Colonization and genetic diversification processes of Leishmania infantum in the Americas

Schwabl, Philipp; Boité, Mariana C.; Bussotti, Giovanni; Jacobs, Arne; Andersson, Bjorn; Moreira, Otacilio; Freitas-Mesquita, Anita L.; Meyer-Fernandes, Jose Roberto; Telleria, Erich L.; Traub-Csekö, Yara; Vaselek, Slavica; Leštinová, Tereza; Volf, Petr; Morgado, Fernanda N.; Porrozzi, Renato; Llewellyn, Martin; Späth, Gerald F.; Cupolillo, Elisa

doi:10.1038/s42003-021-01658-5

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Published: 29 January 2021

Colonization and genetic diversification processes of Leishmania infantum in the Americas

Communications Biology volume 4, Article number: 139 (2021) Cite this article

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Abstract

Leishmania infantum causes visceral leishmaniasis, a deadly vector-borne disease introduced to the Americas during the colonial era. This non-native trypanosomatid parasite has since established widespread transmission cycles using alternative vectors, and human infection has become a significant concern to public health, especially in Brazil. A multi-kilobase deletion was recently detected in Brazilian L. infantum genomes and is suggested to reduce susceptibility to the anti-leishmanial drug miltefosine. We show that deletion-carrying strains occur in at least 15 Brazilian states and describe diversity patterns suggesting that these derive from common ancestral mutants rather than from recurrent independent mutation events. We also show that the deleted locus and associated enzymatic activity is restored by hybridization with non-deletion type strains. Genetic exchange appears common in areas of secondary contact but also among closely related parasites. We examine demographic and ecological scenarios underlying this complex L. infantum population structure and discuss implications for disease control.

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Introduction

Species invasion creates unique opportunity for extreme evolutionary transformation. Small founding populations face unfamiliar selection pressures and sampling effects that drive genetic drift. Rapid changes in genetic makeup can occur and potentially dictate long-term population genetic structure throughout the invasive range¹. Subsequent secondary introductions into the same area can also reshape diversity patterns in the population, e.g., by promoting introgressive hybridization events between ancestrally allopatric groups². One medically relevant but little explored example of species invasion is represented by the introduction of Leishmania infantum, the parasitic agent of visceral leishmaniasis (VL), into the New World in conjunction with European colonization of the Americas beginning ca. 500 years ago^3,4. Population structure and genetic change in Leishmania populations are of major concern to public health, as intra-specific genetic variation within this genus is associated with major differences in pathology^5,6,7, drug resistance^8,9, and other eco-epidemiological traits^10,11. Driven in part by high karyotypic plasticity^12,13, Leishmania parasites are capable of rapid adaptation and epidemic expansion after environmental change and/or bottleneck events⁸. Genetic recombination among L. infantum populations is another potential source of phenotypic diversity. Hybridization between divergent Leishmania isolates and species that cause distinct forms of disease¹⁴ can impact pathogenicity^14,15,16, as well as facilitate vector¹⁷ and geographic range expansion¹⁸.

In the Americas, VL is a zoonosis caused by L. infantum infecting Lutzomyia sandflies, which have evolved in isolation of Phlebotomus, the Old World vector genus, for ca. 200 million years¹⁹. Domestic dogs represent principal reservoir hosts. The New World distribution of L. infantum now extends from the southern United States to northern Argentina²⁰ and Uruguay²¹, but prevalence and/or reporting varies considerably across this range. Over 1000 VL cases have been recorded yearly in Brazil since the 1980s, first limited to the Northeast²² but now increasingly dispersed, including in urban areas such as those in Mato Grosso, Minas Gerais, and São Paulo state. VL infections are significantly less common elsewhere on the continent compared to Brazil²³. Atypical cases, e.g., involving dermotropic or, more rarely, drug-resistant L. infantum isolates, are also sporadically observed in the New World^24,25,26, but direct links between changes in disease progression and specific host or parasite factors are rarely established. A recently published genome-wide association study²⁷, however, reports that L. infantum populations from Piauí, Maranhão, and Minas Gerais (Brazil) show resistance to miltefosine, an important anti-leishmanial drug, and associates this resistance to a large (>12 kb) deletion said to increase in prevalence from northern to southeastern Brazil (e.g., 5% in Rio Grande do Norte and 95% in Minas Gerais). The deletion is homozygous, spanning across all four copies of tetrasomic chromosome 31 (chr31). It covers four open reading frames as follows: LinJ.31.2370 (ecto-3′-nucleotidase/nuclease), LinJ.31.2380 (ecto-3’-nucleotidase precursor), LinJ.31.2390 (helicase-like protein), and LinJ.31.2400 (3,2-trans-enoyl-CoA isomerase). Ecto-3’-nucleotidases take part in purine salvage, macrophage infection, and escape from neutrophil extracellular traps^28,29,30. Helicases are essential to DNA replication and 3,2-trans-enoyl-CoA isomerase contributes to fatty acid oxidation, a critical component of gluconeogenesis in amastigote parasite forms³¹. The simultaneous deletion of these four genes likely occurs through homologous recombination between repetitive elements bordering the deletion site^27,32. The mechanisms by which the sub-chromosomal deletion has emerged in multiple different areas of Brazil, however, remain completely unknown. Its abundance and geographic distribution are also only rudimentarily described²⁷. Analyses of demographic history, epidemiological phenotypes, and genetic covariation in deletion-carrying isolates are urgently required to clarify the emergence of the deletion genotype, quantify its spread, and understand implications for disease treatment and control.

