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Genetic diversity of the msp-1, msp-2, and glurp genes of Plasmodium falciparum isolates in Northwest Ethiopia

  • 1Email author,
  • 1,
  • 1,
  • 1,
  • 1 and
  • 2
Malaria Journal201817:386

https://doi.org/10.1186/s12936-018-2540-x

  • Received: 4 July 2018
  • Accepted: 20 October 2018
  • Published:

Abstract

Background

Determination of the genetic diversity of malaria parasites can inform the intensity of transmission and identify potential deficiencies in malaria control programmes. This study was conducted to characterize the genetic diversity and allele frequencies of Plasmodium falciparum in Northwest Ethiopia along the Eritrea and Sudan border.

Methods

A total of 90 isolates from patients presenting to the local health centre with uncomplicated P. falciparum were collected from October 2014 to January 2015. DNA was extracted and the polymorphic regions of the msp-1, msp-2 and glurp loci were genotyped by nested polymerase chain reactions followed by gel electrophoresis for fragment analysis.

Results

Allelic variation in msp-1, msp-2 and glurp were identified in 90 blood samples. A total of 34 msp alleles (12 for msp-1 and 22 for msp-2) were detected. For msp-1 97.8% (88/90), msp-2 82.2% (74/90) and glurp 46.7% (42/90) were detected. In msp-1, MAD20 was the predominant allelic family detected in 47.7% (42/88) of the isolates followed by RO33 and K1. For msp-2, the frequency of FC27 and IC/3D7 were 77% (57/74) and 76% (56/74), respectively. Nine glurp RII region genotypes were identified. Seventy percent of isolates had multiple genotypes and the overall mean multiplicity of infection was 2.6 (95% CI 2.25–2.97). The heterozygosity index was 0.82, 0.62 and 0.20 for msp-1, msp-2 and glurp, respectively. There was no significant association between multiplicity of infection and age or parasite density.

Conclusions

There was a high degree of genetic diversity with multiple clones in P. falciparum isolates from Northwest Ethiopia suggesting that there is a need for improved malaria control efforts in this region.

Keywords

  • Genetic diversity
  • Plasmodium falciparum
  • Multiclonal infection
  • Ethiopia

Background

Over the last decade, the burden of malaria has declined considerably in Ethiopia, which could be the result of effective implementation of malaria control strategies at the lowest administrative levels [1]. Progress made in the reduction of this burden is attributed to implementation of effective prevention and treatment tools, such as long-lasting insecticidal nets (LLINs), indoor residual spraying (IRS) and prompt treatment of cases using artemisinin-based combination therapy (ACT) [2, 3]. However, malaria still remains one of the major health problems in the country. Approximately 60% of the population lives in malaria endemic areas [4] and malaria remains among the top ten causes of morbidity and mortality in children under 5 years [5].

The population genetic diversity of malaria varies according to the transmission intensity in malaria endemic regions and is higher in hyperendemic areas compared to areas of low endemicity [69]. Parasite genetic characteristics may thus reflect the dynamics of parasite transmission. Furthermore, human migration events may play a role by enhancing change in parasite populations [6]. In addition, declining malaria transmission as a result of scaling-up interventions has been shown to affect the parasite genetic diversity pattern and population structure of Plasmodium falciparum [7, 10], although this has not occurred in all settings. [7, 11].

Genetic diversity of P. falciparum is usually determined through genotyping of the polymorphic regions of the block 2 of merozoite surface protein-1 (msp-1), block 3 of merozoite surface protein-2 (msp-2) and the RII repeated region of the glutamic rich protein (glurp) [12]. Three major allelic families have been identified in block 2 of the msp-1 gene, K1, MAD20, and RO33 [13] and two allelic families in the msp-2 gene, IC/3D7 and FC27 [15]. These markers are used to investigate the genetic diversity, multiplicity of infection, the level of malaria transmission, and to discriminate new from recrudescent infections in therapeutic efficacy monitoring studies [14].

