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Assessment of Plasmodium falciparum drug resistance molecular markers from the Blue Nile State, Southeast Sudan

Abstract

Background

Plasmodium falciparum malaria is a public health problem worldwide. Malaria treatment policy has faced periodic changes due to emergence of drug resistant parasites. In Sudan chloroquine has been replaced by artesunate and sulfadoxine/pyrimethamine (AS/SP) in 2005 and to artemether–lumefantrine (AL) in 2017, due to the development of drug resistance. Different molecular markers have been used to monitor the status of drug resistant P. falciparum. This study aimed to determine the frequency of malaria drug resistance molecular markers in Southeast Sudan.

Methods

The samples of this study were day zero dried blood spot samples collected from efficacy studies in the Blue Nile State from November 2015 to January 2016. A total of 130 samples were amplified and sequenced using illumina Miseq platform. The molecular markers included were Pfcrt, Pfmdr1, Pfdhfr, Pfdhps, Pfk13, exonuclease and artemisinin resistant (ART‐R) genetic background (Pfmdr2, ferroredoxine, Pfcrt and Pfarps10).

Results

Resistance markers for chloroquine were detected in 25.8% of the samples as mutant haplotype Pfcrt 72-76 CVIET and 21.7% Pfmdr1 86Y. Pfdhfr mutations were detected in codons 51, 59 and 108. The ICNI double-mutant haplotype was the most prevalent (69%). Pfdhps mutations were detected in codons 436, 437, 540, 581 and 613. The SGEGA triple-mutant haplotype was the most prevalent (43%). In Pfdhfr/Pfdhps combined mutation, quintuple mutation ICNI/SGEGA is the most frequent one (29%). Six of the seven treatment failure samples had quintuple mutation and the seventh was quadruple. This was significantly higher from the adequately responsive group (P < 0.01). Pfk13 novel mutations were found in 7 (8.8%) samples, which were not linked to artemisinin resistance. Mutations in ART‐R genetic background genes ranged from zero to 7%. Exonuclease mutation was not detected.

Conclusion

In this study, moderate resistance to chloroquine and high resistance to SP was observed. Novel mutations of Pfk13 gene not linked to treatment failure were described. There was no resistance to piperaquine the partner drug of dihydroartemisinin/piperaquine (DHA-PPQ).

Background

Malaria is a major public health problem in the World. In 2017, the World Health Organization (WHO) estimated that 219 million people got malaria with death amounting to 435,000 mainly in Africa [1]. In the Sudan, 720,879 cases were reported as confirmed malaria and 1446 were reported as deaths in 2017. Plasmodium falciparum is the main malaria parasite species responsible for 92% of all malaria cases while, Plasmodium vivax represents approximately 8% [1].

Malaria treatment policy in Sudan has been changed through decades from chloroquine for the uncomplicated cases and quinine for complicated cases to sulfadoxine/pyrimethamine (SP) antifolate drugs to other monotherapies which all failed through time until the introduction of artemisinin-based combination therapy (ACT) in 2005 [2,3,4].

Chloroquine resistance emerged worldwide as early as late fifties in Southeast Asia and South America [5]. In Sudan, chloroquine resistance started in late 1970s, and treatment failure became alarmingly high until the introduction of ACT in 2005 [4, 6, 7].

Single nucleotide polymorphisms (SNPs) in Pfcrt and Pfmdr1 genes have been correlated with chloroquine resistance for P. falciparum around the world [8, 9]. Mutations in these genes have been identified in several studies from different parts of the Sudan [7, 10, 11]. The resistant haplotypes of Pfcrt have been identified as 72–76 CVIET and Pfmdr1 responsible for chloroquine resistance as 86Y [8, 9, 12]. SP was introduced in Sudan for the treatment of malaria in early 1970s as a second-line treatment with chloroquine as the first-line of treatment [6]. SP has gained excellent reputation as a combination therapy that targets two different sites of the folate metabolism pathway [13] and, therefore, was the first combination therapy used for malaria treatment in Sudan. It continued to be used in pregnancy and when chloroquine resistance became a problem. However, malaria parasites developed resistance to this combination as well [14]. Previous researches which were done in Sudan identified the responsible resistance genes for SP. The genes of resistance were mutants of dihydrofolate reductase (dhfr 51I, 59R and 108N) and mutants of dihydropteroate synthase (dhps436A, 437G, 540E and 581G) of the pyrimethamine and sulfadoxine, respectively [14,15,16].