The present study expands surveillance for the sub-chromosomal deletion into 17 states of Brazil, establishing that deletion-carrying isolates occur abundantly in both the country’s North and South. Although non-deletion genotypes appear common in the northern state of Piauí, a North-South gradient in chr31 deletion abundance (previously suggested to increase miltefosine treatment efficacy in Rio Grande do Norte²⁷) does not occur in the dataset. Non-deletion type strains also appear common in the southwestern state of Mato Grosso do Sul. We go on to explore sequence diversity in 126 L. infantum genomes (59 newly sequenced in this study and 67 others from publicly archived datasets representing Brazil^27,33, Honduras³⁴, Panama³⁴, Morocco³⁵, and Europe³⁴) in search of adaptive and/or demographic drivers of the widespread deletion genotype and discontinuous population structures in the New World. We describe phylogenetic relationships characteristic of one or few early ancestral mutant groups having risen to high prevalence by founder effect and observe a possible compensation for reduced ecto-3’-nucleotidase activity via increased ecto-ATPase activity in deletion-carrying isolates. We also demonstrate restored ecto-3’-nucleotidase activity in parasites with partial (heterozygous) sub-chromosomal deletion that clearly derive from natural mating between divergent deletion-carrying and non-deletion isolates. Several hybridizations appear to involve a secondary contact (SC) process in the West of Brazil but endogamic mating is also apparent in several states. Our results suggest a dynamic and yet incompletely charted distribution of L. infantum diversity in the New World. Volatile genotypes and biomarkers in this introduced range must be precisely monitored for effective disease control.

Results

High prevalence of multi-kilobase deletion on chr31

Comparative analysis of 126 L. infantum genomes (19 from the Old World, 107 from the New World) and quantitative PCR (qPCR) screening of 75 additional New World samples (Supplementary Data 1) confirmed the occurrence of a >12 kb homozygous deletion on tetraploid chr31 (see somy values in Supplementary Fig. 1), previously described as a miltefosine sensitivity locus by Carnielli et al.²⁷. The deletion occurred in samples from Brazil (126 of 177) and Honduras (2 of 2) but was absent from the Old World (0 of 19)³⁴. New World samples without the deletion (referred to as “NonDel” as opposed to “Del” in subsequent whole-genome sequencing (WGS) analyses) were concentrated primarily in the Brazilian states of Piauí (20 of 38) and Mato Grosso do Sul (12 of 12) but they also occurred in Bolivia (1 of 1) and, as recently noted³⁴, in Panama (2 of 2) (Supplementary Data 1 and Fig. 1). The deleted region spans chr31 base pair positions 1,122,848 to 1,135,161 in most Del samples (but see slight mapping variability within repetitive boundary regions in Supplementary Data 2) and comprises genes encoding for ecto-3’-nucleotidase (LinJ.31.2370), ecto-3’-nucleotidase precursor (LinJ 31.2380), helicase-like protein (LinJ 31.2390), and 3-2-trans-enoyl-CoA isomerase (LinJ.31.2400). Apart from these four genes, 38 coding regions showed significant copy number variation (CNV) between Del and New World NonDel groups in haploid somy estimate (s) comparison using Mann–Whitney U (MWU)-tests (Supplementary Data 3), but reassessment by analysis of covariance (ANCOVA) suggested that most of these differences are driven by population structure, i.e., common descent. Supplementary Fig. 2 illustrates how CNV profiles cluster by geographic origin, and geographic origin correlates to chr31 read-depth profile. The five coding regions, which remained significantly differentiated between Del and New World NonDel groups after controlling for geographic origin, encode amastin-like protein, nucleoside transporter, and paraflagellar rod protein paralogs (see asterisked columns in Supplementary Fig. 2). Effect size, however, is low (0.317 ≤ |∆s | ≤ 0.552) (Supplementary Data 3). We also did not note any substantial evidence for a direct relationship between the presence of deletion on chr31 and single-nucleotide polymorphism (SNP) or insertion-deletion variant (INDEL) differentiation among New World isolates (Supplementary Note 1, Supplementary Fig. 3, and Supplementary Data 4 and 5).

**Fig. 1: Different read-depth profiles found in *L. infantum* isolates from Brazil.**

Partial deletions occur via hybridizations between Del and NonDel isolates

Six L. infantum samples sequenced in this study had an intermediate read-depth profile within the chr31 deletion site (Supplementary Data 1). In such genotypes, sequences mapped to the deletion site achieve ~50% read coverage relative to the rest of the chromosome (Supplementary Fig. 4), suggesting one of two scenarios: an abundance of cells with “equivalent” heterozygous sub-chromosomal deletion (i.e., cells in which two copies of chr31 carry the deletion and two copies do not) or an equally mixed population of Del and NonDel isolates. We therefore extracted DNA from 11 monoclonal subcultures established from two isolates representing putative heterozygotes (IOCL 2949 and 3134) and measured relative abundance of the deletion target by qPCR. Results from ten monoclonal subcultures showed a reduction of ca. 50% in the abundance of the amplified target sequence relative to the NonDel representative NonDel_MS_2666 (Fig. 2), confirming the presence of cells heterozygous at the deletion locus as opposed to a mix of (homozygous) Del and NonDel genotypes. Clone 2949 G1 showed 25% relative target amplification (Fig. 2b), suggesting the presence of three chromosome copies with the deletion and one copy without. Subpopulations with different levels of heterozygosity appear to occur but equivalent heterozygotes—i.e., cells in which two copies of chr31 carry the deletion and two copies do not—appear most abundant based on read-depths from parental culture sequencing (Supplementary Fig. 4). Aside from these six isolates (hereafter termed “HTZ”), seven isolates sequenced by Carnielli et al.²⁷ simultaneously showed Del and NonDel deletion site PCR amplicons in the previous study but ca. 80–100% read-depth within the deletion site (Supplementary Fig. 4). We refer to these samples as “MIX” without resolving the extent to which their sequence reads represent mixed-strain or monoclonal cell populations.

**Fig. 2: Quantitative PCR confirms that intermediate read-depth profiles represent heterozygous deletions in *L. infantum* clones.**

Given the vast geographic range occupied by Del isolates (Fig. 1), we considered the possibility of independent deletion emergence as an adaptive process recurring frequently across the American continent. Under such scenario, HTZ isolates might represent former NonDel genotypes currently in transition to the homozygous (i.e., complete, fourfold) deletion state. This NonDel to Del transition might occur via successive independent locus deletion on different chromosome copies or via locus deletion on a single chromosome copy followed by over-replication of the deletion-containing copy and under-replication of non-deletion copies during mitosis. Following ADMIXTURE analysis (Supplementary Fig. 5), however, in which HTZ_MT_3134, HTZ_MT_3135, HTZ_MT_3137, HTZ_MT_3224, and HTZ_SP_3254 (i.e., all HTZ samples, except HTZ_PI_2949) received simultaneous Del + NonDel group assignment, we also considered the alternate hypothesis that HTZ isolates represent hybrid offspring forming at contact zones between Del and NonDel groups (Fig. 1). Support for this alternate hypothesis quickly accumulated through several analyses and metrics.