To date, there has been limited assessment of genetic diversity of P. falciparum in Ethiopia [15, 16], despite scaling up of national malaria control interventions [17]. This study aimed to characterize the genetic diversity and allele frequencies of msp-1, msp-2 and glurp genes of P. falciparum isolates from uncomplicated malaria patients in Humera along the Ethiopian border.

Methods

Study site

Samples used for this study were collected from the town of Humera, a sentinel site for monitoring of therapeutic efficacy to artemether-lumefantrine (Coartem®) in Northwest Ethiopia (Fig. 1). The town is situated in the Tekezze river basin and has a suitable habitat to support mosquitoes that transmit malaria. Malaria in this area is mesoendemic, with peak transmission between September and December following the rainy season [18, 19]. A migrant population flows into Humera during the harvest season (September–November), and this population bears the highest malaria burden. Sesame and barley are the main crops in the area. A detailed description of this site has been previously published [20].
Fig. 1
Fig. 1

Map of the sample collection area, Humera, Northwest Ethiopia, orange colour indicated the sampling site

Study population and blood sample collection

A total of 90 blood spot samples were collected from patients with uncomplicated P. falciparum enrolled during therapeutic efficacy monitoring of artemether-lumefantrine between October 2014 and January 2015. Included patients were aged between two and 28 years, were residents within the Humera area, had presented to the local health centre with fever (axillary temperature ≥ 37.5 °C) and were found to be positive for asexual P. falciparum. After consent was obtained, dried blood spots were collected on day zero of enrollment through finger prick bleeding spotted onto Whatman 903® filter paper (Schleicher & Schuell Bio Science, Keene, NH 03431, USA). These dried blood spots were transported and stored at − 20 °C at the Malaria Research Laboratory (Ethiopian Public Health Institute) in Addis Ababa, Ethiopia.

Parasite DNA extraction

Parasite genomic DNA was extracted from the blood spots collected on filter papers using Chelex-100® (Bio-Rad Laboratories CA) method [21], with a final volume of 200 µl for each sample and storage at − 20 °C until it was used for the amplification reaction.

Genotyping of the msp-1, msp-2 and glurp genes of Plasmodium falciparum

Nested PCR of the polymorphic regions of msp-1 (block2), msp-2 (block 3), and glurp (RII repeat region) was performed using primers and methods as previously described [22, 23]. In brief, in the initial amplification, primer pairs corresponding to conserved sequences within the polymorphic regions of each gene were included in separate reactions. The product generated in the initial amplification was used as a template in six separate nested PCR reactions. In the nested reaction, separate primer pairs targeted the respective allelic types of msp-1 (K1, MAD20 and RO33), msp-2 (IC3D7 and FC27), and the RII blocks of glurp with an amplification mixture containing 250 nM of each primer (except glurp nest 1 primers where 125 nM were used (Additional file 1: Table S1), 2 mM of MgCl2 and 125 µM of each dNTPs and 0.4 units Taq DNA polymerase. The cyclic conditions in the thermocycler (MyCycler-BioRad, Hercules, USA), for initial msp-1 and msp-2 PCR and initial and nested glurp PCR were as follows: 5 min at 95 °C, followed by 30 cycles for 1 min at 94 °C, 2 min at 58 °C and 2 min at 72 °C and final extension of 10 min at 72 °C. For msp-1 and msp-2 nested PCR, conditions were as follows: 5 min at 95 °C, followed by 30 cycles for 1 min at 95 °C, 2 min at 61 °C and 2 min at 72 °C and final extension of 5 min at 72 °C. The allelic specific positive control 3D7 and DNA free negative controls were included in each set of reactions [24]. Fragment analysis of msp-1, msp-2 and glurp amplified products were then performed through electrophoresis on 2% agarose gels visualized under ultraviolet transillumination with light after staining with ethidium bromide. The size of DNA fragments were estimated by visual inspection using a 100 bp DNA ladder marker (Invitogen, Kalsruhe, Germany). The detection of a single PCR fragment for each locus was classified as an infection with one parasite genotype (monoclonal infection). Isolates with more than one genotype were considered as polyclonal infection [25]. Alleles in each family were considered the same if fragment sizes were within 20 bp intervals for msp-1 and msp-2 genes [26], and 50 bp intervals for glurp gene [12].