Artemisinin-based combination therapy became the rescue rope for malaria treatment in Sudan where it has been introduced in 2005 by using AS/SP [4]. This combination together with other control measures remarkably reduced the cases of malaria in Sudan during 10 years period [1]. Again treatment failure to this combination became a public health problem [15, 17] and the combination of artemether/lumefantrine as first-line of treatment of uncomplicated malaria and dihydroartemisinin/piperaquine (DHA-PPQ) as a second-line were introduced in March 2017 [17]. Exonuclease gene mutation (415G) has been noticed to be associated with increased tolerance of piperaquine [18].

Quinine has remained to be the first choice for severe malaria and malaria in pregnancy in Sudan. However, there are some concerns about decreased efficacy of quinine [19]. Mutations in the kelch propeller protein gene (k13) have been used as markers for delayed clearance of P. falciparum by artemisinin derivatives. Several non-synonymous mutations in the propeller domain of the gene have been reported from different parts of the world. The identified alleles so far linked to reduced clearance of the parasite have been reported earlier [20]. Parasite genetic background mutations that allow for emergence of Pfk13 mutations have been studied earlier [21], including Pfmdr2, ferroredoxine, Pfcrt and Pfarps10.

This research examined the different resistance markers for P. falciparum malaria from an area of unstable malaria transmission in southeastern Sudan. The main objective was to examine the resistance situation of all previously used drugs like chloroquine and the concurrent anti-malarial artemisinin-based combination therapy using molecular drug resistance markers.

Methods

Study area

The study was conducted in two health centres in Damazin, the Capital of the Blue Nile State, Southeastern Sudan (location 11.7855° N, 34.3421° E). Malaria transmission is seasonal unstable transmission following the rainy season which is July to October [17]. There is another minor peak during December to February winter months [22].

Study samples and DNA extraction

The samples of this study were dried blood spots (DBS) from uncomplicated P. falciparum malaria patients taken at day zero. Samples were part of efficacy studies for AS/SP (n = 63) and DHA-PPQ (n = 67) performed in the Blue Nile state between November 2015 and January 2016, Sudan [17]. The total number of samples was 130 (123 were from the adequately responsive patients and 7 with late parasitological drug failure (LPF) belonging to AS/SP group). Among the group of samples for Pfk13 gene sequencing, 28 were excluded because they were reported earlier [23]. The samples were collected after obtaining informed written consent from patients or the guardians of minor patients. The study received ethical clearance from the Federal Ministry of Health, Sudan.

DNA was extracted from 130 samples using QIAmp DNA Mini Kit (QIAGEN Inc., Germany) following the manufacturer’s instructions. DNA was eluted in 50 µl and stored at − 20 °C for use in the PCR assays.

Plasmodium species confirmation

Plasmodium falciparum was identified by microscopic examination of Giemsa-stained slides. Furthermore, the presence of other Plasmodium species were checked by sequencing of two conserved regions of the Plasmodium parasite mitochondrial genome [24]. This procedure was done to confirm that the samples were only P. falciparum.

Complexity of infection (COI)

Estimation of COI from SNP genotyping data was performed using the programs COIL [25] and Real MCOIL [26]. Both programs used the SNP barcode of 101 bi-allelic unlinked SNPs genotyped by amplicon sequencing (below). The COI is expressed as an integer, which is the estimated number of individual parasites within the sample.

