In vitro selection of Plasmodium falciparum Pfcrt and Pfmdr1 variants by artemisinin
© The Author(s) 2016
Received: 27 February 2016
Accepted: 18 July 2016
Published: 22 July 2016
Anti-malarial drugs are the major focus in the prevention and treatment of malaria. Artemisinin-based combination therapy (ACT) is the WHO recommended first-line treatment for Plasmodium falciparum malaria across the endemic world. Also ACT is increasingly relied upon in treating Plasmodium vivax malaria where chloroquine is failing. The emergence of artemisinin drug-resistant parasites is a serious threat faced by global malaria control programmes. Therefore, the success of treatment and intervention strategies is highly pegged on understanding the genetic basis of resistance.
Here, resistance in P. falciparum was generated in vitro for artemisinin to produce levels above clinically relevant concentrations in vivo, and the molecular haplotypes investigated. Genomic DNA was extracted using the QIAamp mini DNA kit. DNA sequences of Pfk13, Pfcrt and Pfmdr1 genes were amplified by PCR and the amplicons were successfully sequenced. Single nucleotide polymorphisms were traced by standard bidirectional sequencing and reading the transcripts against wild-type sequences in Codon code Aligner Version 5.1 and NCBI blast.
Exposure of parasite strains D6 and W2 to artemisinin resulted in a decrease in parasite susceptibility to artemisinin (W2 and D6) and lumefantrine (D6 only). The parasites exhibited elevated IC50s to multiple artemisinins, with >twofold resistance to artemisinin; however, the resistance index obtained with standard methods was noticeably less than expected for parasite lines recovered from 50 µg/ml 48 h drug pressure. The change in parasite susceptibility was associated with Pfmdr-185K mutation, a mutation never reported before. The Pfcrt-CVMNK genotype (Pfcrt codons 72–76) was retained and notably, the study did not detect any polymorphisms reported to reduce P. falciparum susceptibility in vivo in the coding sequences of the Pfk13 gene.
This data demonstrate that P. falciparum has the capacity to develop resistance to artemisinin derivatives in vitro and that this phenotype is achieved by mutations in Pfmdr1, the genetic changes that are also underpinning lumefantrine resistance. This finding is of practical importance, because artemisinin drugs in Kenya are used in combination with lumefantrine for the treatment of malaria.
Artemisinin resistance phenotype as has been shown in this work, is a decrease in parasites susceptibility to artemisinin derivatives together with the parasite’s ability to recover from drug-induced dormancy after exposure to drug dosage above the in vivo clinical concentrations. The study surmises that Pfmdr1 may play a role in the anti-malarial activity of artemisinin.
Malaria is one of the most serious life-threatening protozoan diseases, classically identified by paroxysm, fever, and flu-like symptoms recurring in 48- or 72-h cycles. The World Health Organization (WHO) recommends artemisinin-based combination therapy (ACT) as the first-line treatment for falciparum malaria in all endemic regions . There is already evidence of reduced susceptibility of P. falciparum to artemisinin derivatives in Southeast Asia which is manifested by the delayed parasite clearance times in vivo [2, 3]. WHO has launched an action plan to stop possibly emerging resistance at an early stage so as to protect ACT .
The P. falciparum multidrug resistance 1 gene (Pfmdr1), P. falciparum chloroquine resistance transporter gene (Pfcrt), and kelch13 propeller region (Pfk13) gene single nucleotide polymorphisms (SNPs) are believed to be markers of resistance to a great number of anti-malarial drugs, including ACT [5, 6].
Increased copy number and sequence variation in Pfmdr1 at the amino acid positions N86Y, S1034, N1042 and D1246Y have been reported to interfere with the parasite susceptibility to dihydroartemisinin , artemisinin [8, 9], mefloquine , quinine , halofantrine , piperaquine , lumefantrine , amodiaquine  and chloroquine . Recent in vitro work have strongly linked Pfmdr1 to drug transportation .