HTZ samples showed marked, statistically significant reductions in total homozygosity and F_IS values (which describe the extent to which individual heterozygosity is reduced by inbreeding) relative to Del and to New World NonDel isolates (Fig. 3a and Supplementary Data 6). Median F_IS was lowest in HTZs (relative to Del and New World NonDel groups) in 33 of 36 chromosomes (Fig. 3b). Except for HTZ_PI_2949, HTZs occurred in peripheral positions relative to monophyletic Del subclades in maximum-likelihood phylogeny (Fig. 4) and showed intermediate positions on PCoA axis 1 (Fig. 5a). We also constructed neighbor-joining trees from phased chromosomes (Supplementary Fig. 6) and homologous haplotypes of Mato Grosso HTZ isolates generally divided between Mato Grosso Del and Mato Grosso do Sul NonDel clades (i.e., one HTZ haplotype appearing similar to both haplotypes of Mato Grosso Del isolates and the other HTZ haplotype appearing more similar to both haplotypes of NonDel isolates from Mato Grosso do Sul). This divided HTZ haplotype clustering suggested a process of nuclear genetic exchange in which homologous chromosomes from distinct progenitors are found within hybrid offspring, consistent with sexual mating or, less parsimoniously (because ploidy levels did not appear aberrant (Supplementary Fig. 1)), genome fusion events. F_ST differentiation to Mato Grosso do Sul samples also fluctuated among HTZ chromosomes, consistent with chromosomal reassortment as a result of mating between Del and NonDel isolates (Supplementary Fig. 7). We further examined a potential hybrid origin by comparing the phylogenetic positions of HTZ isolates from Mato Grosso with those generated by simulated sexual mating (see Supplementary Codes³⁶) between populations from Mato Grosso and nearby Mato Grosso do Sul. Phylogenetic positions for simulated hybrids corresponded to those observed for HTZ isolates (Fig. 5b). In these simulations, we also hypothesized the presence of second-generation (F₂) hybrids, i.e., we simulated backcrossing and hybrid inter-crossing to account for the origin of Mato Grosso samples Del_MT_3223 and NonDel_MT_3210 (respectively). These two samples are not heterozygous for the deletion on chr31 but show low genome-wide F_IS (Fig. 3a) and place near HTZ samples in Principal Coordinates Analysis (PCoA) (Fig. 5a). Phylogenetic positions of the simulated F₂ hybrids matched those observed for Del_MT_3223 and NonDel_MT_3210. Similar F₂ hybridization events may also explain the outlying phylogenetic positions of samples such as NonDel_MG_14A or NonDel_MS_2688 (Figs. 4 and 5a, and Supplementary Fig. 6).

**Fig. 3: Homozygosity relative to Hardy–Weinberg expectations in New and Old World *L. infantum* isolates.**

**Fig. 4: Phylogenetic relationships among New and Old World *L. infantum* isolates.**

**Fig. 5: Metric multidimensional scaling, simulated mating, and tree-to-graph conversion suggest admixture and hybridization between Del and NonDel *L. infantum* groups.**

Demographic drivers of patchy population structure and hybridization events

The L. infantum group from Mato Grosso do Sul stood out in above analyses given its complete lack of Del genotypes and its basal phylogenetic position relative to all other New World isolates (Fig. 4). This outgroup also showed higher nucleotide diversity (π) per site (0.046 vs. 0.061, respectively), more than twice as many private SNP sites per sample (15.3 vs. 31.8) and lower F_ST-differentiation to Old World isolates (0.413 vs. 0.303) than did the rest of the New World sample set (Table 1).

Table 1 Population genetic descriptive metrics for New World and Old World L. infantum groups.

Full size table

We used a pattern-process modeling approach to better understand the divergence history of the MS group and its paths to contemporary admixture with Mato Grosso isolates. We considered a “SC” model of divergence, in which Mato Grosso do Sul parasites diverged in isolation from Mato Grosso parasites but later reestablished gene flow, perhaps due to separate introductions from the Old World into Brazil. Alternatively, Mato Grosso do Sul and Mato Grosso groups may have followed an “isolation with migration” (IM) model of divergence, whereby gene flow between them never fully ceased but Mato Grosso do Sul parasites underwent significant divergence due to local selection pressures or secondary bottleneck events. For both SC and IM models, we simulated individual genome-wide SNP diversity in three variations relating to bottleneck (yes/no in Mato Grosso founder population), admixture type (hard introgression and/or permanent migration vs. temporary genetic exchange), and rate of gene flow (constant or variable over time). We also ran simulations for two implausible models of Mato Grosso do Sul—Mato Grosso divergence, “strict isolation” (SI, i.e., gene flow between the two populations permanently ceased) and “ancient migration” (AM, i.e., gene flow between the two populations permanently ceased following an early period of continuous gene flow). These served as “negative” controls for the Approximate Bayesian Computation via Random Forests (ABCRF)³⁷ method, which uses random forests to rank the fit of observed vs. simulated summary statistics. Simulations for Mato Grosso do Sul—Old World and Mato Grosso—Old World population pairs, both assumed to follow an AM with bottleneck (AM_bot) model of divergence, provided additional “positive” controls (see fastsimcoal2³⁸ template files and model illustrations in Supplementary Data 7, see Supplementary Codes³⁶, and Supplementary Fig. 8). Following expectations, the AM_bot model achieved highest support for both Mato Grosso do Sul—Old World and Mato Grosso—Old World divergence (Table 2). Also as expected, AM and SI models received lowest (near zero) support for the Mato Grosso do Sul—Mato Grosso population pair. Support was highest for the SC base model (350 of 1000 votes, Table 2), with subsequent parameter optimization specifying slightly higher gene flow (Migration - MIG) towards Mato Grosso than towards Mato Grosso do Sul (Table 2) as also previously indicated by tree-to-graph optimization and F₄-statistics (Fig. 5c). The IM_change model, which suggests that rate of gene flow between Mato Grosso do Sul and Mato Grosso changed but never fully ceased over time, received the second-highest support (253 votes). Overall posterior probability (0.504), however, was low due to the inclusion of two highly similar additional variants of each IM and SC base model in analysis (Table 2). We therefore re-ran the ABCRF process using only the four base models SC, IM, SI, and AM. In this analysis, the SC model achieved a much clearer majority (627 votes) over IM (264), SI (65), and AM (44), and posterior probability rose to 61%. Taken together, the above analyses suggest that hybrid genotypes observed in Mato Grosso involve a SC process after the bottlenecking of L. infantum from the Old World into Brazil. It remains to be established, however, if Mato Grosso do Sul and Mato Grosso parasites temporarily diverged in isolation due to independent importations or whether temporary isolation began after common introduction to the New World.

