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High prevalence of Pfcrt 76T and Pfmdr1 N86 genotypes in malaria infected patients attending health facilities in East Shewa zone, Oromia Regional State, Ethiopia

Malaria Journal volume 21, Article number: 286 (2022) Cite this article

Abstract

Background

Plasmodium falciparum resistance to series of anti-malarial drugs is a major challenge in efforts to control and/or eliminate malaria globally. In 1998, following the widespread of chloroquine (CQ) resistant P. falciparum, Ethiopia switched from CQ to sulfadoxine–pyrimethamine (SP) and subsequently in 2004 from SP to artemether–lumefantrine (AL) for the treatment of uncomplicated falciparum malaria. Data on the prevalence of CQ resistance markers after more than two decades of its removal is important to map the selection pressure behind the targets codons of interest. The present study was conducted to determine the prevalence of mutations in Pfcrt K76T and Pfmdr1 N86Y codons among malaria-infected patients from Adama, Olenchiti and Metehara sites of East Shewa zone, Oromia Regional State, Ethiopia.

Methods

Finger-prick whole blood samples were collected on 3MM Whatman ® filter papers from a total of 121 microscopically confirmed P. falciparum infected patients. Extraction of parasite DNA was done by Chelex-100 method from dried blood spot (DBS). Genomic DNA template was used to amplify Pfcrt K76T and Pfmdr1 N86Y codons by nested PCR. Nested PCR products were subjected to Artherobacter protophormiae-I (APoI) restriction enzyme digestion to determine mutations at codons 76 and 86 of Pfcrt and Pfmdr1 genes, respectively.

Results

Of 83 P. falciparum isolates successfully genotyped for Pfcrt K76T, 91.6% carried the mutant genotypes (76T). The prevalence of Pfcrt 76T was 95.7%, 92.5% and 84.5% in Adama, Metehara and Olenchiti, respectively. The prevalence of Pfcrt 76T mutations in three of the study sites showed no statistical significance difference (χ2 = 1.895; P = 0.388). On the other hand, of the 80 P. falciparum samples successfully amplified for Pfmdr1, all carried the wild-type genotypes (Pfmdr1 N86).

Conclusion

Although CQ officially has been ceased for the treatment of falciparum malaria for more than two decades in Ethiopia, greater proportions of P. falciparum clinical isolates circulating in the study areas carry the mutant 76T genotypes indicating the presence of indirect CQ pressure in the country. However, the return of Pfmdr1 N86 wild-type allele may be favoured by the use of AL for the treatment of uncomplicated falciparum malaria.

Background

Despite the reduction of malaria-related morbidity and mortality in recent years, there are 241 million estimated cases and nearly 627 thousand deaths in 2020. The World Health Organization (WHO) African Region alone contributed to 95% and 96% of the estimated global malaria cases and deaths, respectively. Children under 5 years of age are the most risk group, accounting for 77% of all malaria deaths globally in 2020. Plasmodium falciparum is the major causes of disease and deaths in this region [1].

Plasmodium falciparum developed resistance to every class of anti-malarial drugs to date [2]. Chloroquine resistance (CQR) has been associated with mutations in P. falciparum chloroquine resistance transporter (Pfcrt) gene and in P. falciparum multidrug resistance 1 (Pfmdr1) gene; however the former is a strong predictor of CQR [3, 4]. In vitro and in vivo studies indicated that substitutions of charged lysine (K) amino acid by uncharged amino acid threonine (T) at amino acid position 76 (K76T) is a primary marker of CQR [3, 4]. Other mutations at amino acid position 72, 74, 75, 97, 152, 163, 220, 271, 326, 356 and 371 have been also identified in CQR P. falciparum in different geographical regions [4, 5]. CQR strains of P. falciparum originating from CVMNK (CQ sensitive haplotype) are also characterized by CVIET (mostly in Africa) and SVMNT (Asia and South America) haplotypes spanning codons 72–76 of the Pfcrt gene [6, 7].