The Pfcrt protein has capacity to efflux peptides and glutathione , and transport anti-malarials besides chloroquine . Its codon K76T mutation has been linked to the development of chloroquine resistance . Pfcrt SNPs have also been found to be associated with the in vitro and/or in vivo parasite susceptibility to artemisinin , lumefantrine , quinine , mefloquine  and piperaquine .
The Pfk13 SNPs;C580Y, R539T, I543T, and Y493H were the four main alleles which were observed to be significantly involved in artemisinin resistance out of the 17 non-synonymous SNPs found in Cambodia . Other genes associated with artemisinin resistance include; Pfcrt , P. falciparum translationally controlled tumor protein (Pftctp) gene , Pfmdr1, P. falciparum multidrug resistance-associated protein-1 (Pfmrp1)  and ABC transporters . Also there are target proteins; P. falciparum calcium adenosine triphosphatase 6 (Pfatpase6)  and P. falciparum ubiquitin c-terminal hydrolase (Pfubcth), the orthologue of P. chabaudi ubiquitin protein-1 .
The identification of the genetic determinants will be cornerstone for understanding the molecular basis of artemisinin drug resistance and will, therefore, provide basic evidence for molecular surveillance of drug-resistant P. falciparum strains for epidemiological surveys. This study reports an assessment of anti-malarial resistance marker polymorphisms in Pfmdr1, Pfcrt, and Pfk13 genes in chloroquine resistant W2 and chloroquine sensitive D6 lines cultured in presence of artemisinin.
The study was carried out at the Centre for Biotechnology Research and Development (CBRD) malaria laboratory, Kenya Medical Research Institute (KEMRI) Headquarters, Nairobi, Kenya.
Two P. falciparum laboratory clones, W2 (Indochina) and D6 (Sierra Leone) were cultivated by standard methods, as described by Trager and Jensen  with some modifications described by Benoit-Vical et al. . Continuous routine cultures were maintained at 1–5 % parasitaemia in complete medium containing 12.5 % heat inactivated human serum (blood type A, AB and O pooled) and in O+ human erythrocytes. Haematocrit was adjusted to 6 % O+ type RBCs of the 5 ml total culture volume. The choice of the two parasite lines (D6 and W2) was made in the anticipation that different genetic backgrounds of the parasites may provide a wider span of genetic determinants during the in vitro evolution by artemisinin selection.
Development of resistant parasite lines
Artemisinin resistance was induced in P. falciparum W2 and D6 lines as described by Oduola et al. . Plasmodium falciparum W2 and D6 lines were cultured under increasing artemisinin pressure in stepwise increments over 450 days. The starting concentration of artemisinin was 10 µg/ml for the two parasite clones (W2 and D6). Then, increments were in escalations of 10, 20, 30, 40 and 50 µg/ml, with an exposure time of 48 h at each increment.
The drug pressure cycle started with the addition of artemisinin to asynchronous cultures with 4–8 % parasitaemia. The 12.5 % human-serum-supplemented growth medium (RPMI Medium 1640; Gibco®), with or without artemisinin, was changed after 24 h. The artemisinin pressure was removed after 48 h, the time at which parasite morphology was degraded and growth was significantly reduced. The medium containing artemisinin was discarded and parasites washed twice with drug free wash media. Then, drug-free culture medium supplemented with 12.5 % human-serum was added to cultures, which were incubated at 37 °C until parasite growth and morphology became normal.
A parasite was considered “tolerant” to a particular artemisinin concentration when the recovery phase occurred within 48 h. The artemisinin exposure time was between 42 and 173 days so as to reduce the recovery time to below 48 h for the W2 and D6 lines at each increment. This was considered as a cycle of artemisinin pressure. At this point, artemisinin pressure was resumed with the consecutive higher artemisinin concentration in the increment to culture which has attained ≥5 % parasitaemia. During adaptation, parasite was frozen and the procedure was resumed from the cryopreserved stocks to maintain this phenotype.