Table 2 Demographic simulation in fastsimcoal2 and model selection by Approximate Bayesian Computation via Random Forests (ABCRF).

Full size table

Introgression disrupts monophyletic ancestry of Del isolates

In light of the ample evidence for frequent hybridization described above, but also positive inbreeding coefficients in most samples (Fig. 3a), we wondered whether mating between more similar Del and NonDel genotypes likewise occurs frequently in Brazil. This possibility appeared especially relevant in the case of Piauí and Maranhão isolates NonDel_MA_01A, NonDel_MA_03A, NonDel_PI_07A, NonDel_PI_12A, and NonDel_PI_2972, as these were the only NonDel isolates which nested within what otherwise appeared as a Del-exclusive, monophyletic clade (Fig. 4). NonDel_PI_2972 featured the highest genome-wide F_IS value of any NonDel sample (Fig. 3a), and NonDel_MA_03A, NonDel_PI_07A and NonDel_PI_12A shared the dataset’s highest F_IS value for chr31 (F_IS = 0.92). Of all large (>1 Mb) chromosomes (i.e., chromosomes 26 to 36), chr31 ranked highest in F_IS for these 3 samples and for NonDel_MA_01A (F_IS = 0.85). For all other samples, the median rank of F_IS for chr31 relative to other large chromosomes was 3.

We also noted that F_ST between the nested NonDel clade and phylogenetically similar Del isolates increased specifically on chr31 (Supplementary Fig. 7), showing higher values only on the (small) chromosomes 3 and 16 and near zero (i.e., no differentiation) on most other chromosomes. This subtle chr31-specific divergence from Del isolates was not statistically significant (Tukey and Kramer (Nemenyi) test) but was substantiated by analysis focused on “Del-distinctive” sites, i.e., sites at which >90% of Del isolates and <50% of New World NonDel isolates show non-reference genotypes. Of 470 such Del-distinctive sites, 466 also showed a non-reference genotype in at least one member of the nested NonDel group. The remaining 4 sites, however, all occurred on chr31 (nucleotide positions 387,322, 423,106, 1,254,441, and 1,390,994). Chr31-specific divergence was also exposed by running ADMIXTURE analysis at k = 2 separately for all large chromosomes in New World isolates, excluding the putatively outcrossing groups Mato Grosso and Mato Grosso do Sul. The cumulative total of all individual Del ancestry proportions matching the Piauí/Maranhão NonDel population assignment was only 15% for chr31 as opposed to 61% for chr26, 56% for chr27, 81% for chr28, 54% for chr29, 75% for chr30, 71% for chr32, 74% for chr33, 66% for chr34, 46% for chr35, and 37% for chr36.

These observations are consistent with the hypothesis that the nesting of Piauí/Maranhão NonDel isolates in Fig. 4 represents an admixture process between Del isolates and closely related NonDel isolates, whereby introgression of polymorphisms on chr31 may be preserved more so than on other chromosomes during subsequent backcrossing or mitotic haplotype selection events¹³. This possibility of introgression perturbing Del monophyly is also supported by evaluating the likelihood of trees constructed under a constraint that forces Piauí/Maranhão NonDel isolates to group outside of the Del clade, specifically, applying newick constraint = ((Piauí/Maranhão NonDel isolates, Mato Grosso do Sul NonDel isolates), (all Del isolates)). The Shimodaira–Hasegawa test³⁹ suggests that maximum likelihood resulting from such constrained tree construction is not significantly lower than that of Fig. 4’s unconstrained maximum-likelihood tree (p = 0.431). A constraint forcing Honduran Del samples out of the Del clade, by contrast, does result in a significantly less likely tree (p = 0.045), further substantiating the geographically widespread expansion of a monophyletic Del clade. Nevertheless, we cannot conclude definitively whether the deletion found in all isolates of this clade stems from a single ancestral mutant lineage or if multiple, closely related ancestral lineages experienced separate deletion events (see Supplementary Notes 2 and 3, which describe a phylogenetic signal on deletion stop site coordinates listed in Supplementary Data 2; although stop site variation is minimal, its phylogenetic signal raises the possibility that distinct deletion mutations or post-deletion modifications occurred among progenitors the Del clade).