Amplicon sequencing

Amplicon sequencing of parasite DNA samples was performed at the Wellcome Sanger Institute, UK for genotyping of drug resistance markers (Pfcrt, Pfmdr1, Pfdhfr, PfdhPfs, exonuclease, Pfk13 and artemisinin resistance (ART-R) genetic background, Pfarps10, ferredoxin, Pfcrt, Pfmdr2). Parasite genetic barcodes, and specification of the markers will appear in a manuscript in preparation by Wellcome Sanger Institute. In brief, targets for genotyping were identified and multiplex PCR primers were designed using a modified version of the mPrimer software. Primers were designed to amplify products between 190 and 250 bp and were combined into 3 pools. Before targeted amplification by PCR, a selective whole-genome amplification (sWGA) was done on extracted genomic DNA to increase the concentration of parasite DNA [27]. A two-step protocol was used to first amplify the target regions of the parasite genome, followed by a second PCR to incorporate sequencing and multiplexing adapters. PCR products were size selected and pooled into a single volume, and batched samples were sequenced in a single Illumina MiSeq lane. Samples reads were de-plexed using the multiplexing adapters and individual CRAM files were aligned to a modified amplicon Pf3D7 reference genome. Genotyping was done using bcf tools as well as custom scripts to filter and translate genotypes into drug resistance haplotypes [28]. Sequences were deposited in the public repository European Nucleotide Archive (ENA) with accession numbers provided as Additional file 1.

Data analysis

Allele and genotype data were entered into SPSS software v. 20 and frequencies were calculated. A correlations between treatment response and SP genotypes was calculated. Chi2 test was used to calculate the significance.

Results

Out of the 130 samples different numbers were successfully sequenced for the different genes.

Complexity of infection (COI)

All samples were confirmed to be only P. falciparum parasites. Complexity of infection (COI) was detected in 39 (32%) isolates, where 34 (28%) contained 2 parasite clones per sample and 5 (4%) contained 3 clones per sample.

Molecular markers for drug resistance

Genotyping of chloroquine resistance gene (Pfcrt) showed 31 (25.8%) mutant haplotypes at positions 72–76 (CVIET) (Table 1). Other mutations of Pfcrt are also shown (Table 1).

Table 1 Prevalence of Pfcrt haplotypes and alleles in P. falciparum isolates from Southeastern Sudan

N86Y mutation of Pfmdr1 was detected in 25 (21.7%) samples, while Pfmdr1 Y184F was seen in 89.5% of the samples (Table 2).

Table 2 Prevalence of Pfmdr1, Pfdhfr, Pfdhps, Pfk13, ART‐R genetic background alleles in P. falciparum isolates from Southeastern Sudan

Table 2 also shows mutations of Pfdhfr N51I which was detected in 107 (89.9%) samples, Pfdhfr S108N was seen in 116 (97.4%) samples. Alleles of Pfdhps are shown in Table 2 as well, where A437G was detected in 86 (83%) samples and 79 (76%) samples were K540E. There were no mutations detected in exonuclease E415G allele. Pfdhfr genotypes are shown in Table 3 where double mutations (ICNI) were seen in 69% of the samples, while triple mutations were seen in 21% (IRNI).

Table 3 Frequency of genotypes of Pfdhfr and Pfdhps among the AS/SP and DAPPQ groups P. falciparum isolates from Southeastern Sudan

Concerning Pfdhps (Table 3), triple mutations (SGEGA) showed the highest frequency (43.2%). All samples that showed mutation in codon A581 were mutant in codon K540E and A437G and samples that were mutated in codon K540E were also mutant in A437G.

Combination of Pfdhfr and Pfdhps mutations as seen in AS/SP and DHA-PPQ groups are shown in Table 3. The highest combined mutation was the quintuple mutation (ICNI + SGEGA) was 29.8% followed by the quadruple mutation (ICNI + SGEAA) (22.1%). Quintuple mutation was detected in 6 of the seven AS/SP drug failure isolates while the last one harboured quadruple mutation. A correlation between the adequately responsive group and the late parasitological failure group has shown that there is a significant association of the quintuple mutation with the failure group (P < 0.01).

