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Simultaneous detection of Plasmodium vivax dhfr, dhps, mdr1 and crt-o resistance-associated mutations in the Colombian Amazonian region

  • Juan Ricardo Cubides1,
  • Paola Andrea Camargo-Ayala1,
  • Carlos Hernando Niño1,
  • Diego Garzón-Ospina1, 2,
  • Anggie Ortega-Ortegón1,
  • Estefany Ospina-Cantillo1,
  • María Fernanda Orduz-Durán1,
  • Manuel Elkin Patarroyo1, 3 and
  • Manuel Alfonso Patarroyo1, 2Email author
Malaria Journal201817:130

https://doi.org/10.1186/s12936-018-2286-5

Received: 23 October 2017

Accepted: 21 March 2018

Published: 27 March 2018

Abstract

Background

Malaria continues being a public health problem worldwide. Plasmodium vivax is the species causing the largest number of cases of malaria in Asia and South America. Due to the lack of a completely effective anti-malarial vaccine, controlling this disease has been based on transmission vector management, rapid diagnosis and suitable treatment. However, parasite resistance to anti-malarial drugs has become a major yet-to-be-overcome challenge. This study was thus aimed at determining pvmdr1, pvdhfr, pvdhps and pvcrt-o gene mutations and haplotypes from field samples obtained from an endemic area in the Colombian Amazonian region.

Methods

Fifty samples of parasite DNA infected by a single P. vivax strain from symptomatic patients from the Amazonas department in Colombia were analysed by PCR and the pvdhfr, pvdhps, pvmdr1 and pvcrt-o genes were sequenced. Diversity estimators were calculated from the sequences and the haplotypes circulating in the Colombian Amazonian region were obtained.

Conclusion

pvdhfr, pvdhps, pvmdr1 and pvcrt-o genes in the Colombian Amazonian region are characterized by low genetic diversity. Some resistance-associated mutations were found circulating in this population. New variants are also being reported. A selective sweep signal was located in pvdhfr and pvmdr1 genes, suggesting that these mutations (or some of them) could be providing an adaptive advantage.

Keywords

Malaria Plasmodium vivax Antimalarial drug resistanceAmazonian regionColombia pvdhfr pvdhps pvmdr1 and pvcrt-o

Background

Malaria continues being a worldwide problem; it is a vector-born disease (VBD) transmitted by parasites from the genus Plasmodium [1]. About 40% of the world’s population (around three billion people) are currently at risk of suffering from this disease. Malaria causes more than 200 million clinical cases and about 400,000 deaths each year [1]. The climatic and geographical conditions in Colombia enable the transmission of this infection [2], and both Plasmodium vivax and Plasmodium falciparum are prevalent.

There are three large Plasmodium endemic foci in Colombia: Urabá–lower Cauca–southern Córdoba, the Pacific coast and the Orinoquía–Amazonía transition region; such regions favour malarial incidence and dispersion due to their environmental conditions and social, political and cultural variables [1, 3]. The main difficulty in controlling P. vivax lies in the need for treating both blood stage and latent liver forms (hypnozoites), the latter causing relapses months or years after initial infection [4].

First-line treatment for uncomplicated P. vivax malaria in Colombia is currently based on a combination of chloroquine (CQ) for eliminating blood stages (schizonts) and primaquine (PQ) for liver stages (hypnozoites) [5]. In other countries, treatment is also based on the use of sulfadoxine–pyrimethamine (SP) [6]. Although these drugs remain effective overall, cases of resistance have been recorded during the last few years, making this one of the greatest problems in controlling and eliminating malaria. The first report of CQ-resistant P. vivax strains in Latin-America was published in 1989 (including Colombia and Brazil) [7]; however, resistance targets have not been clearly established. Regarding P. falciparum, parasite genes associated with resistance to anti-malarial drugs have been established with greater certainty. Simple, double or quadruple mutations in different genes enable the parasite to cope with anti-malarial drugs. Mutations in pfcrt, pfmdr1, pfdhfr and pfdhps genes have arisen/been fixed in several parasite populations and, since they confer drug resistance, this facilitates their dispersion.