Phenotypic consequences of the sub-chromosomal deletion

Finally, we performed an assay for ecto-3’-nucleotidase activity (Fig. 6a) in Del, NonDel, and HTZ samples representing different levels of phylogenetic similarity and various states of Brazil. Results demonstrate heavily reduced ecto-3’-nucleotidase activity in Del isolates relative to HTZ and NonDel isolates (p < 0.05) (despite no polymorphisms observed in an ecto-3’-nucleotidase paralogue present on chr12). Inter-individual variation in ecto-3’-nucleotidase activity also occurred among NonDel and HTZ samples: NonDel_SC_3737 showed significantly higher activity than all other NonDel and HTZ samples (p < 0.05) and NonDel_PI_2972 showed significantly higher activity than monoclonal HTZ subcultures HTZ_3134_B1 and HTZ_2949_B2 (p < 0.05). Activity in these two subcultures did not significantly differ to that in the uncloned HTZ isolate HTZ_MT_3134 (p < 0.05). We also measured the activity of ecto-ATPase (an enzyme thought to be involved in purine salvage pathways^40,41 independent of ecto-3’-nucleotidase) in Del and NonDel isolates (Fig. 6b). Higher ecto-ATPase activity occurred in Del isolates than in NonDel isolates (p < 0.05), suggesting the possibility that alternative molecular pathways compensate effects of ecto-3’-nucleotidase deletion on chr31.

**Fig. 6: Ecto-3’-nucleotidase and ecto-ATPase activity correlates to read-depth profiles on chr31.**

Discussion

Our results reveal the widespread distribution of a major genetic alteration found in New World L. infantum isolates, clarifying that a four-gene deletion on chr31 predominates in southeastern, eastern, and (unlike previously suggested²⁷) northeastern Brazil. In addition to two Panamanian non-MON-1 samples that do not show this drug resistance-associated mutation³⁴, a divergent non-deletion group occurs in the southwestern Brazilian state of Mato Grosso do Sul. Coalescence modeling suggests a SC process between these divergent NonDel parasites and members of the widespread, likely monophyletic, Del clade. This admixture involves genome-wide hybridization events that transfer Del chr31 homologs into paraphyletic NonDel groups. Genetic exchange between closely related Del and NonDel strains, followed by further inbreeding and/or mitotic haplotype selection¹³, may also explain the presence of NonDel isolates with high homozygosity and low (chromosome-specific) divergence to Del strains in other regions of Brazil, e.g., in Piauí and Maranhão.

The extensive evidence of genetic exchange we describe substantiates the importance of this process in trypanosomatid evolution. We observed a direct effect of hybridization on phenotype, showing substantially higher activity of the potential virulence factor ecto-3’-nucleotidase⁴⁰ in putative F₁ hybrids relative to parental Del genotypes. Changes to human pathogenicity are also directly implied by the association between locus deletion and miltefosine treatment efficacy suggested by Carnielli et al.²⁷. Our observations add to a growing body of evidence that genetic exchange plays an important role in the spread of epidemiologically relevant traits through natural trypanosomatid populations (e.g., drug resistance in Leishmania donovani⁹, vector infectivity in Leishmania major/L. infantum¹⁷, and human infectivity in Trypanosoma brucei^42,43) and are consistent with a “mixed mating model of reproduction”⁴⁴ in the Leishmania genus. Similar to observations in Trypanosoma cruzi⁴⁵, different rates of sex and clonality may occur in L. infantum depending on demographic or ecological variation within landscapes or between the parasite’s evolutionarily native (Old World) and introduced (New World) range. Our study suggests that hybridization occurs frequently at SC zones as well as the possibility that mating is generally common, and perhaps advantageous, in non-native and/or bottlenecked groups. Plasmodium parasites, e.g., have been suggested to alter sex allocation and inbreeding rates to enhance success in the mosquito vector, with rates dependent on the diversity of sympatric strains^46,47.

This study also substantiates that CNV is a highly heritable form of polymorphism in the Leishmania genus⁴⁸. In genome-wide read-depth analysis excluding the focal deletion on chr31, CNV-based hierarchical clustering mirrored the SNP-based phylogeny and geographical origins of the sample set, suggesting that baseline gene copy numbers or deletion/amplification programs triggered in vitro are conserved among related isolates. Results do not suggest that any single CNV regime underlies enzymatic changes (e.g., ecto-ATPase upregulation) that might be occurring to compensate loss of function within the deleted locus on chr31. Such compensation may occur through unique (i.e., sample specific) CNV solutions or by various other epigenetic, post-transcriptional or posttranslational effects. The five copy number differences showing statistical significance between Del and New World NonDel groups do nevertheless deserve further investigation. Effect sizes were small but the transport (LinJ.08.0700, LinJ.15.1240, LinJ.15.1250) and cytoskeletal (LinJ.29.1880, LinJ.29.1890) proteins involved carry out vital cell functions, variation in which has also been linked to drug resistance in previous research^49,50,51.

Taken together, this study highlights the pivotal roles and interplay of genetic exchange and demographic history in shaping L. infantum sequence and karyotypic diversity in the New World. Although the importance of genetic exchange has been increasingly appreciated in recent years, the consequences of post-Columbian range expansion in this species are seldom acknowledged and remain poorly understood. The process is often simplified as yielding a low-diversity, homogeneous L. infantum population, one which might display clinical variation due to environmental or host-related factors but less likely due to parasite genetic traits⁵². Our observations reject such scenario and open up many new questions on the different sources and yet unknown extent of L. infantum diversity in the New World. For example, could distinct local selection pressures (e.g., the presence of Lutzomyia cruzi as opposed to Lutzomyia longipalpis) contribute to the success of a separately introduced parasite population in Mato Grosso do Sul? Might this population, and other unobserved populations, involve importations from different colonial empires, e.g., the French or Spanish, aside from the Portuguese⁵³? Does the widespread distribution of Del genotypes in the Americas reflect fitness advantages within the parasite’s narrow host/vector spectrum in the New World? Could reduced virulence as a consequence of reduced ecto-3’-nucleotidase activity play a role in the predominance of Del strains? Alternatively, is locus deletion neutral or deleterious, and the widespread distribution of deletion-carrying strains is principally an allele surfing effect (a phenomenon in which new mutations spread rapidly across new territories due to their emergence on an expanding wave front, where population density is low and growth rates are high⁵⁴)? We hope that this study inspires much new research on such questions and recommend greater attention to complex L. infantum population structure and hidden genetic diversity in future disease control.