Pfk13 showed novel non‐synonymous mutations in 5 samples F375S, K378R, D389N, E433D, N594K and 2 samples showed synonymous mutations K430K, P443P (Table 2).

No mutations were detected in Pfcrt (C72S, H97Q), Pfmdr1 (S1034C, N1042D, F1226), Pfdhfr (A16V, I164L), (ART‐R genetic background) Pfarps10 (V127M, D128Y\H), Pfmdr2 T484I.

Discussion

This is a study of molecular markers for drug resistance genes of P. falciparum malaria from the Blue Nile State in Sudan. In this study, complexity of infection was observed in 32% of the samples indicating high transmission [29]. Different mutations of Pfcrt indicating resistance have been reported in this study with total of 25.8%. However, this percentage is low compared to other areas in the country where Pfcrt mutations ranging from 63 to 100% were reported [7, 11, 16, 30, 31]. Chloroquine resistance mutations is not reversible. However, when chloroquine pressure is removed sensitive strains dominate [32, 33] so the low percentage may indicate this phenomenon. This percentage of resistance is still high for reinstitution of chloroquine which requires resistance level not exceeding 10% [34].

Mutation of Pfmdr1 N86Y is also a marker for chloroquine resistance (21.7%) is consistent with that of Pfcrt. Other reports in Sudan have shown higher levels of this mutation [7, 30, 31]. The allele Y184F showed high percentage of 89.5%, which favours the use of the first-line treatment AL as this mutation increases susceptibility of the parasite to lumefantrine [35, 36].

Reported mutations in Pfmdr1 at positions 1034, 1042 and 1226 affect several anti-malarial drugs such as mefloquine, chloroquine, quinine, and halofantrine [36, 37]. There are no mutations in these alleles associated with resistance to these drugs in this study.

Resistance to amodiaquine is linked with the same mutation linked to chloroquine resistance Pfmdr1 at positions 86 and 1246 [38, 39]. This needs more verification with in vivo studies for use of amodiaquine as a prophylactic drug.

DHFR and DHPS are the enzymes that metabolize antifolate drugs and mutations in their genes have been reported to cause treatment failure with antifolates pyrimethamine and sulfadoxine, respectively [40]. In this study, multiple mutations of Pfdhfr and Pfdhps are reported (Table 3). Mutant genotype combinations are mostly linked to increasing resistance from double to quintuple mutations [41]. In this study, quadruple and quintuple mutations represent 68%, hextuple mutations are also described in this study forming nearly 10%. The quintuple mutation (ICNI/SGEGA) is strongly linked with the treatment failure group. This finding indicates high level of resistance of SP. Earlier reports in Sudan have shown that multiple mutations were highly prevalent in eastern Sudan [7, 14]. Failure of combination therapy AS/SP in Sudan was ascribed to failure of the partner drug SP [23] and that combination was replaced by AL as the first-line of treatment [17]. This high resistance of SP also means that it cannot be used intermittently for the protection of pregnant women in highly endemic areas in Sudan.

Exonuclease gene mutation is one of the markers for resistance to piperaquine [18] and is reported to be zero in this study. The other markers were not studied. The choice of DHA–PPQ as second line of treatment [17] is well supported by this evidence. PPQ enjoys the fact that it has never been used as a mono-therapy for malaria treatment [42, 43].

Artemisinin-based combination therapy has revolutionized malaria treatment. Mutations associated with delayed clearance of parasites have been reported from Southeast Asia posing a challenge to the rest of the world. Close monitoring of mutations in the propeller protein k13 gene of P. falciparum parasite is required [20]. This study reports 5 non-synonymous and 2 synonymous random mutations among adequately responsive patients to ACT. There was a single non-synonymous mutation from a subset of the same group of patients reported earlier by Abdel Hamid et al. [23]. All these mutations were not linked with treatment failure. Other random mutations not linked to treatment failure from different parts of Africa were reported [44]. A recent report of molecular markers of resistance from different parts of Sudan not including the Blue Nile State, has indicated the absence of Pfk13 mutation [16]. However, reports from Uganda and Equatorial Guinea have indicated the presence of resistant Pfk13 gene mutations in these countries (Pfk13 A675V and C580Y respectively) [45, 46]. Another single mutation in the Pfk13 gene which might be associated with reduced clearance of parasites was reported from Ethiopia [47]. These reports are alarming for the malaria control programmes in Africa.

