Single-nucleotide polymorphism, linkage disequilibrium and geographic structure in the malaria parasite Plasmodium vivax: prospects for genome-wide association studies
- Pamela Orjuela-Sánchez1,
- Nadira D Karunaweera2,
- Mônica da Silva-Nunes1, 3,
- Natal S da Silva1,
- Kézia KG Scopel1, 4,
- Raquel M Gonçalves1,
- Chanaki Amaratunga5,
- Juliana M Sá5,
- Duong Socheat6,
- Rick M Fairhust5,
- Sharmini Gunawardena2,
- Thuraisamy Thavakodirasah7,
- Gawrie LN Galapaththy7,
- Rabindra Abeysinghe7,
- Fumihiko Kawamoto8,
- Dyann F Wirth9 and
- Marcelo U Ferreira1Email author
© Orjuela-Sánchez et al; licensee BioMed Central Ltd. 2010
Received: 20 January 2010
Accepted: 13 July 2010
Published: 13 July 2010
The ideal malaria parasite populations for initial mapping of genomic regions contributing to phenotypes such as drug resistance and virulence, through genome-wide association studies, are those with high genetic diversity, allowing for numerous informative markers, and rare meiotic recombination, allowing for strong linkage disequilibrium (LD) between markers and phenotype-determining loci. However, levels of genetic diversity and LD in field populations of the major human malaria parasite P. vivax remain little characterized.
We examined single-nucleotide polymorphisms (SNPs) and LD patterns across a 100-kb chromosome segment of P. vivax in 238 field isolates from areas of low to moderate malaria endemicity in South America and Asia, where LD tends to be more extensive than in holoendemic populations, and in two monkey-adapted strains (Salvador-I, from El Salvador, and Belem, from Brazil). We found varying levels of SNP diversity and LD across populations, with the highest diversity and strongest LD in the area of lowest malaria transmission. We found several clusters of contiguous markers with rare meiotic recombination and characterized a relatively conserved haplotype structure among populations, suggesting the existence of recombination hotspots in the genome region analyzed. Both silent and nonsynonymous SNPs revealed substantial between-population differentiation, which accounted for ~40% of the overall genetic diversity observed. Although parasites clustered according to their continental origin, we found evidence for substructure within the Brazilian population of P. vivax. We also explored between-population differentiation patterns revealed by loci putatively affected by natural selection and found marked geographic variation in frequencies of nucleotide substitutions at the pvmdr-1 locus, putatively associated with drug resistance.
These findings support the feasibility of genome-wide association studies in carefully selected populations of P. vivax, using relatively low densities of markers, but underscore the risk of false positives caused by population structure at both local and regional levels.
See commentary: http://www.biomedcentral.com/1741-7007/8/90
Plasmodium vivax, the most widespread of the four human malaria parasites, causes 132 to 391 million episodes of disease each year , with 2.6 billion people at risk of infection worldwide . Outside of Africa, P. vivax is the main cause of malaria morbidity, with enormous public health burden. The recent emergence of drug-resistant strains and severe (sometimes fatal) disease challenges the traditional view of vivax malaria as a benign infection and calls for new strategies to examine molecular mechanisms underlying drug resistance and increased virulence .
Linkage analysis of laboratory crosses and population-based genome-wide association studies are powerful approaches to map genetic loci contributing to drug resistance and virulence in malaria parasites . Experimental crosses of P. vivax are currently limited by the lack of practical methods for its long-term propagation and cloning in vitro , which are required to characterize phenotypes in the progeny . The ideal populations for allelic association studies are those with high prevalences of the phenotype of interest and relatively high levels of genetic diversity, allowing for numerous informative markers across the genome. Association studies are usually most cost-effective when low meiotic recombination rates are present in these populations, allowing for strong linkage between markers and phenotype-determining loci. The phenotype-associated allele is presumed to have emerged on a single or a few haplotype backgrounds. Crossover events during meiosis tend to randomize the initial haplotype(s) and to reduce population-level associations, known as linkage disequilibrium (LD), between flanking markers and candidate phenotype-determining loci. Therefore, to determine the feasibility of association studies we need a detailed picture of the overall diversity and LD landscape across the genome of P. vivax. However, patterns of genetic diversity and LD remain little characterized in field populations of this parasite and most nucleotide polymorphism data currently available are for antigen-coding genes . These data may not be informative of genome-wide patterns because of potential biases introduced by natural selection on particular phenotypes . Due to the lack of continuous culture in vitro, only field samples of P. vivax, which are heavily contaminated with host's DNA, are available for use in next-generation sequencing projects for large-scale characterization of new genetic markers.
Microsatellite markers have revealed clear geographic differences in levels of genetic diversity and LD in P. falciparum isolates sampled from four continents. Diversity was highest and LD lowest in populations from holoendemic Africa, while diversity was lowest and LD highest in populations from hypoendemic South America, with intermediate patterns seen in Southeast Asia. Parasite populations clustered according to their continental origins, with most variation found within locations in highly endemic areas. Nevertheless, substantial divergence was seen between subpopulations in South America . Putatively neutral microsatellite markers, sampled from across the genome , have recently been used to characterize field populations of P. vivax [10–12], suggesting that a spectrum of population structures also exists for this species. Again, South American parasite populations sampled from nearby sites are highly divergent [10, 11]. However, because the microsatellite markers analyzed map to different chromosomes, prior studies could not examine chromosome-level LD and infer recombination rates in P. vivax. In addition, microsatellites mutate at very high rates and other neutral genetic markers with different rate and mode of evolution, such as intergenic or synonymous single-nucleotide polymorphisms (SNPs), could offer a different picture . Significant differences detected with rapidly evolving markers, which may remain undetected with more conserved markers, do not necessarily translate into biologically meaningful differences among populations .