There may be a clear association between pfcrt, pfmdr1, pfdhfr and pfdhps allele variants and drug resistance, but such association is not clear regarding P. vivax. Nevertheless, genetic studies of P. vivax drug susceptibility in different parts of the world [813] have identified point mutations in orthologous genes (pvcrt-o, pvmdr1, pvdhfr and pvdhps) to those associated with resistance in P. falciparum, providing potential markers of resistance to P. vivax anti-malarial drugs [1416]. Molecular biology techniques provide a valid alternative for identifying resistance-associated mutations regarding anti-malarial drug therapy in different populations and could therefore be used as a tool for surveillance of P. vivax drug resistance.

Very few studies have been made in Colombia regarding the search for polymorphisms in these genes. A 2015 evaluation in Colombia’s Córdoba department [17] stated that the P. vivax population was more genetically diverse than it had been thought. However, some genome regions had low diversity due to a selective sweep associated with the PvDHPS A383G allele [17] which, in turn, has been associated with sulfadoxine resistance [18]. The region surrounding PvDHFR did not have a loss of genetic diversity, as with PvDHPS; nevertheless, two alleles (S58R and S117N) [17] were reported to be associated with SP resistance [11]. Five non-synonymous mutations have been reported in pvdmr1; the mutation triggering change Y976F has been associated with reduced sensitivity to CQ [19]. However, other studies have not found susceptibility to CQ, despite Y976F being present. This phenotype has been reported in the north of Colombia [17], although such marker’s role in resistance has not been completely clarified [16]. The Colombian Amazon region is another focus for malaria as the people inhabiting the area live far away from city centres (i.e. lacking basic services and sanitation), their insecticide use is infrequent and access to healthcare centres is limited, making them more vulnerable to acquiring the disease and putting them at greater risk of not receiving timely treatment. Bewilderingly, there have been no studies regarding the presence of genotypes associated with resistance to the anti-malarial drugs used against P. vivax in this region. This study was thus aimed at evaluating the genetic diversity of pvmdr1, pvdhfr, pvdhps and pvcrt-o fragments in P. vivax parasites from Colombia’s Amazonian region, thereby providing significant information for the molecular surveillance of drug-resistant P. vivax.

Methods

Study areas

The samples used in this study were taken from several settlements in the municipalities of Leticia and Puerto Nariño in Colombia’s Amazonas department after volunteers had signed informed consent forms. These municipalities are located along the Banks of the Amazonas and Loretoyacu rivers on the Amazonian frontier with Peru and Brazil. All sample taking-related procedures and managing patients were approved by the Universidad del Rosario’s School of Medicine and Health Sciences’ Research Ethics Committee (resolution CEI-ABN026-000161).

Extracting parasite DNA and confirming single Plasmodium vivax infection

Genomic DNA samples were extracted from FTA card-stored blood of Plasmodium spp. infected patients using a Pure Link Genomic DNA mini kit (Invitrogen), following the manufacturer’s specifications. The samples were eluted in 50 µL final volume of buffer containing 10 mM Tris–HCl, at pH 9.0 and 0.1 mM EDTA. P. vivax infection was confirmed, as described previously [20].

Samples positive for P. vivax were explored for selecting those which were only infected by a single strain. A pvmsp3α fragment was amplified and sequenced, as previously described [21, 22]. The resulting electropherograms were assembled and revised using CLC Genomics Workbench (v.3) [23]. Samples having overlapping peaks in electropherograms were discarded; only samples whose electropherograms showed single peaks were involved in analysis.