Mutant alleles of artemisinin resistance genetic background are shown in very low percentages in this study. Mutations of these genes are not directly linked to artemisinin resistance. However, they collectively lead to Pfk13 gene mutation that can lead to failure of treatment [21].

Conclusion

This study has shown that there is moderate resistance to chloroquine, very high resistance to SP and novel mutations in Pfk13 gene not linked to artemisinin resistance. Absence of exonuclease mutations supports absence of PPQ resistance. This study supports the malaria treatment protocol currently used in Sudan.

Availability of data and materials

The datasets used in this study are available as Additional file 2.

References

  1. 1.

    WHO. World malaria report 2018. Geneva: World Health Organization; 2018. https://www.who.int/malaria/publications/world-malaria-report-2018/en/. Accessed 31 Aug 2019.

  2. 2.

    Adam I, A-Elbasit IE, Idris SM, Malik EM, Elbashir MI. A comparison of the efficacy of artesunate plus sulfadoxine–pyrimethamine with that of sulfadoxine–pyrimethamine alone, in the treatment of uncomplicated, Plasmodium falciparum malaria in eastern Sudan. Ann Trop Med Parasitol. 2005;99:449–55.

  3. 3.

    Elamin SB, Malik EM, Abdelgadir T, Khamiss AH, Mohammed MM, Ahmed ES, et al. Artesunate plus sulfadoxine–pyrimethamine for treatment of uncomplicated Plasmodium falciparum malaria in Sudan. Malar J. 2005;4:41.

  4. 4.

    Mohamed AO, Eltaib EH, Ahmed OA, Elamin SB, Malik EM. The efficacies of artesunate–sulfadoxine–pyrimethamine and artemether–lumefantrine in the treatment of uncomplicated, Plasmodium falciparum malaria, in an area of low transmission in central Sudan. Ann Trop Med Parasitol. 2006;100:5–10.

  5. 5.

    Awasthi G, Das A. Genetics of chloroquine-resistant malaria: a haplotypic view. Mem Inst Oswaldo Cruz. 2013;108:947–61.

  6. 6.

    Adeel AA. Drug-resistant malaria in Sudan: a review of evidence and scenarios for the future. Sudan J Paediatr. 2012;12:8.

  7. 7.

    Menegon M, Talha AA, Severini C, Elbushra SM, Mohamedani AA, Malik EM, et al. Frequency distribution of antimalarial drug resistance alleles among Plasmodium falciparum isolates from Gezira State, central Sudan, and Gedarif State, eastern Sudan. Am J Trop Med Hyg. 2010;83:250–7.

  8. 8.

    Wellems TE, Plowe CV. Chloroquine-resistant malaria. J Infect Dis. 2001;184:770–6.

  9. 9.

    Foote SJ, Kyle DE, Martin RK, Oduola AM, Forsyth KK, Kemp DJ, et al. Several alleles of the multidrug-resistance gene are closely linked to chloroquine resistance in Plasmodium falciparum. Nature. 1990;345:255–8.

  10. 10.

    A-Elbasit IE, Elbashir MI, Khalil IF, Alifrangis M, Giha HA. The efficacy of sulfadoxine–pyrimethamine alone and in combination with chloroquine for malaria treatment in rural Eastern Sudan: the interrelation between resistance, age and gametocytogenesis. Trop Med Int Health. 2006;11:604–12.

  11. 11.

    Mohammed WS, Yasin K, Mahgoub NS, Hamid MM. Cross sectional study to determine chloroquine resistance among Plasmodium falciparum clinical isolates from Khartoum, Sudan. F1000Research. 2018;7:208.

  12. 12.