To explore the potential for future genome-wide association studies, we examined SNP diversity and LD across a 100-kb chromosome segment of P. vivax. We sampled parasites from areas of low to moderate endemicity in South America and Asia, where LD tends to be more extensive than in holoendemic populations. We show varying levels of SNP diversity and LD across populations (highest diversity and LD in the area of lowest malaria transmission, Sri Lanka), with substantial genetic differentiation among populations. Frequencies of nucleotide substitutions at pvmdr-1 gene, putatively associated with drug resistance, varied markedly across locations. Although these findings support the use of genome-wide association approaches to map genes underlying drug resistance and other traits in P. vivax, they underscore the risk of false positives if population structure, at both local and regional levels, is left uncorrected in association studies.
Results and Discussion
Chromosome-level SNP diversity
We examined chromosome-level SNP diversity and LD in 238 field isolates of P. vivax from areas of low to intermediate levels of malaria endemicity and two monkey-adapted strains, Belém and Salvador-I. The field isolates originated from three sites in the Amazon Basin of Brazil (Granada, Plácido de Castro and Porto Velho) and three sites (Pursat, Cambodia; Bao Loc, Vietnam; Tricomalee, Sri Lanka) across South and Southeast Asia (Additional file 1 Table S1). We assayed 85 SNPs across 100-kb of contiguous DNA sequence on chromosome 8. Of them, 57 (67.1%) segregated in at least one of the study locations. The number of SNPs that segregated in parasites from Brazil, Cambodia, Sri Lanka and Vietnam were 43, 35, 44 and 24, respectively. Only 13 (15.3%) segregated in all six locations; 8 segregated in Brazil alone and 14 segregated in Asia alone.
We measured SNP π, the average proportion of pairwise differences at assayed SNP loci , to compare diversity across study sites; monkey-adapted strains were not considered in this analysis. We obtained the following SNP π values (standard errors in parentheses): Granada = 0.1264 (0.0006); Plácido de Castro = 0.1298 (0.0026); Porto Velho = 0.1589 (0.0110); Brazil (three sites combined) = 0.1364 (0.0005); Cambodia = 0.1163 (0.0012); Vietnam = 0.0842 (0.0034); Sri Lanka = 0.15476 (0.0063); Asia (three sites combined) = 0.1401 (0.0010). The overall SNP π value for Brazilian populations of P. vivax is identical to the estimate obtained by Neafsey and colleagues for 11 P. falciparum isolates from this country that were assayed for 1638 SNPs across the whole genome .
Parasites were systematically sampled over 30 months (April 2004 through October 2006) in one of the study sites in Brazil, Granada [11, 16]. We hypothesized that local parasite populations gradually diversify over time as a result of migration, genetic drift, mutation and recombination. Accordingly, the proportion of pairwise SNP differences correlated positively with the temporal distance between dates of collection of pairs of isolates in Granada (r = 0.138, P < 0.001, Mantel correlation test). The correlation remained significant when only silent SNPs were considered (r = 0.146, P < 0.001), but not when only nonsynonymous sites were considered (r = 0.007, P = 0.343). The little variation at nonsynonymous SNP loci over time underscores the potential biases introduced by natural selection in studies of malaria parasite diversity. Whether or not similar temporal patterns of genetic divergence occur in other endemic areas remains to be investigated.
Linkage disequilibrium and haplotype blocks
We next examined whether the overall haplotype structure was conserved in different populations. To determine to which extent haplotype block boundaries were shared across populations, we calculated the proportions of pairs of markers assigned to the same block (i. e, non-recombining sites) and to different blocks or no block (i. e., recombining sites) in pairwise population comparisons. This analysis was limited to SNPs that were segregating in both populations analyzed (99 to 227 SNP assignments compared). Overall, the vast majority of SNP pairs had a concordant assignment, especially in comparisons involving Brazil and Cambodia (93%), Vietnam and Sri Lanka (91%), and Brazil and Sri Lanka (83%). These data are consistent with a conserved haplotype structure across P. vivax populations with varying levels of LD, as previously shown for P. falciparum . Lower proportions of concordant assignments were found, however, in comparisons between parasite populations from Vietnam and Cambodia (73%) and Brazil and Vietnam (60%). Most discrepancies were due to marker pairs that were in LD in Sri Lanka and Vietnam but not in Brazil and Cambodia. The vast majority (81-100%) of SNPs with concordant assignment between pairs of populations were silent. We conclude that haplotype block boundaries are shared by parasite populations with different geographic origins, suggesting the existence of conserved recombination hotspots in the genomic region analyzed, with clear implications for future association studies.
Population structure at local and regional levels
As previously shown for P. falciparum populations [15, 19], PCA provided evidence for substantial substructure within the Brazilian population of P. vivax. We thus analyzed separately this population and found that parasites did not cluster according to their collection site (Granada, Plácido de Castro or Porto Velho). In fact, most minor clusters in Brazil comprised samples from at least two of these locations (Additional file 5 Figure S3). We also carried a separate analysis of Asian samples to determine whether further substructuring was apparent. We were unable to differentiate between Cambodian and Vietnamese parasites, but this analysis revealed a large dispersal, with some substructuring, in the Sri Lankan population (Additional file 6 Figure S4). The heterogeneity of parasites from nearby locations in Brazil and from a single outbreak in Sri Lanka indicates that correcting for population structure may be required in future association studies in these endemic sites. Otherwise, there may be a spurious association between a phenotype of interest with varying prevalence among subpopulations (for example, from different locations within the same country) and any candidate genetic marker that display allele frequency differences across these subpopulations.
Natural selection and population differentiation
We focused on two nonsynonymous substitutions in pvmdr-1 thought to be associated with CQ resistance, Y976F and F1076L [21–23]. Double-mutant alleles accounted for all or nearly all samples from Cambodia and Vietnam, while wild-type alleles predominated in Brazil. An intermediate pattern was found in Sri Lanka (Figure 8). All but one single-mutant allele carried the F1076L change; the only allele carrying the Y976F change alone (i. e., not co-occurring with the F1076L change) came from Granada, Brazil. These findings lend further support to the hypothesis that a two-step mutational trajectory (F1076L followed by Y976F) at the pvmdr-1 locus leads to CQ resistance . If this hypothesis is correct, molecular detection of F1076L single mutants may provide an early warning about the risk of emerging CQ resistance before the drug-resistant phenotype itself can be detected in populations.