Five point mutations in Pfmdr1 gene at positions 754, 1049, 3598, 3622 and 4234 result in amino acid changes at codons 86 (N86Y), 184 (Y184F), 1034 (S1034C), 1042 (N1042D) and 1246 (D1246Y), respectively [8]. These mutations have been implicated in increase resistance to CQ, amodiaquine, mefloquine (MQ), quinine (QN) and halofantrine [9]. Out of these mutations N86Y appears to be the most important as it alters the transport activity of the protein and has been implicated as high resistance to CQ [10]. Meanwhile this mutation increases susceptibility to a number of anti-malarial drugs including lumefantrine (LUM), MQ and dihydroartemisinin [9]. Strong linkage disequilibrium was observed between Pfmdr1 N86Y and Pfcrt K76T alleles in CQR isolates of P. falciparum [8]. Amplification of the Pfmdr1 gene also leads to decreased drug sensitivity to QN, LUM and artemisinin [11].

In Ethiopia, CQ treatment failure for P. falciparum and P. vivax was reported in 1996 [12]. Then, due to widespread of CQ resistant P. falciparum, the country changed its treatment policy from CQ to sulfadoxine–pyrimethamine (SP) in 1998 which in turn was replaced by artemether–lumefantrine (AL) for the treatment of uncomplicated falciparum malaria in 2004; however CQ is retained and still continued to be used as a first-line treatment for vivax malaria [6, 13]. Molecular studies from Ethiopia have showed high prevalence of Pfcrt K76T mutation that ranged from 41.5 to 100% [6, 13, 14]. However, only one study has showed the return of CQ sensitive P. falciparum with 84% of Pfcrt K76 sensitive alleles [15]. On the other hand, in Ethiopia, AL pressure might result in directional selection of Pfmdr1 variants N86, 184 F and D1246 due to LUM partner drug pressure [6, 13,14,15]. Therefore, it is important to continue monitoring the prevalence of these markers (Pfcrt and Pfmdr1) that confer resistance to CQ in the hope of possible re-emergence of CQ sensitive P. falciparum as previously observed in Malawi [16]. Due to co-existence of P. falciparum and P. vivax; mixed infections of both parasites are common in Ethiopia [17] that favor the presence of indirect but sustained CQ drug pressure. Therefore, the aim of the present study was to investigate the prevalence of genotypic resistance markers for CQ (Pfcrt K76T and Pfmdr1 N86Y) in P. falciparum isolates from East Shewa zone, Oromia Regional State, Ethiopia.

Methods

Description of study sites

Cross-sectional health facility based study was conducted at Adama (8° 32′ 31″ N and 39° 16′ 33″ E), Olenchiti (8° 38′ 16″ N and 39° 24′ 19″ E) and Metehara (8° 86′ 95″ N and 39° 92′ 02″ E) health facilities of East Shewa zone, Oromia Regional State, Ethiopia. Adama the capital town of East Shewa zone is found at around 99 km from Addis Ababa, the capital city of Ethiopia. Olenchiti and Metehara towns are found to the East of Adama town at about 25 and 91 km, respectively (Fig. 1). The current study was conducted at purposively selected health facilities due to their physical accessibility to Adama malaria research and diagnostic centre to conduct membrane-feeding assay for another experiment.

Fig. 1
figure 1

Map of the study area. Arc GIS version 10.8

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The areas are characterized by low altitude (< 2000 m above sea level), heavy rainfall pattern from June to August followed by major transmission of malaria from September to December and short rains of February and March contributing for minor malaria transmission from April to May [18]. Geographical location of the study areas in Great Rift Valley, at low altitude, with rainfall pattern and average annual temperature of 16–32 °C make the areas favorable environments for breeding of Anopheles mosquitoes, of which Anopheles arabiensis is the major malaria vector [19]. Both P. falciparum and P. vivax co-exist in the area as it is common in different parts of the country.