Data analysis

The msp-1, msp-2 and glurp allele frequencies were expressed as the proportion of samples containing an allelic family compared to the total number of samples that gene was detected in. Multiplicity of infection (MOI) was defined as the number of parasite genotypes per infection. Estimation of mean MOI was calculated by dividing the total number of fragments detected in msp-1, msp-2, or glurp by the number of samples in the same marker. Spearman’s rank correlation coefficient was calculated to assess associations between MOI and parasite density and age. Statistical significance was set at P < 0.05. The heterozygosity index (He), which represents the probability of being infected by two parasites with different alleles at a given locus, was calculated using the formula: He = [n/(n − 1)] [(1 − Σpi2)], where n is the number of isolates sampled and pi is the allele frequency at a given locus [27]. All statistical analyses were performed using SPSS version 20.0 (SPSS Inc., Chicago, IL, USA).

Ethical clearance

Ethical approval for the study was given by the Scientific and Ethical Review Office (SERO) of the Ethiopian Public Health Institute (EPHI). Written informed consent was obtained from parents or guardian prior to recruitment.

Results

Demographic and parasitological data

The characteristics of the study population are demonstrated in Table 1. The 90 patients included 56 (62.2%) males and 34 (37.8%) females, with a mean age of 15.1 ± 5.8 years. They had asexual parasitaemia ranging from 1128 parasites to 199,346 parasites/µl and a geometric mean of 14,140.9 parasites/µl (95% CI 11,047–18,078). Patients 5 to 15 years of age had the highest mean parasite density 30,429 parasites/µl (95% CI 16,104–50,159) compared to other age groups.
Table 1

Demographic, parasitological and clinical features of the study subjects’ profiles from Humera area, Northwest Ethiopia

Characteristic

Value

Sex ratio(M/F)

1.7 (56/34)

Age, years

Range

2 to 28

Mean ± SD

15.1 ± 5.8

Age group

 Children (2–5 years)

3 (3.3%)

 Children (5–15 years)

33 (36.7%)

 Adult(≥ 15 years)

54 (60%)

Geometric mean of parasitemia (parasites/µl)

14,141 (11,046.6–18,077.9)

Parasite density range

1128–199,346

SD standard deviation, µl microliter

Allelic diversity of msp-1, msp-2 and glurp genes in P. falciparum

Alleles of msp-1, msp-2 and glurp were classified according to the size of their PCR amplified fragments (Additional file 2: Figure S1; Additional file 3: Figure S2; Additional file 4: Figure S3). Successful amplification occurred in 97.8% (88/90) of samples for msp-1, 82.2% (74/90) for msp-2 and 46.7% (42/90) for glurp.

Allele genotyping demonstrated the highly polymorphic nature of P. falciparum in Humera isolates with respect to msp-1and msp-2. Among msp-1 isolates, three K1 (150–200 bp), five MAD20 (150–250 bp) and four RO33 (120–230 bp) allelic families were noted. The frequency of samples with only K1, MAD20, and RO33 were 1.1, 10.2 and 5.7%, respectively. The remaining 82.9% (73/88) were polyclonal infections. Among polyclonal infections carrying two allelic types, the frequency of samples with K1/MAD20, K1/RO33, and MAD20/RO33 was 21.6%, 18.2% and 25%, respectively. Infections with all three allelic types were detected in 18.2% of cases (Table 2).
Table 2

Genotyping of P. falciparum msp-1 polymorphic region block 2 in Humera, Ethiopia

MSP-1 (n = 88)

Frequency (%)

Allele size (bp)

No of alleles

MOI

K1

1 (1.1%)

150–200

3

2.0

MAD20

9 (10.2%)

