew T, Kuhls K, Hurissa Z, Weldegebreal T, Hailu W, et al. (2010) Inference of population structure of Leishmania donovani strains isolated from different Ethiopian visceral leishmaniasis endemic areas. PLoS Negl Trop Dis 4: e889.
  56. 56. Rougeron V, De Meeus T, Hide M, Waleckx E, Bermudez H, et al. (2009) Extreme inbreeding in Leishmania braziliensis. Proc Natl Acad Sci U S A 106: 10224–10229.
  57. 57. Pratlong F, Dereure J, Deniau M, Marty P, Faraut-Gambarelli F, et al. (2003) Enzymatic polymorphism during Leishmania/HIV co-infection: a study of 381 Leishmania strains received between 1986 and 2000 at the international cryobank in Montpellier, France. Ann Trop Med Parasitol 97: Suppl 147–56.
  58. 58. Pratlong F, Rioux JA, Marty P, Faraut-Gambarelli F, Dereure J, et al. (2004) Isoenzymatic analysis of 712 strains of Leishmania infantum in the south of France and relationship of enzymatic polymorphism to clinical and epidemiological features. J Clin Microbiol 42: 4077–4082.
  59. 59. Dantas-Torres F (2007) The role of dogs as reservoirs of Leishmania parasites, with emphasis on Leishmania (Leishmania) infantum and Leishmania (Viannia) braziliensis. Vet Parasitol 149: 139–146.
  60. 60. Alvar J, Cañavate C, Molina R, Moreno J, Nieto J (2004) Canine leishmaniasis. Adv Parasitol 57: 1–88.
  61. 61. Martin-Sanchez J, Gramiccia M, Di Muccio T, Ludovisi A, Morillas-Marquez F (2004) Isoenzymatic polymorphism of Leishmania infantum in southern Spain. Trans R Soc Trop Med Hyg 98: 228–232.
  62. 62. Travi BL, Osorio Y, Guarin N, Cadena H (1998) Leishmania (Leishmania) chagasi: clinical and parasitological observations in experimentally infected Didelphis marsupialis, reservoir of New World visceral leishmaniasis. Exp Parasitol 88: 73–75.
  63. 63. Gomes RB, Mendonca IL, Silva VC, Ruas J, Silva MB, et al. (2007) Antibodies against Lutzomyia longipalpis saliva in the fox Cerdocyon thous and the sylvatic cycle of Leishmania chagasi. Trans R Soc Trop Med Hyg 101: 127–133.
  64. 64. Lainson R, Dye C, Shaw JJ, Macdonald DW, Courtenay O, et al. (1990) Amazonian visceral leishmaniasis–distribution of the vector Lutzomyia longipalpis (Lutz & Neiva) in relation to the fox Cerdocyon thous (linn.) and the efficiency of this reservoir host as a source of infection. Mem Inst Oswaldo Cruz 85: 135–137.
  65. 65. Lainson R, Shaw JJ, Silveira FT, Braga RR (1987) American visceral leishmaniasis: on the origin of Leishmania (Leishmania) chagasi. Trans R Soc Trop Med Hyg 81: 517.
  66. 66. Mello DA, Rego Junior Fde A, Oshozo E, Nunes VL (1988) Cerdocyon thous (L.) (Carnivora, Canidae) naturally infected with Leishmania donovani chagasi (Cunha & Chagas, 1973) in Corumba (Mato Grosso do Sul State, Brazil). Mem Inst Oswaldo Cruz 83: 259.
  67. 67. Curi NH, Miranda I, Talamoni SA (2006) Serologic evidence of Leishmania infection in free-ranging wild and domestic canids around a Brazilian National Park. Mem Inst Oswaldo Cruz 101: 99–101.
  68. 68. Luppi MM, Malta MC, Silva TM, Silva FL, Motta RO, et al. (2008) Visceral leishmaniasis in captive wild canids in Brazil. Vet Parasitol 155: 146–151.
  69. 69. Courtenay O, Macdonald DW, Lainson R, Shaw JJ, Dye C (1994) Epidemiology of canine leishmaniasis: a comparative serological study of dogs and foxes in Amazon Brazil. Parasitology 109(Pt 3): 273–279.
  70. 70. Corredor A, Gallego JF, Tesh RB, Pelaez D, Diaz A, et al. (1989) Didelphis marsupialis, an apparent wild reservoir of Leishmania donovani chagasi in Colombia, South America. Trans R Soc Trop Med Hyg 83: 195.
  71. 71. Corredor A, Gallego JF, Tesh RB, Morales A, De Carrasquilla CF, et al. (1989) Epidemiology of visceral leishmaniasis in Colombia. Am J Trop Med Hyg 40: 480–486.
  72. 72. Travi BL, Jaramillo C, Montoya J, Segura I, Zea A, et al. (1994) Didelphis marsupialis, an important reservoir of Trypanosoma (Schizotrypanum) cruzi and Leishmania (Leishmania) chagasi in Colombia. Am J Trop Med Hyg 50: 557–565.
  73. 73. Sherlock IA, Miranda JC, Sadigursky M, Grimaldi G Jr (1984) Natural infection of the opossum Didelphis albiventris (Marsupialia, Didelphidae) with Leishmania donovani, in Brazil. Mem Inst Oswaldo Cruz 79: 511.
  74. 74. Schallig HD, da Silva ES, van der Meide WF, Schoone GJ, Gontijo CM (2007) Didelphis marsupialis (common opossum): a potential reservoir host for zoonotic leishmaniasis in the metropolitan region of Belo Horizonte (Minas Gerais, Brazil). Vector Borne Zoonotic Dis 7: 387–393.