Blood sample collections and processing

Blood samples from one hundred twenty-one microscopically confirmed P. falciparum infected patients were collected between October, 2019 and September, 2021. Inclusion criteria include patients who presented with uncomplicated falciparum malaria and history of fever onset since 24 h of clinical examination. Blood samples were collected after obtaining consents from P. falciparum infected patients or their parents or legal guardians in case of children less than 18 years of age. After consent was obtained patients sex, age and residency were recorded into log-book. Finger-prick blood samples were collected onto microscope slides and Whatman-3MM ® filter papers by experienced laboratory technologists. Filter papers were allowed to air dry in horizontal position at room temperature for at least 4 h away from dust, insects and direct sun light. Each filter paper was labelled with patient code and date of collection and kept into zip-locked plastic bags with silica gels to protect the specimens from moisture. These zip-locked plastic bags then packed in a larger plastic bags and stored in refrigerator at 2–8 °C for short period in the field and further stored in deep freezer at − 20 °C at Aklilu Lemma Institute of Pathobiology for long period until DNA analysis for molecular study.

Microscopic diagnosis and parasite counts

Microscopy diagnosis of both Giemsa-stained thick and thin blood films was conducted according to WHO protocol [20]. At each health facilities slides were read by two experienced laboratory technologists to confirm species identification for P. falciparum. In addition slides re-examinations and parasite counts were performed by two WHO certified malaria microscopists at Adama malaria research and diagnostic centre. Further, asexual stages of the parasite per micro-litre (µl) was determined by counting the number of parasites against 200 white blood cells (WBCs) on a thick blood film assuming a total of standard WBCs count of 8000/µl of blood. Density of the parasite was determined by using the following formula [21]:

$$\text{Parasite density}/ \upmu \text{l} = \frac{\text{No. of asexual parasites counted} \times 8 \times 10^3 \,\text{WBCs}/ \upmu \text{l}}{200 \text{WBCs}}$$

For comparison with Pfcrt K76T wild and mutant alleles, parasitaemia was categorized as low (< 1000 parasites/µl of blood), moderate (1000–9999 parasites/µl of blood) and high (≥ 10,000 parasites/µl of blood) [22].

Molecular analysis

DNA extraction

Plasmodium falciparum genomic DNA was extracted from dried blood spot (DBS) by Chelex extraction method as described elsewhere [19]. Extracted DNA was transferred into 0.5 ml tubes and stored at − 20 °C until further use.

Amplification of the Pfcrt gene

A fragment from Pfcrt gene encompassing 76th codon was successively amplified for 83 DNA samples. Nested polymerase chain reaction (PCR) protocol adapted and modified from the work of Mulenga et al. [23]. Briefly, in primary PCR, 20.0 µl reaction mixture consisting of 11.6 µl nuclease free water, 0.2 µl of each forward and reverse primers, 4.0 µl 5X FIREPol® Master Mix (Solis BioDyne) and 4.0 µl of DNA template was used. PCR was conducted in a thermo cycler (VWR) Schmidt, Germany. Amplification was performed under the following conditions: Hot start denaturations at 94oC for 3 min, followed by 30 cycles of 94 °C for 30 s, 56 °C for 30 s and 65 °C for 1 min and final elongation at 65 °C for 3 min. Then, the primary PCR was followed with nested PCR. Twenty microlitre reaction mixture consisting of 14.6 µl nuclease free water, 0.2 µl of each forward and reverse primers (Additional file 1), 4.0 µl 5X FIREPol Master Mix (Solis BioDyne) and 1.0 µl of DNA template was used. The nested PCR was conducted as follows: Hot start denaturation at 94 °C for 5 min, followed by 40 cycles of 94 °C for 30 s, 52 °C for 30 s and 65 °C for 1 min and lastly, final elongation at 65 °C for 3 min.