Bulk culture of W2 cycle 5 culture A at 50 µg/ml artemisinin (W2 c5A), D6 cycle 3 culture A at 30 µg/ml artemisinin (D6 c3A) and D6 cycle 5 culture A at 50 µg/ml artemisinin (D6 c5A) parasites was cloned by limiting dilution for 35 days to give W2 cycle 5 sub-culture B (W2 c5B), D6 cycle 3 sub-culture B (D6 c3B) and D6 cycle 5 sub-culture B (D6 c5B), respectively. However, W2 cycle 3 culture A at 30 µg/ml artemisinin (W2 c3A) was not cloned. The samples of these cultures were collected and stored in extraction buffer for further analysis. Artemisinin together with other conventional anti-malarials [dihydroartemisinin (DHA), artemisinin (QHS), artesunate (AS), artemether (AM), chloroquine diphosphate (CQ), lumefantrine (LUM) and piperaquine phosphate (PIP)], susceptibilities were assayed by measuring the inhibition of [3H] hypoxanthine uptake in a sterile technique , as described herein.
[3H] hypoxanthine incorporation assays
Plasmodium falciparum growth was determined by measuring incorporation of the nucleic acid precursor [3H] hypoxanthine in the parasites genomic DNA. Test compounds were diluted in DMSO (except CQ; diluted in water) and diluted to >0.2 % DMSO. 25 µl of screening medium was added to each well (except row B) in a 96-well flat-bottom micro-culture plate (Costar®, Corning Incorported, NY, USA). Fifty microlitre of dissolved compounds, containing four times the highest test concentration, were added to wells of row B in duplicates. Two times serial drug dilutions were prepared using a multichannel pipette. Twenty five microlitre of drug solution were taken from wells of row B and transferred, after mixing, to wells of row C and so forth down to row H (a 64-fold range dilution). The 25 µl of diluent removed from wells of row H were discarded. Two hundred microlitre of infected erythrocytes (1.5 % haematocrit and 0.5 % parasitaemia) were then added to each well except for wells A9–A12, to which, 200 µl of uninfected RBCs (diluted in screening medium to 1.5 % haematocrit) were added as a negative control.
The plates were incubated at 37 °C in a chamber gassed by a medical grade gas mixture of 92 % N2, 3 % O2, and 5 % CO2 at 95 % humidity. After a 48-h incubation period, 25 µl of [3H] hypoxanthine working solution was added by pulsing to each well (0.5 µCi per well).
Plates were incubated for an additional 18 h period then frozen at negative 20 °C. After thawing, the content of the plates was harvested onto glass-fiber filter mats (A 1450-421; Perkin Elmer) using a Betaplate cell harvester (1295-004 Betaplate; Wallac Perkin Elmer) and dried in an oven.
The oven-dried filter mats were drenched in 10 ml of scintillation fluid (Beta Scintilla®, Perkin Elmer, Schwerzenbach, CH) in a plastic foil (1450-432; Perkin Elmer) and the [3H] hypoxanthine incorporation was measured in terms of counts per minute (cpm) using a Betaplate liquid scintillation counter (1205 Betaplate; Wallac Perkin Elmer).
The result of each well was recorded as counts per minute and expressed as percentage of the untreated (positive) control (wells A1–A8; cultures without test compound). The negative control was used for background subtraction. IC50s (drug concentration at which 50 % of [3H] hypoxanthine incorporation was inhibited compared to drug-free controls) were estimated by linear interpolation .
Data analysis was done using Graph Pad Prism software, version 5 (Graph Pad Software, Inc.), and the concentrations of the drugs that inhibited parasite growth by 50 % (IC50) were obtained by nonlinear regression analysis of the inhibition of uptake values and log-transformed concentration values.
Genomic DNA isolation
The genomic DNA was extracted from 1 to 2 ml aliquots of parasite cultures by using the QIAamp mini DNA kit (Qiagen, Germany) as per the manufacturer’s specifications and eluted in 50 µl of AE elution buffer. Non-template control samples were obtained by using un-parasitized red blood cells in each extraction. The untreated parasites (i.e., no drug pressure, W2 and D6) samples, cultured for the same period of 450 days, were used as the positive controls.