    Fidock DA, Nomura T, Talley AK, Cooper RA, Dzekunov SM, Ferdig MT, et al. Mutations in the P. falciparum digestive vacuole transmembrane protein PfCRT and evidence for their role in chloroquine resistance. Mol Cell. 2000;6:861–71.

  13. 13.

    Nzila A. The past, present and future of antifolates in the treatment of Plasmodium falciparum infection. J Antimicrob Chemother. 2006;57:1043–54.

  14. 14.

    Al-Saai S, Kheir A, Abdel-Muhsin AM, Al-Ghazali A, Nwakanma D, Swedberg G, et al. Distinct haplotypes of dhfr and dhps among Plasmodium falciparum isolates in an area of high level of sulfadoxine–pyrimethamine (SP) resistance in eastern Sudan. Infect Genet Evol. 2009;9:778–83.

  15. 15.

    Adeel AA, Elnour FA, Elmardi KA, Abd-Elmajid MB, Elhelo MM, Ali MS, et al. High efficacy of artemether–lumefantrine and declining efficacy of artesunate + sulfadoxine–pyrimethamine against Plasmodium falciparum in Sudan (2010–2015): evidence from in vivo and molecular marker studies. Malar J. 2016;15:285.

  16. 16.

    Bakhiet AM, Abdelraheem MH, Kheir A, Omer S, Gismelseed L, Abdel-Muhsin AM, et al. Evolution of Plasmodium falciparum drug resistance genes following artemisinin combination therapy in Sudan. Trans R Soc Trop Med Hyg. 2019;113:693–700.

  17. 17.

    Mohamed AO, Hamid MM, Mohamed OS, Elkando NS, Suliman A, Adam MA, et al. Efficacies of DHA–PPQ and AS/SP in patients with uncomplicated Plasmodium falciparum malaria in an area of an unstable seasonal transmission in Sudan. Malar J. 2017;16:163.

  18. 18.

    Amato R, Lim P, Miotto O, Amaratunga C, Dek D, Pearson RD, et al. Genetic markers associated with dihydroartemisinin–piperaquine failure in Plasmodium falciparum malaria in Cambodia: a genotype–phenotype association study. Lancet Infect Dis. 2017;17:164–73.

  19. 19.

    Saito M, Gilder ME, Nosten F, McGready R, Guérin PJ. Systematic literature review and meta-analysis of the efficacy of artemisinin-based and quinine-based treatments for uncomplicated falciparum malaria in pregnancy: methodological challenges. Malar J. 2017;16:488.

  20. 20.

    Ariey F, Witkowski B, Amaratunga C, Beghain J, Langlois AC, Khim N, et al. A molecular marker of artemisinin-resistant Plasmodium falciparum malaria. Nature. 2014;505:50–5.

  21. 21.

    Miotto O, Amato R, Ashley EA, MacInnis B, Almagro-Garcia J, Amaratunga C, et al. Genetic architecture of artemisinin-resistant Plasmodium falciparum. Nat Genet. 2015;47:226.

  22. 22.

    Federal Ministry of Health. Sudan malaria treatment protocol 2017. https://www.humanitarianresponse.info/sites/www.humanitarianresponse.info/files/2019/07/Sudan-Malaria-Treatment-Protocol_2017.pdf.

  23. 23.

    Abdel Hamid MM, Abdallah WM, Hussien M, Mohammed NM, Malik EM, Ahmed ME, et al. Absence of K13 gene mutations among artesunate/sulfadoxine–pyrimethamine treatment failures of Sudanese Plasmodium falciparum isolates from Damazin, southeast Sudan. Trans R Soc Trop Med Hyg. 2019;113:428–30.

  24. 24.

    Lalremruata A, Jeyaraj S, Engleitner T, Joanny F, Lang A, Bélard S, et al. Species and genotype diversity of Plasmodium in malaria patients from Gabon analysed by next generation sequencing. Malar J. 2017;16:398.

  25. 25.

    Galinsky K, Valim C, Salmier A, De Thoisy B, Musset L, Legrand E, et al. COIL: a methodology for evaluating malarial complexity of infection using likelihood from single nucleotide polymorphism data. Malar J. 2015;14:4.