Amplifying, purifying and sequencing pvmdr1, pvdhfr, pvdhps and pvcrt-o

Fragments from each gene associated with resistance were amplified using 50 samples confirmed as being infected by just one P. vivax strain, using previously described primers (Table 1) and thermal profiles pvmdr1 [19], pvdhfr [24], pvdhps [25] and pvcrt-o [26]. PCR products were then purified using a Wizard SV Gel and PCR Clean-up System kit (Promega), following the manufacturer’s indications. Purified products were then bidirectionally sequenced using the ABI 3730 XL system (Macrogen, Seoul, South Korea).
Table 1

Primers used for sequencing msp3-α, pvmdr1, pvdhfr, pvdhps and pvcrt-o

Gene of interest

Primers used for sequencing

Size (bp)

Primer

Sequence

msp3-α: [21]

P1

5′-CAGCAGACACCATTTAAGG-3′

2194

P2

5′-CCGTTTGTTGATTAGTTGC-3′

N1

5′-GACCAGTGTCATACCATTAACC-3′

1895

N2

5′-ATACTGGTTCTTCGTCTTCAGG-3′

pvcrt-o: [26]

F

5′-AAGAGCCGTCTAGCCATCC-3′

1186

R

5′-AGTTTCCCTCTACACCCG-3′

pvdhps: [25]

PvDHPS-D

5′-GGTTTATTTGTCGATCCTGTG-3′

1301

PvDHPS-B

5′-GAGATTACCCTAAGGTTGATGTATC-3′

pvmdr1: [19]

14-F

5′-CCCTCTACATCTTAGTCATCG-3′

932

14-R

5′-TGGTCTGGACAAGTATCTAAAA

976-F

5′-GGATAGTCATGCCCCAGGATTG-3′

604

976-R

5′-CATCAACTTCCCGGCGTAGC-3′

pvdhfr: [24]

PvDA

5′-ACCGCACCAGTTGATTCCTAC-3′

1018

PvDB

5′-TGTTAAAGCTGAAGTACACGAG-3′

PvDF

5′-ATGGAGGACCTTTCAGATGT-3′

785

PvDR

5′-AACGCATTGCAGTTCTCCGA-3′

Analysing pvmdr1, pvdhfr, pvdhps and pvcrt sequences

The resulting electropherograms were corrected and assembled using CLC Genomics Workbench (v.3) [23] for obtaining a consensus sequence per sample and per gene. Consensus sequences were compared to the respective Salvador I (Sal-I) strain reference sequences having an antimalarial drug sensitivity profile (PlasmoDB access numbers: PVX_080100 for pvmdr1, PVX_089950 for pvdhfr, PVX_123230 for pvdhps and PVX_087980.1 for pvcrt-o). The respective amino acid (aa) sequence was inferred for each nucleotide sequence obtained from the Colombian Amazonian region, as well as Sal-I strain sequences and their orthologues in Plasmodium cynomolgi (a species phylogenetically-related to P. vivax; PlasmoDB access numbers: PCYB_101870 for pvmdr1, PCYB_053150 for pvdhfr, PCYB_143740 for pvdhps and PCYB_011610-t26_1 for pvcrt). The Muscle algorithm was then used for aligning them; this aa alignment was then taken as reference for inferring nucleotide alignment, using PAL2NAL software [27].

Genetic diversity and the effect of natural selection

DnaSP software (v.5.10.00) was used for calculating several genetic diversity estimators from pvmdr1, pvdhfr, pvdhps and pvcrt nucleotide alignment, such as the segregating sites number, the haplotypes number, nucleotide and haplotype diversity and nucleotide polymorphism [28]. The modified Nei–Gojobori method [29] was used with MEGA software (v.7) [30] for evaluating selective pressure by calculating synonymous (dS) and non-synonymous (dN) substitution rates. Tajima [31], Fu and Li [32], and Fay and Wu estimators [33] were used for evaluating deviations from the neutral model of molecular evolution.