150–250

5

 

RO33

5 (5.7%)

120–230

4

 

K1+MAD20

19 (21.6%)

   

K1+RO33

16 (18.2%)

   

MAD20+RO33

22 (25%)

   

K1+MAD20+RO33

16 (18.2%)

   

Bp base pairs, MOI multiplicity of infection

A total of 22 different alleles were identified for msp-2, including ten alleles of FC27 and 12 alleles of IC/3D7. Allele sizes ranged from (250 to 700 bp) for FC27 and (280 to 780 bp) for IC/3D7 allelic families. The frequency of FC27 and IC/3D7 were 77% (57/74) and 76% (56/74), respectively. The frequency of samples with only FC27 and IC/3D7 were 24.3% and 23.0%, respectively. Thirty-nine of the isolates (52.7%) carried both msp-2 allelic families (Table 3).
Table 3

Genotyping of P. falciparum msp-2 polymorphic region block 3 in Humera, Ethiopia

msp-2 (n = 74)

Frequency (%)

Allele size (bp)

No of alleles

MOI

FC27

18 (24.3%)

250–700

10

1.9

IC/3D7

17 (23.0%)

280–780

12

 

FC27+IC/3D7

39 (52.7%)

   

Bp base pairs, MOI multiplicity of infection

Forty-two samples were successfully genotyped for the glurp RII repeat region ranging from 350 to 800 bp. A total of nine different alleles were detected and coded as genotypes I-IX. Genotype III was the most common (26%), followed by genotype I (21%) and genotype IV (19%) (Table 4).
Table 4

Distribution of allelic variants of glurp RII repeat region of P. falciparum populations in Humera, Ethiopia

Genotypes

Allelic size variants (50 bp bin)

N (%)

I

301–350

9 (21)

II

351–400

4 (10)

III

401–450

11 (26)

IV

451–550

8 (19)

V

551–600

2 (5)

VI

601–650

1 (2)

VII

651–700

2 (5)

VIII

701–750

2 (5)

IX

751–800

3 (7)

glurp glutamate rich protein, N number of sample

Multiple infections of msp-1, msp-2 and glurp alleles were detected in 88.6% (78/88), 70.3% (52/74) and 7.1% (3/42), respectively. Sixty-three of 90 samples (70%) harboured multiple genotypes. The overall mean multiplicity of infection was 2.6 (95% CI 2.25–2.97). When considering msp-1, msp-2 and glurp separately, the multiplicity of infection was 1.98 (95% CI 1.68–2.00), 1.89 (95% CI 1.68–2.28) and 1.07 (95% CI 0.99–1.15), respectively. No significant difference was observed between MOI and parasite density (Spearman rank correlation 0.198, p = 0.61; Fig. 2) or MOI and age (Spearman rank correlation 0.019, p = 0.86). The heterozygosity index was 0.82 for msp-1, 0.62 for msp-2 and 0.20 for glurp.
Fig. 2
Fig. 2

Relationship between geometric mean parasite density and multiplicity of P. falciparum infection

Discussion

Transmission intensity can affect the genetic diversity of the parasite population. Studies comparing areas of different transmission intensities of P. falciparum observe that genetic diversity is more diverse in areas of high transmission [28, 29]. Furthermore, studies in high transmission areas in Africa have shown that following enhanced malaria control interventions, genetic diversity reduces as transmission declines [10]. Therefore, understanding of the genetic structure of a parasite population can complement the implementation of malaria control interventions. No study has been conducted previously in Ethiopia using three polymorphic antigen markers, and the present study provides the most detailed assessment of genetic diversity and multiplicity of infection of P. falciparum isolates from Northwest Ethiopia. As Ethiopia moves towards malaria elimination, analysing the genotypes circulating along the border area is likely to be beneficial for ongoing evaluation of malaria control interventions and in understanding parasite dynamics related to imported cases.