Sequencing of the Pfmdr1, Pfcrt and Pfk13 genes
Primers used in PCR
Pfk13 PlasmoDB PF3D7_1218300
K13-2 (5′-gccaagctgccattcatttg -3′)
K13-3 (5′-gccttgttgaaagaagcaga -3′)
Nucleotide sequence accession numbers
The DNA sequences of representative samples showing mutant types were submitted to Gen-Bank and assigned accession numbers KU236713 and KU236714.
Discontinuous drug pressure generates P. falciparum lines tolerant to increased levels artemisinin in vitro
In vitro susceptibility testing of parental and resistant lines to anti-malarial drugs
2.85 ± 0.55
127.66 ± 1.96
64.18 ± 10.18
10.49 ± 0.06
3.92 ± 0.66
0.45 ± 0.16
0.60 ± 0.15
9.13 ± 0.127
60.63 ± 8.62
51 ± 4.23
10.5 ± 0.27
5.44 ± 0.20
0.94 ± 0.26
2.35 ± 0.65
3.06 ± 0.19
12.67 ± 0.03
44.37 ± 11.69
54.9 ± 3.99
8.74 ± 0.35
1.64 ± 0.45
1.454 ± 0.35
8.26 ± 0.55
11.67 ± 2.05
55.46 ± 3.4
84.58 ± 1.64
12.26 ± 0.66
4.19 ± 1.03
7.66 ± 0.36
15.5 ± 0.95
13.36 ± 1.09
55.04 ± 0.81
54.52 ± 5.88
9.68 ± 2.17
2.78 ± 0.14
4.66 ± 0.93
Resistant phenotype was due to polymorphism in Pfmdr1 gene
Pfmdr1 and Pfcrt allelic types in parental and resistant P. falciparum lines
Pfmdr1 Amino acid position
Pfcrt Amino acid positions
Codons 72–76 of Pfcrt
The wild-type Pfcrt allele, encoding CVMNK at codons 72–76 of the crt protein was confirmed as present in both D6 (one sample of the one sequenced, D6 isolate) and its tolerant progenies (four samples of the four sequenced, D6 c3A, D6 c3B, D6 c5A and D6 c5B), but W2 (one sample of the one sequenced, W2 isolate) and its subsequent progenies (three samples of the three sequenced, W2 c3A, W2 c5A and W2 c5B) harboured the CVIET allele.
The changes in amino acid sequences at codon C580Y, R539T, I543T, and Y493H as has been reported by Ariey et al. , were not detected in either parent lines W2 and D6 or their artemisinin tolerant progenies and all the coding sequences were “wild type”.
There are several drawbacks to ACT as the current strategy, despite its success over the last decade. The WHO  currently endorses five combinations artemether-lumefantrine, dihydroartemisinin–piperaquine phosphate, artesunate-amodiaquine, artesunate-mefloquine, and artesunate–pyronaridine. ACT is a highly used anti-malarial, creating a substantial selection advantage for parasites to evolve resistance independently with a precipitous decline in the artemisinin susceptibility.
In 2014, the number of courses treatment using various artemisinin-based combinations increased from 11 million in 2005 to 337 million , but the mechanisms by which artemisinin act is still under investigation. Deducing molecular genetics on its resistance is paramount for determining treatment strategies, mapping the spread of resistance and guiding elimination [27, 35, 36]. For the new tools for resistance surveillance to be validated a better understanding of the mechanisms of artemisinin resistance is needed. These tools are essential in guiding national treatment policies and helping in designing and deploying new drug combinations that may counter the emergence and spread of resistance.