The finding of parasites with wild-type pvmdr-1 alleles that are CQ-resistant [22, 24] suggests that other polymorphisms may contribute to this phenotype. Similar to P. falciparum , in vitro susceptibility to CQ in P. vivax appears to be modulated by pvmdr-1 copy number. Gene amplification correlates with increased susceptibility to CQ and decreased susceptibility to amodiaquine, artesunate and mefloquine . Different country-specific drug policies may therefore favor parasites with increased pvmdr-1 copy number or select for Y976F alleles, further complicating geographic comparisons of allele frequencies and associated phenotypes.
Prospects for genome-wide population association studies
Here we describe long-ranging chromosome-level LD and relatively conserved haplotype blocks in P. vivax populations from areas with low to moderate levels of malaria transmission. The most favorable conditions for association studies with relatively low marker density were observed in Brazil, where parasites were reasonably diverse (SNP π values comparable to those estimated for local P. falciparum populations) and strong LD was observed at relatively short intermarker distances (~40 kb) but gradually declined with increasing physical distance between pairs of markers. In contrast, the similar levels of LD, along the whole 100-kb region analyzed, in the Asian populations may increase the probability of detecting false-positive associations between phenotype-associated loci and genetic markers located at considerable map distances. These findings, although limited to a single chromosome segment that comprises only 0.4% of the whole genome of the parasite, indicate that genome-wide association studies can represent a feasible strategy to map genetic regions associated with drug resistance, virulence and other phenotypes of interest in carefully selected P. vivax populations. Genome-wide studies with higher marker density are required to confirm these findings.
We have also observed substantial genetic differentiation among populations, at both local and regional levels. Consistent with previous studies of P. falciparum , we found significant geographic structure revealed by synonymous SNPs, which are putatively free of strong directional selection. In addition, we found large differences in the frequencies of nucleotide substitutions at the pvmdr-1 locus among populations. We note that, because of the underlying geographic structure, allele frequency differences observed among populations may be unrelated to the genetics of the particular phenotype under study, resulting in false-positive results or reduced power of association studies. Even when studies are restricted to a single continental origin, false positives may still result from major differences in the ancestry of local parasites, such as those found in Brazil. Accounting for the geographic structure is a major practical issue in future population-based studies of genetic determinants of P. vivax traits. Statistical methods have now been developed  to address this issue when ideally homogeneous (unstructured) parasite populations are not available for sampling.
We found varying levels of SNP diversity and LD across P. vivax populations, with the most favorable conditions for genome-wide association studies, relatively high diversity and strong LD that declines with increasing intermarker distance, observed in Brazil. However, we have also observed substantial genetic differentiation among populations at both local and regional levels, especially in the Brazilian population. Although these results suggest that association studies are feasible in selected P. vivax populations, they highlight the need for correcting for population structure to avoid false-positive associations.
Geographical parasite sampling
We collected venous or finger-prick blood samples from 432 patients with slide-confirmed P. vivax infection from three locations in Brazil and one location each in three Asian countries (Cambodia, Vietnam, and Sri Lanka (Figure 5). All sites in Brazil are characterized by year-round but hypoendemic malaria transmission, with P. vivax prevalence rates typically below 1% [29, 30]. The 249 samples from Brazil were collected in the rural settlement of Granada and the town of Plácido de Castro (50 km south of Granada), both in Acre State, and in the city of Porto Velho (500 km east of Granada), in Rondônia State. The samples from Granada (n = 193) were collected during prospective cohort studies between 2004 and 2006 [11, 16, 30], those from Plácido de Castro (n = 38) were collected in 2008 from patients attending the town's malaria clinic , and those from Porto Velho (n = 17) were collected from patients attending the Oswaldo Cruz Outpatient Clinic in June-July 1995 . The 70 samples from Cambodia were collected between June and December 2008 in Pursat town from individuals who became infected in the nearby forests (ClinicalTrials.gov identifier, NCT00663546). In April 2008, a cross-sectional survey of 1056 individuals living in the forest fringe of Pursat province, near the border with Thailand, estimated a P. vivax prevalence rate of 2.2% (CA and RMF, unpublished results). The 23 samples from Vietnam were collected in January-December 1995 from patients attending the outpatient clinic of the Lam Dong Provincial Hospital, in the town of Bao Loc, 150 km northwest of Ho Chi Mihn City, Lam Dong Province . Prevalence rates of P. vivax infection in the rural communities surrounding Bao Loc, on the southern highlands of Vietnam, were estimated to be around 2.5-7.5% at the time of sample collection . The 29 samples from Sri Lanka were collected during a malaria outbreak in Trincomalee, Eastern Province . Between January and August 2007, a total of 87 cases of vivax malaria were reported from Trincomalee (Anti-Malaria Campaign, Ministry of Health, Sri Lanka and TT, unpublished information). Over the past few years malaria transmission has declined steadily in Sri Lanka, from 210,039 cases of malaria in 2001 to only 196 cases country-wide in 2007 . In contrast, no drastic reduction in malaria transmission has been documented over the past decade in the other Asian sites included in this study.
DNA from field samples was extracted using standard protocols referenced in the original publications. Additional DNA samples, from monkey-adapted strains, Belém (isolated in Brazil, 1980) and Salvador-I (El Salvador, 1969), were provided by the Malaria Research and Reference Reagent Resource Center (MR4), ATCC (Manassas, United States). To obtain adequate DNA concentrations for SNP assays, parasite DNA was submitted to whole-genome amplification (WGA) prior to typing. WGA was performed on 10 ng of genomic DNA, with high-fidelity multiple displacement technology , using a REPLI-g Minikit (Qiagen, Valencia, United States) according to the manufacturer's instructions.