Amplification of Pfmdr1 gene

Pfmdr1 gene was amplified to identify mutation at codon N86Y according to the protocol described by Fontecha et al. [24] with certain modifications. Briefly, both primary and nested PCRs were conducted in a total reaction volume of 18.0 µl consisting of 11.4 µl ddH2O, 1.0 µl of each forward and reverse primers (Additional file 1), 3.6 µl 5X FIREPol Master Mix and 1.0 µl DNA template. In primary PCR, the target gene was amplified starting with hot start denaturation at 95 °C for 3 min, followed by 20 cycles of 95 °C for 30 s, 52 °C for 30 s and 72 °C for 1 min and lastly, final extension at 60 °C for 5 min. Nested PCR amplification was conducted beginning with hot start denaturation at 95 °C for 3 min, followed by 25 cycles of 95 °C for 30 s, 54 °C for 30 s, and 72 °C for 60 s and final extension at 72 °C for 5 min.

For both Pfcrt K76T and Pfmdr1 N86Y codons, PCR conditions were conducted along with nuclease free water (negative control) instead of parasite DNA, 3D7 (CQ sensitive) and K1 (MRA-159G, CQ resistant) clones of P. falciparum genomic DNA (positive controls). The two strains were provided by Ethiopian Public Health Institute and Aklilu Lemma Institute of Pathobiology, respectively. Five microlitre of nested PCR products were resolved in 2.0% and 2.5% agarose, type I gel (Sigma Alorich, USA) stained with ethidium bromide (EtBr) respectively, for Pfcrt K76T and Pfmdr1 N86Y codons. Electrophoresis conditions were conducted at 100 volts for 45 min in a Thermo Scientific apparatus filled with 0.5X TBE buffer solution (BIONEER Corp, Korea). Then, DNA bands were observed through ultra-violet (UV) trans-illuminator (USA). The band sizes were estimated by relating with 100 bp DNA ladder marker (Bionexus). The remaining 15 µl and 13 µl nested PCR products of Pfcrt K76T and Pfmdr1 N86Y, respectively were stored at 2–8 °C until used for genotyping by restriction fragment length polymorphism (RFLP).

Genotyping of Pfcrt K76T and Pfmdr1 N86Y codons by RFLP of PCR products

Following amplification of the two codons, genotyping by PCR-RFLP was made by digesting the fragments with APoI restriction enzyme (New England Biolabs). Nested PCR products were used without purification procedures as this will represent common situations in malaria settings [25]. Restriction digestion was conducted according to the manufacturer’s protocol. Restriction enzyme digestion was done in 20.0 µl of reaction mixture containing 12.5 µl nuclease free water, 5U ApoI restriction enzyme, 2.0 µl NEBuffer r3.1 and 5 µl nested PCR products. Known positive controls (Pf3D7, wild-type and K1, mutant type) and uncut DNA samples were included in the reactions. The enzyme cuts Pfcrt 76K and Pfmdr1 N86 but not Pfcrt 76T and Pfmdr1 86Y alleles. Cleaved PCR products (bands) of Pfcrt K76T and Pfmdr1 N86Y codons were then visualized with UV trans-illuminator after electrophoresis using 2.0% and 2.5% agarose gel, respectively.

Amplifications of merozoite surface protein-1 (msp-1) gene

For the subsets of samples that amplifications of Pfcrt and Pfmdr1 genes were not successful, msp1 gene amplification was made. Thirty-eight samples which were microscopically detected as P. falciparum were not amplified particularly for Pfcrt K76T codon. In order to verify the presence of intact genes and quality of DNA for those samples, nested PCR targeting msp-1 of polymorphic region (block-2) was performed as described elsewhere [19].

Statistical analysis

Data were first entered into Microsoft Office Excel ® 2007 (Microsoft Corporation). Comparisons of prevalence of 76T allele and parasite densities across study sites and associations of K76 and 76T alleles with parasite density were performed using Pearson’s Chi-square test of Statistical Package for Social Science (SPSS) (IBM Inc., Chicago, IL, USA) version 26. Fisher exact test was used to test correlation between Pfcrt 76T alleles and age groups. Statistical significance was set at a P-value < 0.05.