In the present study, the discontinuous method of inducing resistance/tolerance to artemisinin in W2 and D6 lines of P. falciparum was used . In agreement with other study , the in vitro developed artemisinin-tolerant parasites could not grow permanently under artemisinin pressure. Hence resistance to artemisinin is different from resistance to other conventional anti-malarial drugs, such as amodiaquine. The culmination of in vitro resistance as used here in, is the ability for parasites to survive pharmacologically relevant exposure of artemisinin (levels considered clinically relevant in vivo) over many generations and by major increases in the IC50. After conducting the [3H] hypoxanthine incorporation susceptibility assays, it was found that resistant parasites showed the greatest tolerance for artemisinin (W2 c5B and D6 c5B). The study hypothesized a reduced susceptibility to this drug, because it was used to induce resistance in these strains. The discontinuous drug pressure selection scheme is supposedly to have been the key to success in selecting the tolerant lines . After adapting, the parasites were able to tolerate as much as 50 µg/ml of artemisinin for 48 h without noticeable changes in growth rate or morphology. The results also showed resistant parasites generally had decreased susceptibility to artemisinin, but were more susceptible to CQ, which is in agreement with other studies [7, 37, 38]. There was a significant degree of cross-resistance to various other artemisinin derivatives, including artemether, artesunate, and dihydroartemisinin which were not utilized in the generation of resistance in those particular lines. This highlights that, it is possible to select resistance in a drug-sensitive background (D6) African isolate, in antagonism to conclusion from other studies in which it was stated that multiple resistance phenotypes must pre-exist [39, 40].
These artemisinin-tolerant parasites provided a unique resource for the study of the artemisinin resistance mechanism(s) and modes of action based on analysis of SNPs in Pfmdr1, Pfk13 and haplotypes in Pfcrt. The rationale for considering using these three genes were (i) that a relationship between SNPs in Pfmdr1 and ACT has been reported, suggesting that Pfmdr1-N86 or -184F was selected in reinfections after artemether-lumefantrine treatment; and moreover, Pfcrt-76K and Pfmdr1-N86 were selected by artemether-lumefantrine in recurrent infections . Pfmdr1 and Pfcrt were selected for chloroquine resistance and they also both have been reported to be associated with in vitro reduced susceptibility to artesunate and amodiaquine . (ii) Genome association studies strongly suggested a locus on P. falciparum chromosome 13 gene PF3D7_1343700 (bases 1,724,817–1,726,997, PlasmoDB 11.1) to artemisinin resistance and mutations discovered in the Pfk13 were strongly linked to artemisinin resistance .
It is well known that Pfmdr1 is associated with drug resistance in Asia [7, 38]. Pfmdr1 encode protein of the ATP binding cassette (ABC) transporter superfamily encoding P-glycoprotein homologue-1 , which are localized to the parasite food vacuole membrane or plasma membrane and can decrease intracellular drug accumulation by pumping out drugs.
SNPs at codons 86, 184, and 1246 of the Pfmdr1 gene has been suspected to be the markers of changes in parasite susceptibility to various drugs, including ACT . This shows that monitoring of changes in prevalence of SNPs in the Pfmdr1 gene may serve as an early warning tool to selection of P. falciparum tolerant/resistant to ACT .
In the two artemisinin-tolerant parasite lines used in the present study, the decrease in parasite susceptibility to the drug was associated with substitution of mutation at codon Y184F for I185K. This conforms with other studies where sequence variation and increase in copy number in Pfmdr1 were reported to interfere with the parasite susceptibility to dihydroartemisinin  and artemisinin . This is because; the mutation at codon Y184F was not detected in the two studies. However, other studies have shown a relationship between SNPs in Pfmdr1 and ACT drugs, in that Pfmdr1-N86 or -184F was selected in reinfections and Pfcrt-K76 and the Pfmdr1-N86 in recurrent infections after artemether-lumefantrine treatment .
It is established that ACT can select for particular alleles of two genes, Pfmdr1 and Pfcrt, which are firmly associated with resistance to the 4-aminoquinolines chloroquine and amodiaquine. The Pfcrt gene that encodes a 424-amino acid integral 10 trans-membrane domains protein is a transporter present in the parasite digestive vacuole membrane.
In this work, it was observed that Pfcrt-CVMNK were the favoured haplotypes. This can be attributed to compensatory mutation at C350R in a different study, which was shown to explain the seemingly discordant chloroquine response in Pfcrt-CVIET haplotype . This may suggest the benefit of the two wild-type genes, Pfmdr1-N86 Y184 and Pfcrt-CVMNK, was enhanced by the presence of artemisinin.