Genotyping of msp-1 and msp-2 identified a higher diversity of alleles than glurp. This is in line with previous reports [30, 31]. Of the three allelic families of the msp-1 gene, MAD20 was the predominant allelic type, similar to reports from Indonesia [32], Malaysia [33] and Sudan [34]. In contrast, in isolates from Southwest Ethiopia [15], Côte d’Ivoire and Gabon [35], K1 was the most prevalent allelic family. Variations in the prevalence of block 2 alleles between different studies likely reflect differences in geographic locations and local transmission intensity [35, 36], in a gene that is highly polymorphic and has a dynamic genetic structure that can reflect transmission pressures [37]. Allele typing of msp-2 showed that the frequency of FC27 and IC/3D7 allelic families was nearly identical among the isolates; similar to findings from a study in Cambodia [24]. In agreement with previous reports [12, 38], the RII region of the glurp gene was also polymorphic, with nine distinct allelic fragment sizes detected.

Genetic diversity values were high according to the heterozygosity index for msp-1 and moderate for msp-2. Similar genetic diversity was identified for these genes in P. falciparum isolates in Southwest Ethiopia from 2008 [15]. In Djibouti, a neighboring country to Ethiopia, an initially moderate level of genetic diversity declined over an 11-year period to the point that expected heterozygosity reached zero in 2009 consistent with very low diversity [39].

The present study found that nearly three-quarters of the isolates harboured multiple genotypes, with about one-quarter monoclonal. This is a similar finding to a previous study from Northwest Ethiopia that only analysed msp-2 [16]. However, it is a significantly higher proportion with multiple clones than many of the locations sampled by the International Centers of Excellence for Malaria Research [9].

Population genetic studies have shown that MOI in the human population can be a proxy for transmission intensity. However, transmission intensity can also be affected by other factors such as vector biting behaviour and endemicity [9]. Inferring high transmission intensity from the presence of multiclonal infections alone has additional limitations including estimates of MOI varying by genotyping method, potential impact from sampling frequency and a non-linear relationship between MOI and transmission intensity [9]. Despite these limitations, the high levels of mixed infection in the present study, combined with evidence of moderate to high genetic diversity would be consistent with high transmission intensity in the study area. This is further supported by the presence of a high prevalence of malaria in screened patients during the study period (67%) consistent with malaria being highly endemic [20]. It is also compatible with reports from studies of African countries with intense malaria transmission in Cameroon, and Tanzania [40, 41].

High genetic diversity and MOI are evident in the present study despite the scale-up of malaria control efforts in Ethiopia. These findings are similar to reports from Sudan [11], western Kenya [42], northeastern Myanmar [43] and Nigeria [38]. Persistent genetic diversity likely reflects in part the ongoing high transmission intensity that exists in this region. While the results contrast with declining rates of genetic diversity and MOI in Djibouti and Thailand, these locations also had a reduction in malaria transmission [7, 39].

MOI has been correlated with parasite density in a number of studies, including in Congo, Brazzaville and West Uganda [26, 44]. However, similar to a study in south Benin, there was no association between MOI and parasite density in the present study [45]. This may have been due to the small number of isolates analysed. Similarly, the relationship between MOI and age remains unclear. The present study found no association between MOI and patients’ age, in agreement with studies conducted in south Benin and Senegal [45, 46], but in contrast to Central Sudan [47]. This variation may relate to differences in endemicity and the development antiparasite specific immunity. For example, there may be no association with MOI and age in regions of mesoendemicity such as the present study where immunity is similar across all ages, while there is an association in regions with intense transmission where immunity develops with age [46, 48, 49].

There is also the possibility that seasonal migration of individuals into and out of Humera contributed to the MOI and genetic diversity. Parasite gene flux mediated by human migration events is recognized to be a possible hindrance to malaria control interventions [50]. However, the current study was unable to investigate this in detail due to limits to the genotyping technique used in our study. To better understand the contribution of migration and malaria control interventions to malaria control in Ethiopia further studies on the genetic structure and diversity of P. falciparum in Ethiopia are needed, including across wider geographical area. In addition, use of microsatellite sequences, single nucleotide polymorphisms (SNPs) or whole-genome sequencing would provide improved insights into parasite transmission dynamics [8, 10].