Methods

Parasite samples and whole-genome sequencing

All 201 L. infantum samples assessed in this study are listed in Supplementary Data 1, which also provides information on alternative nomenclatures, geographic origin, chr31 read-depth profile (i.e., whether or not isolates carry the sub-chromosomal deletion described by Carnielli et al.²⁷) and analysis type (i.e., WGS analysis or quantitative real-time PCR). All 59 L. infanum strains sequenced in this study were obtained from the Coleção de Leishmania da Fundação Oswaldo Cruz (CLIOC). 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. All strains were cultured in biphasic (Novy–MacNeal–Nicolle (NNN) + Schneider’s) medium prior to genomic DNA extraction (DNeasy Blood & Tissue Kit (Qiagen). Fragmented DNA (mean insert size = 377 nt) was sequenced using Illumina NextSeq 500 and HiSeq 2500 instruments, and mapped to the MCAN/ES/98/LLM-724 (termed JPCM5 elsewhere in the text) reference assembly available at https://tritrypdb.org/common/downloads/release-33/LinfantumJPCM5/fasta/ using default settings for BWA-mem v0.7.3⁵⁵. Publicly archived and/or previously published L. infantum reads^27,33,34,35 were mapped using the same conditions as the newly generated WGS data (see mapping coverage per sample in Supplementary Data 1). For enzymatic assays (see below), parasites were cultivated in flasks containing Schneider’s medium with 20% fetal calf serum (FCS) and 2% filtered urine until late log-phase expansion. Growth curves were obtained to rule out samples with possible confounding differences in replication rate. All parasites used in the experiments showed similar replication rates. These parasites had been kept in culture between 10 and 20 passages after isolation and cryopreservation by CLIOC.

Phylogenetic, demographic modeling, and selection analyses

SNPs and INDELs were called using population-based genotype and likelihood assignment in Genome Analysis Toolkit (GATK) v3.7.0⁵⁶ (programs “HaplotypeCaller” and “GenotypeGVCFs”). We excluded tightly clustered variants (i.e., more than three SNPs or INDELs within ten bases) as well as those achieving <1500 phred-scaled call quality (QUAL as calculated by GATK). We also excluded variants detected in non-unique mapping positions of the reference genome. Specifically, we generated synthetic, non-overlapping 125 nt sequence reads from the JPCM5 reference assembly (excluding unassigned contigs) and mapped these reads back to this same assembly using the “mappability” program in the Genomic Multi-tool software suite v1.376^57,58. Only variants from areas with perfect synthetic mapping coverage were retained. The above filtering decisions were guided by results for the JPMC5 reference strain (re-sequenced in this study using paired-end 2 × 150 nt Illumina NextSeq).

We visualized genome-wide phylogenetic relationships among samples by maximum-likelihood tree construction in IQ-Tree v1.5.4⁵⁹, optimizing a general time-reversible substitution model based on single-nucleotide differences at polymorphic sites. The pseudo-sequence alignment used as input for IQ-tree was generated without phasing, assuming allele order as reference allele first and alternate allele second at heterozygous sites. L. donovani isolate MHOM/NP/03/BPK282/0 was temporarily included as an outgroup in order to root the tree. Five samples were excluded from the tree and all other SNP/INDEL-based analyses due to radical divergence from the rest of the sample set. These were NonDel_MS_MAM (likely a mixture of divergent strains³⁴), NonDel_PA_317 and NonDel_PA_85 (both non-MON-1³⁴), and NonDel_FR_47 and NonDel_PT_151 (reason for divergence unclarified). Euclidean dissimilarities among genotypes were visualized by metric multidimensional scaling (PCoA)⁶⁰ using the base “stats” package v3.4.1 in R v3.4.1⁶¹. Ancestry estimation was performed using ADMIXTURE v1.3⁶² (using all SNPs for which genotypes were called in all individuals) and putative first-generation (F₁) hybrid genotypes simulated from observed data by calculating allele frequencies of two parental populations, then drawing gametes following a multinomial distribution in the R package “adegenet”⁶³. Second-generation (F₂) hybrids were simulated by iterating the same process but with parental populations comprising the prior F₁ genotypes. Neighbor-joining (NJ) relationships based on a Euclidian distance matrix of alternate allele counts (i.e., 0 = homozygous reference, 1 = heterozygous reference/non-reference, and 2 = homozygous non-reference) were plotted for the simulated and observed data with the ‘ape’ package v5.0⁶⁴ in R v3.4.1⁶¹ (see Supplementary Codes³⁶). For haplotype-based NJ trees, heterozygous SNPs were computationally phased over 30 iterations using BEAGLE v4.1⁶⁵. Manual verifications are provided in the Supplementary Information. We tested for admixture events in populations showing poor fit (high residuals) in tree-based phylogenies by searching non-treelike (graph) structures for higher maximum-likelihood in TreeMix v1.13⁶⁶. The program also implements F₄-statistics to test significance of the improved fit.

Demographic histories inferred from phylogenetic analyses above were further tested by simulating ten different scenarios of pairwise divergence (AM; AM with bottleneck, isolation with (constant) migration; isolation with (constant) migration and bottleneck; isolation with change in migration; SC; SC without hard admixture; SC without hard admixture with bottleneck; strict isolation; and strict isolation with bottleneck) and associated genome-wide SNP polymorphism in fastsimcoal2 v2.5.2³⁸. For each of >100,000 random parameter sets simulated per divergence model, 12 summary statistics (total number of polymorphic sites; mean total heterozygosity; number of segregating sites per population; number of private sites per population; number of pairwise differences per population; mean and SD of segregating sites over populations; and mean and SD of pairwise differences over populations) were computed in ARLSUMSTAT v3.5.2⁶⁷. Model selection and parameter estimations followed by ABCRF using 1000-tree regression forests in the “abcrf” package v1.7³⁷ in R v3.4.1⁶¹. Observed genotypes of putative F₁ and F₂ hybrids were not included in the calculation of summary statistics for modeling divergence between New World groups.