Ariey et al.  linked artemisinin resistance in P. falciparum to slow clearance rates in patients which he strongly associated with single point mutations in the “propeller” domain of the P. falciparum kelch protein gene on chromosome 13 (kelch13) (PlasmoDB identifier PF3D7_1218300). 17 mutations in the propeller region are linked to artemisinin drug resistance. The Pfk13 gene is well conserved across Plasmodium species and is thought to mediate protein–protein interactions .WHO included Pfk13 mutations (Y493H, I543T, R539T, C580Y and M476I) in the new working definition for suspected artemisinin resistance in August 2014 . The present study did not detect any polymorphisms reported elsewhere to reduce P. falciparum susceptibility in vivo in the coding sequences of the Pfk13 gene.
Although it is clear that Pfmdr1 may play a significant role in artemisinin resistance, some studies also demonstrated that changes in susceptibility to mefloquine or halofantrine could be achieved without changes in the expression level or allelic type of Pfmdr1 [47, 48], suggesting a possible involvement of other genes and/or mechanisms of sustaining resistance in these parasites, including transient changes in gene expression.
Other work has reported lack of mutations in Pfmdr1 and Pfcrt in parasites cultured for 5 years under artemisinin derivatives in vitro, and Pfmdr1 amplification was not observed. Further, four mutations were discovered in Pfk13 (Y493H, I543T, R539T and C580Y). In the same study, 17 single K 13-propeller mutations were detected in naturally circulating parasites in Cambodia . However in the present study, there was Pfmdr1 novel mutation at codon I185K and no non-synonymous mutations in Pfk13 gene. This difference can be attributed to the shorter period (450 days) of artemisinin exposure.
ACT is the critical tool for controlling the world’s most important parasitic disease; malaria. This necessitates research on artemisinin resistance markers for epidemiological surveys in malaria endemic regions. This work has demonstrated that resistance to artemisinin can be induced in P. falciparum in vitro. Although long-term stability studies at high levels of drug exposure have not been completed; this data suggest that stable artemisinin tolerance was selected for by multiple pulse exposures to drug over time. This is reflected in the substitution of Pfmdr1 Y184F mutation for I185K. Clearly, more studies are required to identify the mechanism(s) by which resistance to artemisinin emerges and to find molecular genetic markers that can be used for epidemiological studies to track the possible emergence of artemisinin resistance.
High artemisinin resistant lines should be selected and probably to a line which can grow continuously under artemisinin pressure. Thereafter, the investigations into artemisinin resistance markers mainly targeting the implicated genes Pfk13, Pfmdr1 and Pfubcth associated with reduction in drug efficacy should be performed. Structured studies that mitigate confounding factors such as multiple clonal infections in a variety of crossing experiments should be investigated in vivo. This is because in the laboratory, the effect of the mutation is determined in only one genetic background but a wide variety of backgrounds are found in the field due to recombination.
JNK was the principal investigator for the study, initiated, mapped the design, supervised and assisted in data analysis and manuscript review. FTK supervised the project activities, laboratory experiments and provided guidance on the analysis plan and manuscript review. DK initiated, mapped the designed, supervised and manuscript review. JK supervised the project; assisted in data analysis and manuscript review. MJN initiated, contributed to the study design, performed all experiments, analysed the data and wrote the manuscript. All authors read and approved the final manuscript.
We would like to express our gratitude to all the administrative authorities the Director KEMRI and the entire staff of the Centre for Biotechnology Research and Development (CBRD) malaria laboratory, KEMRI in Nairobi.
The authors declare that they have no competing interests.
Ethics approval and consent to participate
The study was approved by Scientific Ethical Review Committee (SERU), in Kenya Medical Research Institute, KEMRI (SERU/CBRD/132/3127). The blood for obtaining host red blood cells (RBCs) and human sera was obtained upon signed acceptance of informed consent terms and conditions by the participant.
This work was supported by the AFRICA-ai-JAPAN Project through the ICMoB (Innovation Centre for Molecular Biology and Biochemistry) and JKUAT research project and extension office.
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