Results

Socio-demographic and parasitological characteristics of study population

Eighty- three and eighty samples were successfully analysed for Pfcrt K76T and Pfmdr1 N86Y codons, respectively. The patients were aged between 1 and 68 years and the mean age was 23 ± 14.7 years (interquartile range: 13–30). Seventy-percent of the patients were adults older than 15 years of age. Among patients involved in the study 65% and 35% were males and females, respectively. Parasite density ranged from 79 to 157,538 asexual stages/µl of blood, with a parasitaemia geometric mean of 5366 or median 6579 asexual parasites/µl (Table 1).

Table 1 Socio-demographic and parasitological characteristics of the patients recruited in the study (n = 83)
Full size table

Average parasites density at Adama, Olenchiti and Metehara sites were 10781.84/µl, 9870.95/µl and 15089.22/µl, respectively; however, the difference is not statistically significant (χ2 = 162.75; P = 0.469) (Fig. 2).

Fig. 2
figure 2

Mean parasites density versus study sites

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Number of P. falciparum clinical samples collected per study site

A total of 121 samples (31 from Adama, 22 from Olenchiti and 68 from Metehara) which were collected from health centres confirmed for P. falciparum isolates were allowed for PCR. Eighty three (68.6%) samples were successfully amplified for Pfcrt K76T codon; 38 samples were not amplified for the codon. From those samples amplified for Pfcrt K76T, 80 were found successfully amplified for Pfmdr1 N86Y codon.

Prevalence of Pfcrt K76T and Pfmdr1 N86Ycodons per study site

Digestion of the nested PCR products carrying K76 alleles of Pfcrt gene with APoI restriction produced 100 and 45 bps, but remained uncut when 76T mutant allele presents (hence a single band of 145 bp) while digestion of N86 allele of Pfmdr1 gene with the same restriction enzyme resulted in 239 and 179 bp fragments (denoting wild-type) (Additional file 2).

Among 83 P. falciparum isolates successfully genotyped for Pfcrt K76T, 91.6% and 8.4% mutant- type allele (76T) and wild-type alleles (K76), respectively were detected (Fig. 3). Accordingly, high prevalence of 76T mutant allele was detected at Adama (95.7%), Olenchiti (84.2%) and Metehara (92.7%) study sites with no statistical significant difference (χ2 = 1.895; P = 0.388). On the other hand low prevalence of wild-type K76 alleles were detected at each health centres (Table 2). Most of them were detected in P. falciparum isolates with moderate parasitaemia level (1000–99,999 parasites/µl). Isolates with 76T allele had a higher mean parasite density of 15,420 parasites/µl while those with K76 allele had a mean parasite density of 7623.14 parasites/µl. However, no significant association was observed between parasite density and allele type (χ2 = 76.53; P = 0.620). Eighty nested PCR products of N86Y codons were analysed by restriction enzyme digestion produced N86 (100%) wild-type allele; no 86Y mutant type-allele was detected (Fig. 3).

Fig. 3
figure 3

Prevalence of wild and mutant alleles for Pfcrt K76T and Pfmdr1 N86Y codons among P. falciparum isolates from Adama, Olenchiti and Metehara study sites

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Table 2 Prevalence of Pfcrt wild-type and mutant alleles at Adama, Olenchiti and Metehara study areas
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Prevalence of Pfcrt 76T allele by gender

Out of 83 isolates successfully genotyped for Pfcrt K76T codon, 54 and 29 were males and females, respectively. Males were more represented and contributed for higher prevalence (64.5%) of mutant Pfcrt 76T allele. However, the difference was not statistically significant (P = 0.712).

Prevalence of Pfcrt 76T allele across different age groups per study site

Prevalence of Pfcrt 76T allele was assessed among age groups at Adama, Olenchiti and Metehara sites. High prevalence of Pfcrt 76T alleles was detected among 15–30 age groups with frequencies of 56.3%, 45.5% and 42.1% at Olenchiti, Adama and Metehara sites, respectively (Fig. 4). However, no statistical significance difference of 76T alleles were detected among age groups (Fisher’s exact test, P = 0.69).