  26. 26.

    Chang HH, Worby CJ, Yeka A, Nankabirwa J, Kamya MR, Staedke SG, et al. THE REAL McCOIL: a method for the concurrent estimation of the complexity of infection and SNP allele frequency for malaria parasites. PLoS Comput Biol. 2017;13:e1005348.

  27. 27.

    Oyola SO, Ariani CV, Hamilton WL, Kekre M, Amenga-Etego LN, Ghansah A, et al. Whole genome sequencing of Plasmodium falciparum from dried blood spots using selective whole genome amplification. Malar J. 2016;15:597.

  28. 28.

    Pearson RD, Amato R, Kwiatkowski DP, MalariaGEN Plasmodium falciparum Community Project. An open dataset of Plasmodium falciparum genome variation in 7,000 worldwide samples. bioRxiv. 2019;824730.

  29. 29.

    Arnot D. Unstable malaria in Sudan: the influence of the dry season: clone multiplicity of Plasmodium falciparum infections in individuals exposed to variable levels of disease transmission. Trans R Soc Trop Med Hyg. 1998;92:580–5.

  30. 30.

    Anderson TJ, Nair S, Jacobzone C, Zavai A, Balkan S. Molecular assessment of drug resistance in Plasmodium falciparum from Bahr El Gazal province, Sudan. Trop Med Int Health. 2003;8:1068–73.

  31. 31.

    Tagelsir N, Ibrahim Z, Medani A, Salih O, Hamad A, Giha H, et al. High frequency of Plasmodium falciparum PfCRT K76T and PfpghN86Y in patients clearing infection after chloroquine treatment in the Sudan. Acta Trop. 2006;97:19–25.

  32. 32.

    Frosch AE, Laufer MK, Mathanga DP, Takala-Harrison S, Skarbinski J, Claassen CW, et al. Return of widespread chloroquine-sensitive Plasmodium falciparum to Malawi. J Infect Dis. 2014;210:1110–4.

  33. 33.

    Lu F, Zhang M, Culleton RL, Xu S, Tang J, Zhou H, et al. Return of chloroquine sensitivity to Africa? Surveillance of African Plasmodium falciparum chloroquine resistance through malaria imported to China. Parasit Vectors. 2017;10:355.

  34. 34.

    WHO. Global report on antimalarial drug efficacy and drug resistance: 2000–2010. Geneva: World Health Organization; 2010. https://apps.who.int/iris/bitstream/handle/10665/44449/9789241500470_eng.pdf. Accessed 31 Aug 2019.

  35. 35.

    Malmberg M, Ferreira PE, Tarning J, Ursing J, Ngasala B, Björkman A, et al. Plasmodium falciparum drug resistance phenotype as assessed by patient antimalarial drug levels and its association with pfmdr1 polymorphisms. J Infect Dis. 2013;207:842–7.

  36. 36.

    Veiga MI, Dhingra SK, Henrich PP, Straimer J, Gnädig N, Uhlemann AC, et al. Globally prevalent PfMDR1 mutations modulate Plasmodium falciparum susceptibility to artemisinin-based combination therapies. Nat Commun. 2016;7:11553.

  37. 37.

    Reed MB, Saliba KJ, Caruana SR, Kirk K, Cowman AF. Pgh1 modulates sensitivity and resistance to multiple antimalarials in Plasmodium falciparum. Nature. 2000;403:906–9.

  38. 38.

    Nsobya SL, Kiggundu M, Nanyunja S, Joloba M, Greenhouse B, Rosenthal PJ. In vitro sensitivities of Plasmodium falciparum to different antimalarial drugs in Uganda. Antimicrob Agents Chemother. 2010;54:1200–6.

  39. 39.