  75. 75. Courtenay O, Quinnell RJ, Garcez LM, Dye C (2002) Low infectiousness of a wildlife host of Leishmania infantum: the crab-eating fox is not important for transmission. Parasitology 125: 407–414.
  76. 76. de Pita-Pereira D, Cardoso MA, Alves CR, Brazil RP, Britto C (2008) Detection of natural infection in Lutzomyia cruzi and Lutzomyia forattinii (Diptera: Psychodidae: Phlebotominae) by Leishmania infantum chagasi in an endemic area of visceral leishmaniasis in Brazil using a PCR multiplex assay. Acta Trop 107: 66–69.
  77. 77. Watts PC, Hamilton JG, Ward RD, Noyes HA, Souza NA, et al. (2005) Male sex pheromones and the phylogeographic structure of the Lutzomyia longipalpis species complex (Diptera: Psychodidae) from Brazil and Venezuela. Am J Trop Med Hyg 73: 734–743.
  78. 78. Mestre GL, Fontes CJ (2007) [The spread of the visceral leishmaniasis epidemic in the State of Mato Grosso, 1998–2005]. Rev Soc Bras Med Trop 40: 42–48.
  79. 79. dos Santos SO, Arias J, Ribeiro AA, de Paiva Hoffmann M, de Freitas RA, et al. (1998) Incrimination of Lutzomyia cruzi as a vector of American visceral leishmaniasis. Med Vet Entomol 12: 315–317.
  80. 80. Brazil RP, Hamilton JG (2002) Isolation and identification of 9-methylgermacrene-B as the putative sex pheromone of Lutzomyia cruzi (Mangabeira, 1938) (Diptera: Psychodidae). Mem Inst Oswaldo Cruz 97: 435–436.
  81. 81. Ribeiro AL, Missawa NA, Zeilhofer P (2007) Distribution of phlebotomine sandflies (Diptera: Psychodidae) of medical importance in Mato Grosso State, Brazil. Rev Inst Med Trop Sao Paulo 49: 317–321.
  82. 82. Missawa NA, Lima GB (2006) [Spatial distribution of Lutzomyia longipalpis (Lutz & Neiva, 1912) and Lutzomyia cruzi (Mangabeira, 1938) in the State of Mato Grosso]. Rev Soc Bras Med Trop 39: 337–340.
  83. 83. Vigoder FM, Araki AS, Bauzer LG, Souza NA, Brazil RP, et al. (2010) Lovesongs and period gene polymorphisms indicate Lutzomyia cruzi (Mangabeira, 1938) as a sibling species of the Lutzomyia longipalpis (Lutz and Neiva, 1912) complex. Infect Genet Evol 10: 734–739.
  84. 84. Thomaz-Soccol V, Lanotte G, Rioux JA, Pratlong F, Martini-Dumas A, et al. (1993) Phylogenetic taxonomy of New World Leishmania. Ann Parasitol Hum Comp 68: 104–106.
  85. 85. Thomaz-Soccol V, Lanotte G, Rioux JA, Pratlong F, Martini-Dumas A, et al. (1993) Monophyletic origin of the genus Leishmania Ross, 1903. Ann Parasitol Hum Comp 68: 107–108.
  86. 86. Kreutzer RD, Souraty N, Semko ME (1987) Biochemical identities and differences among Leishmania species and subspecies. Am J Trop Med Hyg 36: 22–32.
  87. 87. Rioux JA, Lanotte G, Serres E, Pratlong F, Bastien P, et al. (1990) Taxonomy of Leishmania. Use of isoenzymes. Suggestions for a new classification. Ann Parasitol Hum Comp 65: 111–125.
  88. 88. Cupolillo E, Grimaldi G Jr, Momen H (1995) Discrimination of Leishmania isolates using a limited set of enzymatic loci. Ann Trop Med Parasitol 89: 17–23.
  89. 89. Waki K, Dutta S, Ray D, Kolli BK, Akman L, et al. (2007) Transmembrane molecules for phylogenetic analyses of pathogenic protists: Leishmania-specific informative sites in hydrophilic loops of trans- endoplasmic reticulum N-acetylglucosamine-1-phosphate transferase. Eukaryot Cell 6: 198–210.
  90. 90. Kuhls K, Mauricio IL, Pratlong F, Presber W, Schonian G (2005) Analysis of ribosomal DNA internal transcribed spacer sequences of the Leishmania donovani complex. Microbes Infect 7: 1224–1234.
  91. 91. Mauricio IL, Stothard JR, Miles MA (2004) Leishmania donovani complex: genotyping with the ribosomal internal transcribed spacer and the mini-exon. Parasitology 128: 263–267.
  92. 92. Mauricio IL, Gaunt MW, Stothard JR, Miles MA (2001) Genetic typing and phylogeny of the Leishmania donovani complex by restriction analysis of PCR amplified gp63 intergenic regions. Parasitology 122: 393–403.
  93. 93. Courtenay O, Santana EW, Johnson PJ, Vasconcelos IA, Vasconcelos AW (1996) Visceral leishmaniasis in the hoary zorro Dusicyon vetulus: a case of mistaken identity. Trans R Soc Trop Med Hyg 90: 498–502.
  94. 94. Volf P, Myskova J (2007) Sand flies and Leishmania: specific versus permissive vectors. Trends Parasitol 23: 91–92.
  95. 95. Myskova J, Svobodova M, Beverley SM, Volf P (2007) A lipophosphoglycan-independent development of Leishmania in permissive sand flies. Microbes Infect 9: 317–324.