Fig. 4
figure 4

Prevalence of Pfcrt 76T CQ-resistant marker among age groups per study sites

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Nested PCR amplification of Pfmsp1 for samples not amplified for Pfcrt K76T and Pfmdr1 N86Y

Out of thirty-eight (38) samples which were not amplified especially for Pfcrt K76T, 26 (68%) of them were amplified by nested PCR for Pfmsp1 allelic families of polymorphic region (Block-2). However, still amplification was unsuccessful for 12 of them.

Discussion

To date, the most important challenge to control and/or eliminate malaria globally is because of emerging and wide-spread anti-malarial drug resistance Plasmodium parasites. In this regard a development in drug resistance by P. falciparum to series of anti-malarial drugs is the most challenge in fighting malaria for several years [2]. The current study aimed to investigate the prevalence of Pfcrt K76T and Pfmdr1 N86Y codons, in P. falciparum isolates collected from Adama, Olenchiti and Metehara sites of East Shewa zone, Oromia Regional State, Ethiopia.

In this study, high frequencies of Pfcrt 76T (91.6%) with no significance difference (P = 0.388) was reported from the study areas. Wild-type Pfcrt K76 allele was only detected in 8.4% P. falciparum isolates. The high proportions of Pfcrt 76T allele in this study is in agreement with studies from various parts of Ethiopia [6, 13, 26]. This persistence of high frequency of 76T allele in Ethiopia may be associated with incomplete withdrawal of CQ as it is currently the first-line anti-malarial drug for the treatment of P. vivax which accounts nearly for 40% of malaria cases in Ethiopia. Moreover, the persistence of vivax malaria in the form of relapse during dry season may also expose P. falciparum to CQ pressure [18]. The dominance of P. vivax over P. falciparum in the study area was already documented which might contribute for such high frequency of 76T allele [13, 18].

Another potential probable reason for circulations of high frequency of Pfcrt 76T mutant allele in the study areas may be because of the existence of mixed infections of P. falciparum and P. vivax [17]. Misdiagnosis of malaria [27], such as mixed infections, as P. vivax and treating patients with CQ was commonly encountered during the study period (unpublished observations) and this may expose P. falciparum to indirect CQ pressure selecting for the mutant genotypes.

To the best of our knowledge, in the present study areas there is no base-line data regarding the prevalence of 76T allele at the time when CQ was replaced with AL. However, 2 years later study conducted by Schunk et al. [28] in Southern Ethiopia showed fixation of 76T in parasite isolates in the area. Ten years later, since the implementation of AL, study conducted at Adama by Golassa et al. [6] revealed fixation of 76T mutant allele in parasite population, however; in the current study wild-type K76 allele was recovered in the frequency of 8.4%. In the current low malaria endemic area [29], the mutant allele still may circulate at high frequencies in parasite populations between human host and Anopheles vectors in the study areas. In this low malaria transmission setting, lower rate of sexual recombination parasite genotypes may take place in Anopheles mosquitoes, which might result in more resistant genotypes to be established in the human host. Therefore, malaria transmission involving multiple genotypes is uncommon in low transmission areas. Conversely, in high malaria transmission areas competition between drug sensitive and drug resistant parasites may slow the spread of drug resistant parasites [23, 30]. Study conducted by Hailemeskel et al. [13] which investigated the prevalence of Pfcrt K76T genotype in low and high malaria endemic areas of Ethiopia [29] showed significantly higher prevalence of 76T and K76 alleles in low and high malaria endemic areas, respectively.

In countries like Ethiopia where CQ drug pressure persists for the treatment of vivax malaria, high frequency of the mutant allele is being reported from Yemen [31], Malaysia [22], Nigeria [32], India [33], Bangladesh [34] and Angola [35]. Conversely, progressive decrease in 76T allele and recovery of K76 allele were documented particularly in sub-Saharan African countries such as Malawi [16] Tanzania [36], Kenya [37] and Uganda [38], where AL is being implemented. Though AL is used as first-line treatment for P. falciparum in Ethiopia low recovery of parasites harbouring wild-type K76 was detected in the study areas may be because of reasons already described above.