Single-nucleotide polymorphisms (SNPs)
We identified SNPs across chromosome 8 by aligning 100 kb of contiguous DNA sequence from five P. vivax isolates [37, 38] (GenBank accession numbers AY003872 and AY216936-AY216939). DNA sequences were derived from two isolates from Brazil (Belém strain  and a field isolate from Rondônia ), one from El Salvador (Salvador-I strain ), one from India (India VII strain ), and one from Thailand (Thai NYU strain ). SNPs were selected to fit two criteria: that they are located in nonrepetitive regions and that they are surrounded by 200 bp of upstream sequence and 200 bp of downstream sequence with no significant similarity to human sequences, as determined by BLAST search against the human genome, to prevent cross-amplification of human DNA present in the field-collected test samples. We examined a single chromosome region (spanning ~0.4% of the whole genome) because other genomic regions of P. vivax have not been systematically screened for SNPs using a worldwide parasite sample . We designed assays to 108 candidate SNPs meeting the criteria above, which were screened in 50 field-collected samples. Of them, 22 were discarded because alleles were called in less than 10% of these 50 test samples and one was discarded because of cross-amplification from human DNA. The final set comprised 85 markers across chromosome 8, with 75 silent SNPs (39 intergenic, 1 intronic, 9 located in 5' or 3' untranslated regions (UTR) and 26 synonymous nucleotide replacements in open reading frames of genes encoding annotated or hypothetical proteins) and 10 nonsynonymous SNPs (Additional file 8 Table S3).
We also examined nucleotide replacements at two loci encoding digestive-vacuole membrane proteins that are potentially involved in chloroquine (CQ) resistance in P. vivax (Additional file 7 Figure S5). Since parasites are exposed to different drug treatment regimes in each country, local adaptation may theoretically result in more geographic structure revealed by these polymorphisms than neutral markers . Although the molecular mechanisms of CQ resistance in P. vivax remain unknown, we focused on the two most likely candidate genes. We typed five nonsynonymous SNPs (L47 S, K76T, S250P, F276V, and L384F) in the pvcrt-o gene  that were recently found in field isolates of P. vivax [44, 45]. K76T mutant alleles of the P. falciparum orthologue of pvcrt-o, which encodes the protein chloroquine resistance transporter (PfCRT), confer CQ resistance to this species , but the limited data available to date fail to support associations between mutations in pvcrt-o alleles and CQ resistance in P. vivax [44, 45]. We also typed one synonymous (at codon 4065) and five nonsynonymous (N89 S, N500 D, M908L, Y976F, and F1076L) SNPs previously described at the multidrug resistance 1 gene of P. vivax (pvmdr-1) [21, 22, 24, 45], which encodes a P-glycoprotein of the family of ATP binding cassette (ABC) transporters. The Y976F mutation (TAC→TTC) has been associated with CQ resistance in Southeast Asia  and Papua New Guinea . Interestingly, the Y976F change is rarely, if ever, observed in alleles that do not carry the F1076L (TTT→CTT) change, suggesting a two-step mutation pathway leading to CQ resistance . All SNPs were genotyped, under contract, by K-Biosciences (Cambridge, UK), with an amplifluor assay [47, 48]. Primer sequences for amplifying the SNPs are provided in the additional file 9 Table S4; the annealing temperature for all primers was 60°C. Accuracy of genotyping was empirically assessed as 99.8% in blind replicate analyses of 5493 SNPs.
Estimation of allele frequencies in malaria parasite populations is complicated by the co-occurrence of multiple clones within infections. Counting all alleles identified within an infection results in overestimation of frequencies of rare alleles and underestimation of common alleles. To minimize bias, we excluded 101 infections in which > 1 allele was observed in any of the SNP loci. For the analysis of chromosome-level SNP diversity and LD patterns, we also excluded 93 infections with allele calls for < 60 markers across chromosome 8. Analysis of the pvcrt-o and pvmdr-1 loci was based on complete genotypes; infections with one or more SNPs without allele calls were excluded. The number of isolates considered for further analysis is shown in the additional file 1 Table S1.
Population-level diversity was measured with the SNP π statistic, defined as the average number of pairwise differences at assayed SNPs between all members of a population . SNP π values were also calculated separately for silent (synonymous or noncoding) and nonsynonymous SNPs, with standard errors estimated by bootstrapping, and compared with nonparametric Wilcoxon tests. To test whether average SNP π values increased with increased distance between dates of collection of sympatric isolates, we used Poptools (version 2.7.1) software  to run a Mantel matrix correlation test , with 1000 permutations, on the Granada subpopulation dataset (isolates systematically sampled between 2004 and 2006).
A key factor in the success of association studies is the level of LD observed within and across populations. We examined the evidence for LD within each country and in two subpopulations from Brazil (Granada and Plácido de Castro) with enough samples. The LD statistic r2  was calculated for all pairs of SNPs across chromosome 8, within populations, using LDA software . Statistical significance of LD was tested, at the 5% level, using χ2 tests. Correlation between the physical distance between markers and LD was assessed using the Pearson's coefficient of correlation (r). We defined chromosome 8 haplotype blocks as clusters of adjacent markers over which evidence of meiotic recombination was minimal, using the four-gamete rule . For each pair of markers, the frequencies of all four combinations of alleles were computed; blocks were built with consecutive markers where only three or less combinations were observed with a frequency ≥ 0.01. Haplotype blocks were generated with Haploview (version 4.1) software . To compare haplotype block boundaries across different populations, we examined the proportions of pairs of markers assigned to the same block (i. e, non-recombining sites) and to different blocks of no block (i. e., recombining sites) in each population. A SNP pair was considered concordant if the assignment was the same in both populations analyzed and discordant if the assignments disagreed . These comparisons were made for pairs of SNPs spaced up to 31 kb, since this is the length of the largest haplotype block found in our study populations.