Results

pvmdr1, pvdhfr, pvdhps and pvcrt-o polymorphism

Fifty samples infected by a single population of P. vivax were used for evaluating the polymorphism of several fragments from genes associated with resistance. Five polymorphisms were observed for pvdmr1 (Fig. 1), four being non-synonymous and just one being synonymous; this gene’s nucleotide diversity (π) was 0.0013 and no substitution producing a change in aa Y976F (one of the first chemoresistance molecular marker candidates) [8] was found in samples from the Colombian Amazonian region. However, 62% of samples evaluated had T958M polymorphism and variant D994E was observed in 54% of the samples (Table 2 and Fig. 2). F983L and L1022 polymorphisms, encoding singleton sites, were observed as well as phenylalanine being replaced by leucine in position 1070 (Table 2 and Fig. 2). Concerning DNA, the 5 polymorphisms produced 5 different haplotypes (Fig. 1), haplotype 3 occurring most frequently (53%), followed by haplotype 2 (39%). The synonymous substitution of a cytosine for a thymine was found in position 3064, located in position 1 of the codon triplet (2% frequency).
Figure 1
Fig. 1

DNA haplotypes found in the Colombian Amazon region. a Aligning pvmdr1 gene non-conserved residues. b Aligning pvdhps non-conserved residues. c Aligning pvdhfr non-conserved residues. Dots indicate conserved residues. Nucleotide positions are indicated according to the P. vivax Sal-I strain numbering (PlasmoDB accession PVX_089950 for pvmdr1, PVX_123230 for pvdhps and PVX_080100 for pvdhfr)

Table 2

P. vivax resistance-associated molecular marker prevalence

Codon

% of mutations

Mutation

Protein change

mdr1

 2873

62

ACG>ATG

T958M

 2949

38

TTT>TTA

F983L

 2982

54

TTC>CTC

D994E

 3064

2

CTA>TTA

L1022

 3208

2

TTC>CTC

F1070L

dhfr

 45

12.2

GCA>GCG

A15

 57

12.2

GTC>GTT

V19

 149

2.44

AAC>ATC

N50I

 171

2.44

TTC>TTG

F57L

 173

31.7

AGC>AAG

S58K

 174

97.5

AGC>AGG/AGA

S58R

 207

82.9

TAT>TAC

Y69

 350

97.6

AGC>AAC

S117N

 517

4.88

ATT>CTT

I173L

 524

4.88

GGA>GAA

G175E

dhps

 1145

8.3

TCC>TGC

S382C

 1148

41.6

GCC>GGC

A383G

 1385

2

AAG>AGAG

K462R

Figure 2
Fig. 2

Amino acid haplotypes found in the Colombian Amazon region. a PvMDR1 alignment. b PvDHPS alignment. c PvDHFR alignment. Dots indicate conserved residues. Amino acid positions are indicated according to P. vivax Sal-I strain numbering (PlasmoDB accession PVX_089950 for PvMDR1, PVX_123230 for PvDHPS and PVX_080100 for PvDHFR)

pvdhfr fragments could only be obtained in 41 of the 50 samples; 10 polymorphisms were observed (Fig. 1), with a π = 0.0037 and 10 different haplotypes (Fig. 1). Some polymorphisms observed coincided with those reported in other populations; 97.6% of the samples evaluated here had S117N substitutions, Y69 had 82.9% prevalence and S58K 31.7%, whilst the S58R polymorphism occurred in 97.5% of the samples (Table 2 and Fig. 2). Regarding DNA haplotypes, haplotype 9 occurred with the greatest frequency (32%) compared to haplotypes 1, 2 and 3 (Fig. 1). Synonymous substitutions were observed in changes A15 and V19 (12.2%).

A pvdhps fragment was obtained in 48 of the 50 samples; three polymorphisms and 4 haplotypes were observed in this gene (Fig. 1), the π was 0.0011, all polymorphisms being non-synonymous. The A383G substitution occurred in 41.6% of samples, whilst polymorphism A382C was only observed in 8.3% of them (Table 2 and Fig. 2). Haplotype 1 occurred in 55% of samples compared to haplotype 4 in 33% of them (Fig. 1). Finally, there was no polymorphism in pvcrt-o, showing that all isolates from the Colombian Amazonian region analysed here had 100% identity with the Sal-1 reference strain.