    Venkatesan M, Gadalla NB, Stepniewska K, Dahal P, Nsanzabana C, Moriera C, et al. Polymorphisms in Plasmodium falciparum chloroquine resistance transporter and multidrug resistance 1 genes: parasite risk factors that affect treatment outcomes for P. falciparum malaria after artemether-lumefantrine and artesunate–amodiaquine. Am J Trop Med Hyg. 2014;91:833–43.

  40. 40.

    Gregson A, Plowe CV. Mechanisms of resistance of malaria parasites to antifolates. Pharmacol Rev. 2005;57:117–45.

  41. 41.

    Naidoo I, Roper C. Mapping ‘partially resistant’, ‘fully resistant’, and ‘super resistant’ malaria. Trends Parasitol. 2013;29:505–15.

  42. 42.

    Basco LK, Ringwald P. In vitro activities of piperaquine and other 4-aminoquinolines against clinical isolates of Plasmodium falciparum in Cameroon. Antimicrob Agents Chemother. 2003;47:1391–4.

  43. 43.

    Davis TM, Karunajeewa HA, Ilett KF. Artemisinin-based combination therapies for uncomplicated malaria. Med J Aust. 2005;182:181–5.

  44. 44.

    Taylor SM, Parobek CM, DeConti DK, Kayentao K, Coulibaly SO, Greenwood BM, et al. Absence of putative artemisinin resistance mutations among Plasmodium falciparum in sub-Saharan Africa: a molecular epidemiologic study. J Infect Dis. 2015;211:680–8.

  45. 45.

    Ikeda M, Kaneko M, Tachibana SI, Balikagala B, Sakurai-Yatsushiro M, Yatsushiro S, et al. Artemisinin-resistant Plasmodium falciparum with high survival rates, Uganda, 2014–2016. Emerg Infect Dis. 2018;24:718.

  46. 46.

    Lu F, Culleton R, Zhang M, Ramaprasad A, von Seidlein L, Zhou H, et al. Emergence of indigenous artemisinin-resistant Plasmodium falciparum in Africa. N Engl J Med. 2017;376:991–3.

  47. 47.

    Bayih AG, Getnet G, Alemu A, Getie S, Mohon AN, Pillai DR. A unique Plasmodium falciparum K13 gene mutation in northwest Ethiopia. Am J Trop Med Hyg. 2016;94:132–5.

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Acknowledgements

This publication used samples from Blue Nile state, Sudan collected by the authors; and the sequencing data were generated by the Malaria GEN Spot Malaria Project as described online [malariagen.net] https://www.malariagen.net/projects/spotmalaria [malariagen.net] pending citable publication; the project is coordinated by the MalariaGEN Resource Centre with funding from Wellcome (098051, 090770). We would like to thank the staff of Wellcome Sanger Institute specially Dr Sonia Morgado Goncalves, Kimberly Johnson and Mozam Ali.

Funding

This research received partial funding from the Federal Ministry of Health and Al Neelain University, Sudan.

Author information

AOM, EMM, and MMAH: conception and design of project, AOM, AS, NSE: sample collection and preservation. MH and HA: conducted the lab work. MH, MHA, AOM, and MMAH: analysis and interpretation of data. AOM, AH, AM and MMAH: drafted and corrected the manuscript. All authors read and approved the final manuscript.

Correspondence to Abdelrahim O. Mohamed or Muzamil Mahdi Abdel Hamid.

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Ethics approval and consent to participate

The study was approved by the Federal Ministry of Health, Sudan. Written informed consent was obtained from each individual who was willing to participate in the study. All experimental procedures were performed following the IRB approved protocol.

Consent for publication

Not applicable.

Competing interests

The authors declare that they have no competing interests.

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Mohamed, A.O., Hussien, M., Mohamed, A. et al. Assessment of Plasmodium falciparum drug resistance molecular markers from the Blue Nile State, Southeast Sudan. Malar J 19, 78 (2020). https://doi.org/10.1186/s12936-020-03165-0

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Keywords

  • P. falciparum
  • Molecular marker
  • Sudan
  • Pfcrt
  • Pfmdr1
  • Pfdhfr
  • Pfdhps
  • Pfk13
  • Exonuclease

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