We assessed population differentiation using the θ estimator  of FST statistic using FSTAT software ; 95% confidence intervals were derived by bootstrapping to determine whether values differed significantly from zero. We used principal component analysis (PCA) to determine whether isolates could be regarded as randomly chosen from a single, genetically homogeneous population or whether they were clustered, defining subpopulations . We carried out separate analysis for the whole dataset and for the populations from Brazil and Asia, using the MeV software . Because strong intermarker LD may distort PCA results , we compared clustering patterns obtained with all informative SNPs (e.g., those that segregated in the population under analysis) with the patterns obtained with a filtered SNP set, in which a single marker was selected from every haplotype block detected by Haploview (defined as above). We also employed STRUCTURE 2.2 software  to examine parasite population structure. This software uses a Bayesian clustering approach to assign isolates to K populations characterized by a set of allele frequencies at each locus. We run the program 10 times each for K values between 1 and 6. Each analysis involved 100,000 iterations, with 50,000 burn-in cycles. We used the linkage model to account for the LD among markers across the same chromosome. We computed the posterior probability for each K and show here clustering patterns associated with the strongest statistical support. Again, separate analyses were made for the whole dataset and for Brazilian and Asian samples.
The parasitized blood samples described in this paper were collected under protocols approved by the relevant ethical review committees in the respective countries. Patients or their parents or legal guardians provided written informed consent before donating samples. Ethical clearance was also obtained from the Institutional Review Board (IRB) of the University of São Paulo, Brazil; the IRB of the NIAID, USA; the National Research Ethics Committee of the Brazilian Ministry of Health; and the Cambodian National Ethics Committee for Health Research.
This research was supported by funds from the National Institutes of Health (NIH) grants RO1 AI 075416-01 to MUF and 5R03TW007966-02 to NK and DFW, the Intramural Research Program of the National Institute of Allergy and Infectious Diseases (NIAID), NIH, to RMF, the Conselho Nacional de Desenvolvimento Científico e Tecnológico (CNPq) grant 470570/2006-7 to MUF, and the Fundação de Amparo à Pesquisa do Estado de São Paulo (FAPESP) grants 05/51988-0 and 07/51199-0 to MUF. POS, NSS and MUF receive or received scholarships from CNPq and MdSN, KKGS and RMG receive or received scholarships from FAPESP. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript. We thank the patients from all field sites for their enthusiastic cooperation, the field work collaborators Rosely S. Malafronte and Adamilson Luís de Souza for their support in Brazil, Suon Seila and Sreng Sokunthea for their support in Cambodia, and H. Van Thien for his support in Vietnam, Maria José Menezes, Melissa da Silva Bastos and Michelle Cristina Brandi (University of São Paulo, Brazil) for excellent laboratory support, Apuã Paquola for help in computational analyses and Cassiano Nunes Pereira for artwork.
- Hay SI, Guerra CA, Tatem AJ, Noor AM, Snow RW: The global distribution and population at risk of malaria: past, present, and future. Lancet Infect Dis. 2004, 4: 327-336. 10.1016/S1473-3099(04)01043-6.PubMed CentralView ArticlePubMedGoogle Scholar
- Guerra CA, Snow RW, Hay SI: Mapping the global extent of malaria in 2005. Trends Parasitol. 2006, 22: 353-358. 10.1016/j.pt.2006.06.006.PubMed CentralView ArticlePubMedGoogle Scholar
- Price RN, Douglas NM, Anstey NM: New developments in Plasmodium vivax malaria: severe disease and the rise of chloroquine resistance. Curr Opin Infect Dis. 2009, 22: 430-435. 10.1097/QCO.0b013e32832f14c1.View ArticlePubMedGoogle Scholar
- Su X, Hayton K, Wellems TE: Genetic linkage and association analyses for trait mapping in Plasmodium falciparum. Nat Rev Genet. 2007, 8: 497-506. 10.1038/nrg2126.View ArticlePubMedGoogle Scholar
- Udomsangpetch R, Kaneko O, Chotivanich K, Sattabongkot J: Cultivation of Plasmodium vivax. Trends Parasitol. 2008, 24: 85-88. 10.1016/j.pt.2007.09.010.View ArticlePubMedGoogle Scholar
- Cui L, Escalante AA, Imwong M, Snounou G: The genetic diversity of Plasmodium vivax populations. Trends Parasitol. 2003, 19: 220-226. 10.1016/S1471-4922(03)00085-0.View ArticlePubMedGoogle Scholar
- Cornejo OE, Rojas A, Udhayakumar V, Lal AA: Assessing the effect of natural selection in malaria parasites. Trends Parasit. 2004, 20: 388-395. 10.1016/j.pt.2004.06.002.View ArticleGoogle Scholar