Natural selection in genes associated with resistance

Several tests based on the neutral molecular evolution model were performed to determine whether fragments from genes associated with resistance were under some selective pressure; dN–dS ratio values had no significant values (Table 3). Tajima, and Fu and Li tests revealed gave negative values; however, they were not significant. Nevertheless, Fay and Wu H estimator gave significant P. vivax pvdhfr and pvdmr1 negative values for the population in the south of the Colombian Amazonian region (Table 3).
Table 3

Genetic diversity estimators and neutral tests

n

Gene

Sites

Ss

H

Hd

θ

π

dN–dS

Fay and Wu

H

41

dhfr

558

10

10

0.84

0.0040

0.0037

− 0.006*

− 3.64

48

dhps

648

3

4

0.56

0.0010

0.0011

0.002

0.32

50

mdr1

522

5

5

0.55

0.0021

0.0013

0.001

− 1.50

33

crt-o

375 

0

0

0.00

0.0000

0.0000

n total sequences used for analysis, Sites total sites used to rule out gap sites, Ss amount of segregating sites, H amount of haplotypes, Hd haplotype diversity, θ nucleotide polymorphism per site, π nucleotide diversity per site, d N d S ratio of non-synonymous to synonymous nucleotide polymorphism

p = 0.038

p < 0.01

Discussion

Plasmodium vivax genetic diversity is an important challenge which must be overcome in attempts to control this infection [34]. Such diversity could enable the parasite to evade host immune responses and confer an adaptive advantage for resisting anti-malarial drugs [35].

The transmission of Plasmodium species in Colombia varies according to each geographical area, enabling several of them to cohabit in the same area. Plasmodium falciparum/P. vivax multiple infections could go unnoticed during diagnosis [6, 20] and thus the attending doctor cannot prescribe suitable treatment for patients; in turn, this could exercise selective pressure on parasite populations. Choosing the right treatment is thus crucial for preventing the appearance and propagation of resistance [1]. The samples analysed here came from a tri-border region involving Colombia, Peru and Brazil. First-line treatment for uncomplicated P. vivax infections is similar for the three countries, where a combination of CQ and PQ is used [5, 36, 37]. Previous studies have reported polymorphisms associated with resistance to anti-malarial drugs in South and Central America [7, 10].

Polymorphisms have been found in Central America in pvmdr1 and pvdhfr which may be related to a loss of P. vivax susceptibility to anti-malarial drugs [10]. Nevertheless, no in vitro susceptibility studies have been reported so far to support such association. Cases of CQ therapeutic failure concerning treating P. vivax malaria have been documented in South America. Around 12% of therapeutic failure due to CQ-resistant parasites and 6.4% due to mefloquine-resistant parasites have been reported in Brazil’s Amazon region [38]. Taking into account that the sampling site in this study was near the tri-border area, the interchange of parasite strains carrying resistance mutations was likely and such haplotypes would become dispersed throughout neighbouring endemic areas. Although, P. vivax CQ resistance mechanisms have not been fully elucidated, they could involve various genetic loci. Plasmodium falciparum pfcrt-o and pfmdr1 variants have been identified as being associated with CQ resistance; these genes’ orthologues in P. vivax have thus been evaluated for determining whether they might be associated with resistance [39].

Previous studies have found that PvMDR1 Y976F and F1076L variants seem to have been associated with CQ resistance [40]. One such polymorphism (variant Y976F) has been found to occur frequently in the east of the Brazilian Amazonian region [7]. Nevertheless, the role of Y976F in CQ resistance is not yet clear [16]. Neither Y976F nor F1076L have been observed in the Colombian Amazonian region’s population. Even so, other PvMDR1 polymorphisms were found in this population which have not been reported previously and could thus be substitutions in the strains circulating in the Colombian Amazon region. This suggested that haplotypes segregating in the Brazilian Amazonian region are different to those segregating in the Colombian equivalent and, therefore, gene flow between the Brazilian and Colombian Amazon regions seems to be limited or restricted. Further analysis is required to corroborate whether additional substitutions found in Colombia are related to clinical-resistance phenotypes.