In this study, associations of Pfcrt K76T mutation with parasite density, age and gender were investigated. Some studies have associated this mutation with parasite density [22, 31]; while others have found no such associations [39]. In the current study we have found no association of these mutations with parasite density. On the other hand, the detection of high prevalence of this mutation among 15–30 age groups in this study may be explained by more exposure of these groups to mosquito bite and CQ pressure than others. However, no significant association was found between K76T mutation and age of patients which is in agreement with findings of Atrosh et al. [22] and Edogun et al. [40]. Similarly, no positive association of this mutation with gender was detected in this study.

In this study, P. falciparum clinical isolates analysed carried the wild-type genotypes for Pfmdr1 N86. The return to the wild-type genotypes was successful in the gene under report after cessation of CQ and use of AL for the treatment of uncomplicated falciparum malaria in Ethiopia. No single mutant Pfmdr1 86Y genotype was detected in the study under report. This finding is comparable with the previous reports from different parts of Ethiopia [6, 13, 15, 41]. Study conducted 2 years later after implementation of AL in Ethiopia showed the dominance of 86Y allele over its wild allele counterpart [28]. The current high prevalence of N86 allele (CQ sensitive) showed the survival advantage of wild-type over the mutant type since the implementation of AL for the treatment of falciparum malaria in Ethiopia as evident the selection of this allele by AL elsewhere [42].

In different African countries after adoption of AL for the treatment of falciparum malaria progressive increase in N86 allele and decline in 86Y allele have been documented [43, 44]. In vivo therapeutic studies have showed that N86 wild-type is more prevalent in recurrent infections following AL treatment [45]. In support of this meta-analysis of thirty-one clinical trials have showed a five-fold risk of parasite recrudescence in patients infected with parasites harbouring wild-type N86 allele following treatment with AL compared to patients infected with 86Y mutant parasites [46]. Similarly, allelic replacement study conducted by Veiga et al. [9] revealed that substitution of N86Y mutation with N86 withstands three-four fold higher LUM (partner drug of artemether) and MQ concentrations compared to 86Y residues. Although there is no clear evidence linking N86 allele with treatment failure, high prevalence of this allele in treatment failures in Angola [47] and parasite tolerance to LUM [9, 42], is a clear warning signal for plausible emergence of resistance against AL.

There was unsuccessful nested-PCR amplification for 38 of the samples; particularly for Pfcrt K76T codon as was the case for other studies [48]. However, amplification of Pfmsp1gene was successful for 26 of them. This indicated that such parasites may have low concentrated intact DNA that could not be amplified. Still, those 12 samples which were not again amplified for Pfmsp1 indicated that they may be microscopically false positive for P. falciparum [27].

Limitations of the study

The current study is not without limitations. Some of the limitations of the study are small sample size analysed due to logistic constraints, lack of data of copy number variations of the Pfmdr1 -86 as parasites possessing multiply copy of the Pfmdr1 N86 showed decreased susceptibility to MQ, artesunate-amodiaquine and LUM [46] and lack of clinical data on the susceptibility of the parasite to LUM that could be obtained from therapeutic efficacy study.

Conclusion

In conclusion, the present study gives an update on the prevalence of K76T and N86Y alleles in the study areas. A reversal of K76 wild-type allele was detected in non-significant proportions while a fixation of N86 allele was investigated across the study areas. The data obtained from this study calls for continuous monitoring anti-malarial drug resistance against falciparum malaria to maintain efficacy of AL for the treatment of uncomplicated P. falciparum malaria. Based on this assessment we also recommend careful monitoring of CQ usage for P. vivax treatment.

Availability of data and materials

The datasets used and/or analysed for this study are available from the correspondent author on reasonable request.