- Anderson TJC, Haubold B, Williams JT, Estrada-Franco JG, Richardson L, Mollinedo R, Bockarie M, Mokili J, Mharakurwa S, French N, Whitworth J, Velez ID, Brockman AH, Nosten F, Ferreira MU, Day KP: Microsatellite markers reveal a spectrum of population structures in the malaria parasite Plasmodium falciparum. Mol Biol Evol. 2000, 17: 1467-1482.View ArticlePubMedGoogle Scholar
- Carlton JM, Adams JH, Silva JC, Bidwell SL, Lorenzi H, Caler E, Crabtree J, Angiuoli SV, Merino EF, Amedeo P, Cheng Q, Coulson RM, Crabb BS, del Portillo HA, Essien K, Feldblyum TV, Fernandez-Becerra C, Gilson PR, Gueye AH, Guo X, Kang'a S, Kooij TW, Korsinczky M, Meyer EV, Nene V, Paulsen I, White O, Ralph SA, Ren Q, Sargeant TJ, Salzberg SL, Stoeckert CJ, Sullivan SA, Yamamoto MM, Hoffman SL, Wortman JR, Gardner MJ, Galinski MR, Barnwell JW, Fraser-Liggett CM: Comparative genomics of the neglected human malaria parasite Plasmodium vivax. Nature. 2008, 455: 757-763. 10.1038/nature07327.PubMed CentralView ArticlePubMedGoogle Scholar
- Imwong M, Nair S, Pukrittayakamee S, Sudimack D, Williams JT, Mayxay M, Newton PN, Kim JR, Nandy A, Osorio L, Carlton JM, White NJ, Day NPJ, Anderson TJ: Contrasting genetic structure in Plasmodium vivax populations from Asia and South America. Int J Parasitol. 2007, 37: 1013-1022. 10.1016/j.ijpara.2007.02.010.View ArticlePubMedGoogle Scholar
- Ferreira MU, Karunaweera ND, da Silva-Nunes M, Silva NS, Wirth DF, Hartl DL: Population structure and transmission dynamics of Plasmodium vivax in rural Amazonia. J Infect Dis. 2007, 195: 1218-1226. 10.1086/512685.View ArticlePubMedGoogle Scholar
- Karunaweera ND, Ferreira MU, Munasinghe A, Barnwell JW, Collins WE, King CL, Kawamoto F, Hartl DL, Wirth DF: Extensive microsatellite diversity in the human malaria parasite Plasmodium vivax. Gene. 2008, 410: 105-112. 10.1016/j.gene.2007.11.022.View ArticlePubMedGoogle Scholar
- Schlötterer C: The evolution of molecular markers - just a mater of fashion?. Nat Rev Genet. 2004, 5: 63-69. 10.1038/nrg1249.View ArticlePubMedGoogle Scholar
- Hedrick PW: Perspective: Highly variable loci and their interpretation in evolution and conservation. Evolution. 1999, 53: 313-318. 10.2307/2640768.View ArticleGoogle Scholar
- Neafsey DE, Schaffner SF, Volkman SK, Park D, Montgomery P, Milner DA, Lukens A, Rosen D, Daniels R, Houde N, Cortese JF, Tyndall E, Gates C, Stange-Thomann N, Sarr O, Ndiaye D, Ndir O, Mboup S, Ferreira MU, Moraes S do L, Dash AP, Chitnis CE, Wiegand RC, Hartl DL, Birren BW, Lander ES, Sabeti PC, Wirth DF: Genome-wide SNP genotyping highlights the role of natural selection in Plasmodium falciparum population divergence. Genome Biol. 2008, 9: R171-10.1186/gb-2008-9-12-r171.PubMed CentralView ArticlePubMedGoogle Scholar
- Orjuela-Sánchez P, da Silva NS, da Silva-Nunes M, Ferreira MU: Parasitemia recurrences and population dynamics of Plasmodium vivax polymorphisms in rural Amazonia. Am J Trop Med Hyg. 2009, 81: 961-968. 10.4269/ajtmh.2009.09-0337.View ArticlePubMedGoogle Scholar
- Mu J, Awadalla P, Duan J, McGee KM, Joy DA, McVean GA, Su XZ: Recombination hotspots and population structure in Plasmodium falciparum. PLoS Biol. 2005, 3: e335-10.1371/journal.pbio.0030335.PubMed CentralView ArticlePubMedGoogle Scholar
- Patterson N, Price AL, Reich D: Population structure and eigenanalysis. PLoS Genet. 2006, 2: e190-10.1371/journal.pgen.0020190.PubMed CentralView ArticlePubMedGoogle Scholar
- Machado RL, Povoa MM, Calvosa VS, Ferreira MU, Rossit AR, dos Santos EJ, Conway DJ: Genetic structure of Plasmodium falciparum populations in the Brazilian Amazon region. J Infect Dis. 2004, 190: 1547-1555. 10.1086/424601.View ArticlePubMedGoogle Scholar
- Pritchard JK, Stephens M, Donnelly P: Inference of population structure using multilocus genotype data. Genetics. 2000, 155: 945-959.PubMed CentralPubMedGoogle Scholar
- Brega S, Meslin B, de Monbrison F, Severini C, Gradoni L, Udomsangpetch R, Sutanto I, Peyron F, Picot S: Identification of the Plasmodium vivax mdr-like gene (pvmdr1) and analysis of single-nucleotide polymorphisms among isolates from different areas of endemicity. J Infect Dis. 2005, 191: 272-277. 10.1086/426830.View ArticlePubMedGoogle Scholar
- Suwanarusk R, Russell B, Chavchich M, Chalfein F, Kenangalem E, Kosaisavee V, Prasetyorini B, Piera KA, Barends M, Brockman A, Lek-Uthai U, Anstey NM, Tjitra E, Nosten F, Cheng Q, Price RN: Chloroquine resistant Plasmodium vivax: in vitro characterisation and association with molecular polymorphisms. PLoS One. 2007, 2: e1089-10.1371/journal.pone.0001089.PubMed CentralView ArticlePubMedGoogle Scholar
- Marfurt J, de Monbrison F, Brega S, Barbollat L, Müller I, Sie A, Goroti M, Reeder JC, Beck HP, Picot S, Genton B: Molecular markers of in vivo Plasmodium vivax resistance to amodiaquine plus sulfadoxine-pyrimethamine: mutations in pvdhfr and pvmdr1. J Infect Dis. 2008, 198: 409-417. 10.1086/589882.View ArticlePubMedGoogle Scholar