Various mutations in pvdhfr and pvdhps have been associated with resistance to SP [41]. SP in Colombia and Brazil is not currently used as first-line treatment for P. vivax infection, even though having been included in Colombian Ministry of Health guidelines towards the end of the 1990s [5]. However, SP is used as the drug of choice for treating P. falciparum in Colombia [37, 42] and in northern Perú [43]. Diagnosis in the three countries is by thick smear; however, several reports have highlighted under-recording of cases by this method and a high rate of coinfection on the Colombia–Brazil–Perú frontier [20, 44]. This diagnostic technique’s inherent limitations and the large amount of misdiagnosed co-infections could affect selecting the proper treatment, thereby creating selective pressure on the parasite, leading to the fixing of SP resistance in P. vivax strains [45], even if SP may not be being used for treating vivax malaria. Polymorphisms found in PvDHFR (F57L/I, S58R, T61M and S117T/N) usually appear in patients having therapeutic failure [46]. Parasites having double substitutions (F57L–S117N), triple substitutions (5F7L–5S8R–S117N) and quadruple substitutions (F57L–S58R–T61M–S117T) have thus been associated with SP resistance [10, 47, 48]. Ten different polymorphisms were found in the Amazon region evaluated in this work; double substitutions (S58R–S117N) were observed in 59% of them. It has been proposed that the current use of SP in Colombia has exercised selective pressure on both P. falciparum and P. vivax [49]; validation follow-up is thus recommended to observe its efficacy as treatment. A triple mutation haplotype was observed (S58R–S117N–I173L) in 17% of samples; however, it is not clear whether this haplotype could be associated with resistance.

PvDHPS polymorphisms in aa 382, 383, 512, 553 and 585 (homologues for P. falciparum positions 436, 437, 540, 581 and 613, respectively) [26] seem to be involved in resistance to sulfadoxine. A high S382C mutation prevalence in chloroquine and mefloquine-resistant parasites has been observed in Brazil’s Amazon region [38, 50]. A383G substitution prevalence was 41.6%, the most prevalent in this study, unlike S382C and K462R mutations; this could have been related to changes in aa position 382 and 383 which are frequent in regions having high SP use [51]. In addition to the aforementioned polymorphisms, new pvdhfr and pvdhps variants and haplotypes were found in P. vivax strains from the Colombian Amazonian region.

pvcrt is an orthologue of pfcrt whose association with resistance to CQ is controversial [52]; CRT has shown no contribution whatsoever to resistance to chloroquine regarding P. vivax, even though sensitive or resistant P. vivax parasites cause substitution 76K [53]. Concerning the Colombian Amazonian region this gene fragment was seen to be highly conserved, having 100% identity with the P. vivax Sal-1 strain which is susceptible to anti-malarial drugs.

Selective sweep could be taking place, fixing advantageous variants

Point mutations or determined haplotypes in P. falciparum that alter dhfr, dhps, mdr1 and crt-o protein products, enable the parasite to resist several drugs. Such mutations are usually fixed rapidly in populations due to a selective advantage causing DNA regions containing such genes to have low genetic diversity (such effect is known as selective sweep). The pvdhfr, pvdhps, pvmdr1 and pvcrt-o fragments analysed in the population from Colombia’s southern Amazon region had low genetic diversity; such polymorphisms seemed to be neutral according to Tajima, Fu and Li and dN–dS tests. However, the Fay and Wu H estimator gave significant pvdhfr and pvmdr1 values, suggesting a selective sweep. A candidate-resistant gene (pvdhps) having this pattern has been recorded previously in Colombia’s Córdoba department [17] according to information regarding the complete genome of P. vivax clinical isolates. Some mutations found in these P. vivax genes could have been fixed by conferring an advantage, in turn fixing neutral variants and thus reducing genetic diversity. As Fay and Wu tests gave statistically significant values, the southern Colombian Amazonian region’s parasite population might be under selective pressure, probably exerted by anti-malarial drugs; a selective sweep might thereby be fixing mutations enabling the appearance of resistant phenotypes. However, genes involved in selective sweep were different between Tierra Alta and the Colombian Amazonian region, probably due to differential treatment in these populations or populations in Colombia being structured with low gene flow between them, as seen in previous studies [5456]. Further analysis is required to assess the selective sweep hypothesis regarding these genes in the Colombian Amazonian region.