Abbreviations

ACT:

Artemisinin-based combination therapy

AL:

Artemether–lumefantrine

CQ:

Chloroquine

CQR:

Chloroquine resistance

DBS:

Dried blood spot

LUM:

Lumefantrine

MQ:

Mefloquine

QN:

Quinine

PCR:

Polymerase chain reaction

Pfcrt :

Plasmodium falciparum chloroquine resistane transporter

Pfmdr1 :

Plasmodium falciparum multidrug resistance 1

RFLP:

Restriction fragment length polymorphism

SP:

Sulfadoxine–pyrimethamine

SPSS:

Statistical package for social science

WBCs:

White blood cells

WHO:

World Health Organization

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Acknowledgements

This work is supported by Human, Heredity and Health in Africa (H3Africa) [H3A-18-002]. H3Africa is managed by Science for Africa Foundation (SFA Foundation) in partnership with Wellcome, NIH and AfSHG. We would like to thank participants of this study and laboratory technologists who were involved in collection and examining blood specimen collected from patients attending health facilities. We gratefully acknowledge Oromia Health Bureau for their consent and organizing selected health facilities to collect the data. We would like to extend our gratitude to Aklilu Lemma Institute of Pathobiology who allowed us to use laboratory facilities to perform PCR-RFLP experiments. We also thank Ms. Yergalem G/hiwot and Roza Yoseph for their assistance in laboratory work.

Funding

This work was partially supported by the PAMGEN H3 Africa project (H3A/002/18) through Addis Ababa University, Aklilu Lemma Institute of Pathobiology.

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Authors and Affiliations

  1. Department of Applied Biology, School of Applied Natural Science, Adama Science and Technology University, P. O. Box 1888, Adama, Ethiopia

    Jifar Hassen & Hunduma Dinka

  2. Research and Community Service Center, College of Health Science, Defense University, P. O. Box 1419, Bishoftu, Ethiopia

    Gezahegn Solomon Alemayehu

  3. Aklilu Lemma Institute of Pathobiology, Addis Ababa University, P. O. Box 1176, Addis Ababa, Ethiopia

    Lemu Golassa

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  1. Jifar Hassen
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  2. Gezahegn Solomon Alemayehu
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  3. Hunduma Dinka
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  4. Lemu Golassa
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Contributions

JH designed the study, performed experiments, analysed data, drafted and wrote draft manuscript. LG and GS organized molecular laboratory platform. GS reviewed the manuscript. HD supervised the work and reviewed the manuscript. LG conceived the idea, designed the study, supervised the overall work, participated in the interpretation of results and reviewed the manuscript. All authors read and approved the final version of the manuscript.

Corresponding author

Correspondence to Jifar Hassen.

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Ethical approval and consent to participate

The study was reviewed and approved by Adama Science and Technology University research and ethical committee (certificate Reference No: RECSoANS/BIO/02/2019). Permission latter was also obtained from Oromia Regional State Health Bureau.

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Not applicable.

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Authors declared that they do not have competing interests.

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Supplementary Information

Additional file 1.

Primers sequences used in nested PCR for the amplification of Pfcrt and Pfmdr1 genes.

Additional file 2.

Representative gel image showing digested nested PCR products. (A): K76T codon cleaved with APoI restriction enzyme run in 2.0% agarose gel. L = 100 bp DNA ladder marker, lanes 1–9 are samples, lane 10 is uncut control and lane 11 is wild-type control (Pf3D7). (B): N86Y codon cleaved with APoI restriction enzyme run in 2.5% agarose gel. L = 100 bp ladder, Lanes 1–9 are samples, lane 10 is wild-type pos. cont. (3D7), lane 11 is mutant- type pos. cont. (K1), and lane 12 uncut control.

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Hassen, J., Alemayehu, G.S., Dinka, H. et al. High prevalence of Pfcrt 76T and Pfmdr1 N86 genotypes in malaria infected patients attending health facilities in East Shewa zone, Oromia Regional State, Ethiopia. Malar J 21, 286 (2022). https://doi.org/10.1186/s12936-022-04304-5

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Keywords

  • Plasmodium falciparum
  • Anti-malarial drug resistance
  • Pfcrt
  • Pfmdr1
  • Ethiopia

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