- Sá JM, Nomura T, Neves J, Baird JK, Wellems TE, del Portillo HA: Plasmodium vivax: allele variants of the mdr1 gene do not associate with chloroquine resistance among isolates from Brazil, Papua, and monkey-adapted strains. Exp Parasitol. 2005, 109: 256-259. 10.1016/j.exppara.2004.12.005.View ArticlePubMedGoogle Scholar
- Duraisingh MT, Refour P: Multiple drug resistance genes in malaria - from epistasis to epidemiology. Mol Microbiol. 2005, 57: 874-877. 10.1111/j.1365-2958.2005.04748.x.View ArticlePubMedGoogle Scholar
- Suwanarusk R, Chavchich M, Russell B, Jaidee A, Chalfein F, Barends M, Prasetyorini B, Kenangalem E, Piera KA, Lek-Uthai U, Anstey NM, Tjitra E, Nosten F, Cheng Q, Price RN: Amplification of pvmdr1 associated with multidrug-resistant Plasmodium vivax. J Infect Dis. 2008, 198: 1558-1564. 10.1086/592451.PubMed CentralView ArticlePubMedGoogle Scholar
- Anderson TJ, Nair S, Sudimack D, Williams JT, Mayxay M, Newton PN, Guthmann JP, Smithuis FM, Tran TH, van den Broek IV, White NJ, Nosten F: Geographical distribution of selected and putatively neutral SNPs in Southeast Asian malaria parasites. Mol Biol Evol. 2005, 22: 2362-2374. 10.1093/molbev/msi235.View ArticlePubMedGoogle Scholar
- Tian C, Gregersen PK, Seldin MF: Accounting for ancestry: population substructure and genome-wide association studies. Human Mol Genet. 2008, 17: R143-R150. 10.1093/hmg/ddn268.View ArticleGoogle Scholar
- Camargo LMA, Ferreira MU, Krieger H, Camargo EP, Pereira da Silva L: Unstable hypoendemic malaria in Rondônia (Western Brazilian Amazon): epidemic outbreaks and work-associated incidence in an agro-industrial rural settlement. Am J Trop Med Hyg. 2004, 51: 16-25.Google Scholar
- da Silva-Nunes M, Codeço CT, Malafronte RS, da Silva NS, Juncansen C, Muniz PT, Ferreira MU: Malaria on the Amazonian frontier: transmission dynamics, risk factors, spatial distribution, and prospects for control. Am J Trop Med Hyg. 2008, 79: 624-635.PubMedGoogle Scholar
- Orjuela-Sánchez P, da Silva-Nunes M, da Silva NS, Scopel KKG, Gonçalves RM, Malafronte RS, Ferreira MU: Population dynamics of genetically diverse Plasmodium falciparum lineages: community-based prospective study in rural Amazonia. Parasitology. 2009, 136: 1097-1105. 10.1017/S0031182009990539.PubMed CentralView ArticlePubMedGoogle Scholar
- da Silveira LA, Dorta ML, Kimura EAS, Katzin AM, Kawamoto F, Tanabe K, Ferreira MU: Allelic diversity and antibody recognition of Plasmodium falciparum merozoite surface protein 1 during hypoendemic malaria transmission in the Brazilian Amazon region. Infect Immun. 1999, 67: 5906-5916.PubMed CentralPubMedGoogle Scholar
- Ferreira MU, Liu Q, Zhou M, Kimura M, Kaneko O, Van Thien H, Isomura S, Tanabe K, Kawamoto F: Stable patterns of allelic diversity at the Merozoite surface protein-1 locus of Plasmodium falciparum in clinical isolates from southern Vietnam. J Eukaryot Microbiol. 1998, 45: 131-136. 10.1111/j.1550-7408.1998.tb05080.x.View ArticlePubMedGoogle Scholar
- Gunawardena S, Karunaweera ND, Ferreira MU, Phone-Kyaw M, Pollack RJ, Alifrangis M, Rajakaruna RS, Konradsen F, Amerasinghe PH, Schousboe ML, Galappaththy GNL, Abeyasinghe RR, Hartl DL, Wirth DF: Geographic structure of Plasmodium vivax: microsatellite analysis of parasite populations from Sri Lanka, Myanmar and Ethiopia. Am J Trop Med Hyg. 2010, 82: 235-242. 10.4269/ajtmh.2010.09-0588.PubMed CentralView ArticlePubMedGoogle Scholar
- Fernando SD, Abeyasinghe RR, Galappaththy GNL, Rajapaksa LC: Absence of asymptomatic malaria infections in previously high endemic areas of Sri Lanka. Am J Trop Med Hyg. 2009, 81: 763-767. 10.4269/ajtmh.2009.09-0042.View ArticlePubMedGoogle Scholar
- Dean FB, Hosono S, Fang L, Wu X, Farugi AF, Bray-Ward P, Sun Z, Zong Q, Du Y, Du J, Driscoll M, Song W, Kingsmore SF, Egholm M, Lasken RS: Comprehensive human genome amplification using multiple displacement amplification. Proc Natl Acad Sci USA. 2002, 99: 5261-5266. 10.1073/pnas.082089499.PubMed CentralView ArticlePubMedGoogle Scholar
- Tchavtchitch M, Fischer K, Huestis R, Saul A: The sequence of a 200 kb portion of a Plasmodium vivax chromosome reveals a high degree of conservation with Plasmodium falciparum chromosome 3. Mol Biochem Parasitol. 2001, 118: 211-222. 10.1016/S0166-6851(01)00380-2.View ArticlePubMedGoogle Scholar
- Feng X, Carlton JM, Joy DA, Mu J, Furuya T, Suh BB, Wang Y, Barnwell JW, Su XZ: Single-nucleotide polymorphisms and genome diversity in Plasmodium vivax. Proc Natl Acad Sci USA. 2003, 100: 8502-8507. 10.1073/pnas.1232502100.PubMed CentralView ArticlePubMedGoogle Scholar
- del Portillo HA, Longacre S, Khouri E, David PH: Primary structure of the merozoite surface antigen 1 of Plasmodium vivax reveals sequences conserved between different Plasmodium species. Proc Natl Acad Sci USA. 1991, 88: 4030-4034. 10.1073/pnas.88.9.4030.PubMed CentralView ArticlePubMedGoogle Scholar