Selection analyses between predefined groups (deletion-carrying and non-deletion type isolates) were performed by assessing site-wise F_ST neutrality with BayeScan v2.1⁶⁸. We set prior odds for the neutral model to 100 and retained loci with log₁₀ q-values < −2, where false discovery rate is expected to fall below 1%. Results were then filtered for coding regions and SNP and INDEL effects predicted with SNPEff v3t⁶⁹ using the JPCM5 annotation file available at https://tritrypdb.org/common/downloads/release-33/LinfantumJPCM5/gff/data/.

Chromosomal and gene copy number analyses

To estimate chromosomal somy, we calculated mean-read-depth (m) for successive 1 kb windows using SAMtools v0.1.18⁷⁰ “depth” (default options) and then calculated a “median-of-means” (M_m) for each chromosome. We let the 40th percentile (p40) of M_m values represent expectations for the disomic state, estimating copy number for each chromosome by dividing its M_m by the sample’s p40 value and multiplying by two. Copy numbers were then visualized with the “heatmap.2” function in the “gplots” package v3.0.1.2⁷¹ in R v3.4.1⁶¹. Samples were organized in the heatmap based on UPGMA clustering of Bray–Curtis dissimilarities measured using the “vegdist” function in the “vegan” package v2.4.4⁷².

Gene copy number analyses were performed using scripts from Imamura et al.⁹. Briefly, we calculated median read-depth for each coding region (c) in the JPCM5 annotation file and then divided each c value by the median of c-values across the chromosome to obtain a normalized copy number estimate (s) for each coding region of each sample. We then averaged s-values from corresponding coding regions across samples within each of two predefined groups (deletion-carrying and non-deletion type isolates). Coding regions for which group means differed by >0.3 were selected for MWU significance tests using SciPy v1.3.1⁷³. Following Bonferroni correction (i.e., dividing the standard p-value cutoff of 0.05 by the number of coding regions submitted to MWU), we generated a heatmap of s-values at coding regions, which showed significant differences between the two groups, organizing samples by UPGMA clustering of Bray–Curtis similarities as in chromosomal somy visualization above. Coding regions with significant MWU results were also reassessed by ANCOVA using the “car” package v3.0.2⁷⁴ in R v3.4.1⁶¹ to determine whether p-values remained significant after controlling for sample geographic origin. Isolates from Teixeira et al.³³ (see Supplementary Data 1) were excluded from gene copy number analyses as these had not been made available as complete read-pairs in public sequence archives.

Monoclonal subcultures and qPCR

Single cell sorting was performed on a MoFLO ASTRIOS Cell Sorter (Beckman Coulter) at the Oswaldo Cruz Institute in Rio de Janeiro, Brazil. L. infantum isolates IOCL 2949 and IOCL 3134 entered cell sorting at 10⁶ cells/µl and individual cells were collected in a 96-well plate, each well containing 200 µl Schneider’s medium supplemented with 2% FCS. Wells were inspected five days later using an inverted microscope and liquid from those containing single parasites transferred to separate tubes of NNN. Parasites were pelleted three days later at 1,200 g for 15 min and DNA extracted with DNeasy Blood and Tissue Kit (Qiagen). Primer sequences 5′-ACGATCGGCCTCAAAACACT-3′ (forward) and 5′- GGTGAAGTCTTCGTCCGTGT-3′ (reverse) were designed to target LinJ.31.2380 (within the chr31 deletion site), and primer sequences 5′-CGAACCTTGGAGCTTCCCTT-3′ (forward) and 5′-TCAAGGTTGTGTCCGTCGAG-3′ (reverse) were designed to target LinJ.31.2330 (downstream of the chr31 deletion site). IOCL 2666 was used as a reference sample to calibrate the ΔΔCt method described by Livak and Schmittgen⁷⁵. Briefly, qPCR cycle thresholds (Ct values) for both chr31 sequence targets were determined for the samples of interest (IOCL 2949 and 3134, and their monoclonal subcultures) and for IOCL 2666. Ct values for the LinJ.31.2330 target were assumed to be equivalent between the sample of interest and the reference in the case of equal quantities of input DNA. Deviations from the 1 : 1 ratio for the LinJ.31.2330 target were used to normalize Ct ratios for the LinJ.31.2380 target between the sample of interest and the reference. The normalized ratios were considered to represent a fold change estimate of gene dose within the deletion site relative to that within downstream sequence. The qPCR reaction used 0.2 nM primer input and 1× SYBR Green Master Mix with 40 amplification cycles and an annealing temperature of 62 °C. Three experiments were performed per sample, each in technical triplicate. The same fold change estimation protocol was performed in follow-up analysis of monoclonal subcultures 2949 B2 and 2949 G1 using the parental culture IOCL 2949 as the reference.

Ecto-3’-nucleotidase and ecto-ATPase activity measurement

Ecto-3′-nucleotidase activity was quantified by measuring inorganic phosphate (Pi) release during adenosine 3’-monophosphate (3’-AMP) hydrolysis as in Freitas-Mesquita et al.²⁸. Briefly, L. infantum promastigotes (10⁷ cells/ml) were incubated at 25 °C for 1 h in 0.5 ml reaction mixture containing 16.0 mM NaCl, 5.4 mM KCl, 5.5 mM d-glucose, 50.0 mM HEPES (pH 7.4), and 3.0 mM 3’-AMP. Reactions were terminated by adding 1.0 ml ice-cold 25% charcoal in 0.1 M HCl and centrifuged at 1500 × g for 15 min to remove nonhydrolyzed 3’-AMP. Equal volumes of supernatant and Fiske & Subbarow reagent (0.1 ml each) were mixed to affect the (phosphate-dependent) reduction of ammonium molybdate to phosphomolybdate and absorbance at 660 nm in samples and _Pi standards measured after 30 min to derive sample Pi. Ecto-ATPase activity was measured with the same protocol except replacing 3’-AMP with 1.0 mM adenosine 5’-triphosphate and 1.0 mM MgCl₂. Experiments were performed in technical triplicates using IOCL 2664, 2666, 2972, 3598, and 3634, and monoclonal subcultures 2949 B2 and 3134 B1.

Statistics and reproducibility

Statistical analyses of the data, sample sizes, number of replicates, and general information on the reproducibility of experiments are depicted at each specific description within the “Methods” section.