Conclusions

Even though studies in malaria-endemic regions have focused on the search for alternatives for improving the available treatment against malaria, the impact of these strategies on the evolution of P. vivax populations must be evaluated, due to the appearance and dispersion of resistance in such regions. Although, resistance is not fully understood concerning P. vivax and resistance-markers have not been clearly defined yet [16], dhfr, dhps, mdr1 and crt-o genes have mutations which (in some cases) seem to provide resistance or at least reduced susceptibility to anti-malarial drugs [57]. Even though not all four genes have confirmed roles regarding P. vivax drug susceptibility, they are potential targets for P. vivax resistance. These four genes have low genetic diversity in the Colombian Amazon region. However, some of the mutations found were associated with resistance, i.e. the F1070L mutation in PvMDR1, S117N and S58R/K in PvDHFR and A383G and A382C in PvDHPS, whilst other new variants were also found in these genes. pvmdr1 and pvdhfr fragments’ diversity pattern could be the consequence of a selective sweep, indicating that these genes’ variants might be becoming fixed in the population due to an adaptive advantage; these mutations could endow the parasite population with lower sensitivity to anti-malarial drugs. However, additional sequence analysis and in vitro assays are needed to confirm whether these variants are associated with resistance and/or therapeutic failures. The results reported here could be taken as a base tool for advising on how malaria control measures are implemented in Colombia and avoid the dispersion of haplotypes associated with resistance in this region.

Abbreviations

Pvmdr1

P. vivax multidrug resistance 1 gene

Pvdhfr

P. vivax dihydrofolate reductase

Pvdhps

P. vivax dihydropteroate synthase

Pvcrt-o

P. vivax chloroquine resistance transporter

CQ: 

chloroquine

PQ: 

primaquine

SP: 

sulfadoxine–pyrimethamine

Declarations

Authors’ contributions

JRC conceived and designed the experiments. JRC, PAC-A, CHN, AO-O, EO-C and MFO-D performed the experiments. DG-O performed the evolutionary analysis. JRC, CHN, PAC-A, DG-O, MAP analysed the data. JRC, DG-O, PAC-A, CHN, MEP, MAP wrote the paper. All authors read and approved the final manuscript.

Acknowledgements

The authors would like to thank the Amazonian region Governor’s office for providing resources through Colombia’s General Royalties System and Colombia’s Science, Technology and Innovation Fund’s (Project BPIN-266) special agreement (020) for financing this project. We would like to express our gratitude to Jason Garry for translating and revising this manuscript.

Competing interests

The authors declare that they have no competing interests.

Availability of data and materials

The DNA sequences and the data related were deposited in the GenBank database with Accession Numbers: MG100841–MG100859.

Ethics approval and consent to participate

The P. vivax-infected patients from whom parasite genomic DNA was obtained gave their informed consent after having been notified about the research’s purpose. All procedures were approved by the Fundación Instituto de Inmunología de Colombia and the Universidad del Rosario’s School of Medicine and Health Sciences’ research ethics committee (Resolution CEI-ABN026-000161).

Funding

This project was funded by the Colombian Royalties System as approved by the body overseeing the Colombian Science, Technology and Innovation Fund, Project BPIN-266, special agreement (020).

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Authors’ Affiliations

(1)
Molecular Biology and Immunology Department, Fundación Instituto de Inmunología de Colombia (FIDIC), Bogotá, Colombia
(2)
School of Medicine and Health Sciences, Universidad del Rosario, Bogotá, Colombia
(3)
School of Medicine, Universidad Nacional de Colombia, Bogotá, Colombia

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