- Camargo AA, Fischer K, Lanzer M, del Portillo HA: Construction and characterization of a Plasmodium vivax genomic library in yeast artificial chromosomes. Genomics. 1997, 42: 467-473. 10.1006/geno.1997.4758.View ArticlePubMedGoogle Scholar
- Collins WE, Contacos PG, Krotoski WA, Howard WA: Transmission of four Central American strains of Plasmodium vivax from monkey to man. J Parasitol. 1972, 58: 332-335. 10.2307/3278097.View ArticlePubMedGoogle Scholar
- Sullivan JS, Strobert E, Yang C, Morris CL, Galland GG, Richardson BB, Bounngaseng A, Kendall J, McClure H, Collins WE: Adaptation of a strain of Plasmodium vivax from India to New World monkeys, chimpanzees, and anopheline mosquitoes. J Parasitol. 2001, 87: 1398-1403.View ArticlePubMedGoogle Scholar
- Arnot DE, Stewart MJ, Barnwell JW: Antigenic diversity in Thai Plasmodium vivax circumsporozoite proteins. Mol Biochem Parasitol. 1990, 43: 147-149. 10.1016/0166-6851(90)90140-H.View ArticlePubMedGoogle Scholar
- Nomura T, Carlton JM, Baird JK, del Portillo HA, Fryauff DJ, Rathore D, Fidock DA, Su X, Collins WE, McCutchan TF, Wootton JC, Wellems TE: Evidence for different mechanisms of chloroquine resistance in 2 Plasmodium species that cause human malaria. J Infect Dis. 2001, 183: 1653-1661. 10.1086/320707.View ArticlePubMedGoogle Scholar
- Orjuela-Sánchez P, de Santana Filho FS, Machado-Lima A, Chehuan YF, Costa MR, Alecrim MG, del Portillo HA: Analysis of single-nucleotide polymorphisms in the crt-o and mdr1 genes of Plasmodium vivax among chloroquine-resistant isolates from the Brazilian Amazon region. Antimicrob Agents Chemother. 2009, 53: 3561-3564. 10.1128/AAC.00004-09.PubMed CentralView ArticlePubMedGoogle Scholar
- Fidock DA, Nomura T, Talley AK, Cooper RA, Dzekunov SM, Ferdig MT, Ursos LM, Sidhu AB, Naudé B, Deitsch KW, Su XZ, Wootton JC, Roepe PD, Wellems TE: Mutations in the P. falciparum digestive vacuole transmembrane protein PfCRT and evidence for their role in chloroquine resistance. Mol Cell. 2000, 6: 861-871. 10.1016/S1097-2765(05)00077-8.PubMed CentralView ArticlePubMedGoogle Scholar
- Nazarenko IA, Bhatnagar SK, Hohman RJ: A closed tube format for amplification and detection of DNA based on energy transfer. Nucleic Acids Res. 1997, 25: 2516-2521. 10.1093/nar/25.12.2516.PubMed CentralView ArticlePubMedGoogle Scholar
- Newton CR, Graham A, Heptinstall LE, Powell SJ, Summers C, Kalsheker N, Smith JC, Markham AF: Analysis of any point mutation in DNA. The amplification refractory mutation system (ARMS). Nucleic Acids Res. 1989, 17: 2503-2516. 10.1093/nar/17.7.2503.PubMed CentralView ArticlePubMedGoogle Scholar
- Poptools (version 2.7.1). [http://www.cse.csiro.au/poptools]
- Mantel N: The detection of disease clustering and a generalized regression approach. Cancer Res. 1967, 27: 209-220.PubMedGoogle Scholar
- Hill WG, Robertson A: Linkage disequilibrium in finite populations. Theor Appl Genet. 1968, 38: 226-231. 10.1007/BF01245622.View ArticlePubMedGoogle Scholar
- Ding K, Zhou K, He F, Shen Y: LDA - a java based linkage disequilibrium analyzer. Bioinformatics. 2003, 19: 2147-2148. 10.1093/bioinformatics/btg276.View ArticlePubMedGoogle Scholar
- Wang N, Akey JM, Zhang K, Chakraborty R, Jin L: Distribution of recombination crossovers and the origin of haplotype blocks: the interplay of population history, recombination, and mutation. Am J Hum Genet. 2002, 71: 1227-1234. 10.1086/344398.PubMed CentralView ArticlePubMedGoogle Scholar
- Barrett JC, Fry B, Maller J, Daly MJ: Haploview: analysis and visualization of LD and haplotype maps. Bioinformatics. 2005, 21: 263-265. 10.1093/bioinformatics/bth457.View ArticlePubMedGoogle Scholar
- Gabriel SB, Schaffner SF, Nguyen H, Moore JM, Roy J, Blumenstiel B, Higgins J, DeFelice M, Lochner A, Faggart M, Liu-Cordero SN, Rotimi C, Adeyemo A, Cooper R, Ward R, Lander ES, Daly MJ, Altshuler D: The structure of haplotype blocks in the human genome. Science. 2002, 296: 2225-2229. 10.1126/science.1069424.View ArticlePubMedGoogle Scholar
- Weir BS, Cockerham CC: Estimating F-statistics for the analysis of population structure. Evolution. 1984, 38: 1358-1370. 10.2307/2408641.View ArticleGoogle Scholar
- FSTAT version 22.214.171.124. [http://www2.unil.ch/popgen/softwares/fstat.htm]
- Saeed AI, Sharov V, White J, Li J, Liang W, Bhagabati N, Braisted J, Klapa M, Currier T, Thiagarajan M, Sturn A, Snuffin M, Rezantsev A, Popov D, Ryltsov A, Kostukovich E, Borisovsky I, Liu Z, Vinsavich A, Trush V, Quackenbush J: TM4: a free, open-source system for microarray data management and analysis. Biotechniques. 2003, 34: 374-378.PubMedGoogle Scholar
This article is published under license to BioMed Central Ltd. This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/2.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.