Reporting summary

Further information on research design is available in the Nature Research Reporting Summary linked to this article.

Data availability

New sequence data generated by this study is available at Sequence Read Archive (SRA) BioProject PRJNA658892 (BioSamples SAMN15892565 – SAMN15892623). All other relevant data are available from the corresponding author on reasonable request.

Code availability

Codes can be accessed at the public repository Zenodo (http://zenodo.org) under the https://doi.org/10.5281/zenodo.42761887³⁶.

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Acknowledgements

This study was supported by Inova Fiocruz/VPPCB Fundação Oswaldo Cruz and MCTIC/CNPq No 28/2018–Universal, processo 425347/2018-4 (M.C.B.); Division of Microbiology and Infectious Diseases, the National Institute of Allergy and Infectious Diseases and the National Institutes of Health (DMID/NIADID/NIH grants AI077896-01 and AI105749-01A1 to P.S.), and the Scottish Universities Life Sciences Alliance, The Wellcome Trust; CNPq Grant number: 401134/2014-8, CAPES Grant number: 0012917, FAPERJ Grant number: e-26/201. 300 2014 (J.R.M.-F.); ERD Funds, project CePaViP (16_019/0000759) (P.V.); Seeding grant from the Institut Pasteur International Department to the LeiSHield Consortium (G.S.F.); Coordenação de Aperfeiçoamento de Pessoal de Nível Superior–Brasil (CAPES)–Finance Code 001; CNPq-Researcher Fellow (302622/2017-9) Faperj–CNE-E26-202.569/2019 and Apoio às Instituições Sediadas no estado do Rio de Janeiro–E-26/010.101083/2018; PASTEUR–FIOCRUZ–USP PROGRAM (2018), Programa PRINT FIOCRUZ-CAPES (E.C.). We thank Mrs. Thaize Chometon and Dr. Alvaro Luiz Bertho of Flow Cytometry Sorting Core Facility of Oswaldo Cruz Institute, FIOCRUZ, Rio de Janeiro, Brazil, for Flow Cytometry Cell Sorting; and Mrs Caroline Batista of Coleção de Leishmania do Instituto Oswaldo Cruz (CLIOC), Plataforma de PCR em Tempo Real RPT09A (Fiocruz).

Author information

These authors contributed equally: Philipp Schwabl, Mariana C. Boité.

Authors and Affiliations

School of Life Sciences, Institute of Biodiversity, Animal Health and Comparative Medicine, University of Glasgow, G12 8QQ, Glasgow, UK
Philipp Schwabl, Arne Jacobs & Martin Llewellyn
Laboratório de Pesquisa em Leishmaniose, Instituto Oswaldo Cruz, FIOCRUZ, 21040-365, Rio de Janeiro, Brazil
Mariana C. Boité, Fernanda N. Morgado, Renato Porrozzi & Elisa Cupolillo
Institut Pasteur-Bioinformatics and Biostatistics Hub-C3BI, USR 3756 IP CNRS, 75015, Paris, France
Giovanni Bussotti
Department of Parasites and Insect Vectors, Institut Pasteur, INSERM U1201, Unité de Parasitology moléculaire et Signalisation, 75015, Paris, France
Giovanni Bussotti & Gerald F. Späth
Department of Cell and Molecular Biology, Science for Life Laboratory, Karolinska Institutet, Biomedicum 9C, 171 77, Stockholm, Sweden
Bjorn Andersson
Laboratório de Biologia Molecular e Doenças Endêmicas, Instituto Oswaldo Cruz, Fiocruz, 21040-365, Rio de Janeiro, RJ, Brazil
Otacilio Moreira
Instituto de Bioquímica Médica Leopoldo de Meis (IBqM), Universidade Federal do Rio de Janeiro (UFRJ), 21941-590, Rio de Janeiro, RJ, Brazil
Anita L. Freitas-Mesquita & Jose Roberto Meyer-Fernandes
Laboratório de Biologia Molecular de Parasitas e Vetores, Instituto Oswaldo Cruz, 21040-365, Rio de Janeiro, Brazil
Erich L. Telleria & Yara Traub-Csekö
Faculty of Science, Department of Parasitology, Charles University, 128 44, Prague, Czech Republic
Erich L. Telleria, Slavica Vaselek, Tereza Leštinová & Petr Volf

Authors

Philipp Schwabl
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Mariana C. Boité
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Giovanni Bussotti
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Arne Jacobs
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Bjorn Andersson
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Otacilio Moreira
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Anita L. Freitas-Mesquita
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Jose Roberto Meyer-Fernandes
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Erich L. Telleria
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Yara Traub-Csekö
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Slavica Vaselek
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Tereza Leštinová
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Petr Volf
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Fernanda N. Morgado
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Renato Porrozzi
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Martin Llewellyn
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Gerald F. Späth
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Elisa Cupolillo
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Contributions

P.S. and M.C.B. share co-first authorship and wrote the original draft and final version. M.C.B. and P.S. designed and coordinated the analysis. P.S. analyzed the genomic data. G.B. performed detection of the deleted locus and gene copy number variation analyses. P.S. and A.J. performed demographic simulation modeling. B.A., E.L.T., P.V., Y.T.-C., S.V., T.L., F.N.M., and R.P. performed preliminary assays and were scientific partners within the main project that substantiated the paper. O.M. contributed to the qPCR protocol. A.L.F.-M. and J.R.M.-F. developed and performed enzymatic activity assays. M.L., G.F.S., and E.C. were principal scientific coordinators and performed main revisions of the data and manuscript.

Corresponding author

Correspondence to Mariana C. Boité.

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Schwabl, P., Boité, M.C., Bussotti, G. et al. Colonization and genetic diversification processes of Leishmania infantum in the Americas. Commun Biol 4, 139 (2021). https://doi.org/10.1038/s42003-021-01658-5

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Received: 11 March 2020
Accepted: 04 January 2021
Published: 29 January 2021
DOI: https://doi.org/10.1038/s42003-021-01658-5

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