Genotyping by size polymorphism is limited by processes that may lead to an inability to differentiate unique allelic fragments. Fragment size polymorphism of msp-1 is under positive natural selection and alleles may converge at the population level, with fragments of the same or similar size having different sequences [13, 14]. These events may lead to an underestimation of MOI and genetic diversity, and limit the generalizability of results to other settings. However, convergence at a population level does not prevent comparison within the same population at an alternative time period, such as to assess the impact of interventions.

Conclusions

This study reveals high genetic diversity and multiple infections in P. falciparum isolates from Northwest Ethiopia and is comparable to similar reports from other high transmission areas. The human population events occurring in this region may also contribute to this diversity and provide another challenge for malaria control efforts. These results suggest that additional strengthening of malaria control efforts is required. This information will serve as baseline data for future studies on dynamics of parasite transmission, and for evaluation of the effect of malaria control interventions along the Northwest border of Ethiopia.

Abbreviations

bp: 

basepairs

glurp

glutamate rich protein

MOI: 

multiplicity of infection

msp-1

merozoite surface protein1

msp-2

merozoite surface protein 2

PCR: 

polymerase chain reaction

Declarations

Authors' contributions

HM was involved in all phases of the study, Data collection, molecular analysis, data analysis, interpretation, and write up, AA and MK design the study and data collection, GT was involved in statistical analysis of data, RJC and KM contributed to write up and revised the manuscript. All authors read and approved the final manuscript.

Acknowledgements

We would like to thank the staff of Humera Health Center and the study participants and also the International Atomic Energy Agency (IAEA) for assisting with molecular analysis. We would like to acknowledge Haven Sime for assistance with the statistical work. In addition, we thank Dr Eugene W Liu for his valuable ideas and comments on the manuscript.

Competing interests

The authors declare that they have no competing interests.

Availability of data and materials

The dataset supporting the conclusion of this article is included within the article and the additional files.

Consent for publication

Not applicable.

Data availability statement

All relevant data are within the paper.

Ethics approval and consent to participate

Ethical approval for the study was obtained from the Scientific and Ethical Review Office (SERO) of the Ethiopian Public Health Institute (EPHI). Written informed consent was obtained from parents or guardian prior to recruitment.

Funding

Funding partially was obtained from Ethiopia Federal Ministry of Health (FMoH). Funding agency did not play a role in the design of the study, collection of sample, analysis, and interpretation of the data and writing of manuscript.

Publisher’s Note

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Authors’ Affiliations

(1)
Malaria, Neglected Tropical Diseases Research Team Bacterial, Parasitic, Zoonotic Diseases Research Directorate, Ethiopian Public Health Institute, Addis Ababa, Ethiopia
(2)
Menzies School of Health Research and Charles Darwin University, Darwin, Australia

References

  1. Federal Democratic Republic of Ethiopia, Ministry of Health. Health sector transformation plan. Addis Ababa. 2015/16–2019/20.Google Scholar
  2. Abeku TA, Helinski ME, Kirby MJ, Kefyalew T, Awano T, Batisso E, et al. Monitoring changes in malaria epidemiology and effectiveness of interventions in Ethiopia and Uganda: beyond Garki project baseline survey. Malar J. 2015;14:337.View ArticleGoogle Scholar
  3. Aregawi M, Lynch M, Bekele W, Kebede H, Jima D, Taffese HS, et al. Time series analysis of trends in malaria cases and deaths at hospitals and the effect of antimalaria interventions, 2001–2011, Ethiopia. PLoS ONE. 2014;9:e106359.View ArticleGoogle Scholar
  4. Federal Ministry of Health Ethiopia. HSDP IV Annual Performance Report EFY 2006 (2013–2014). Federal Ministry of Health; 2014.Google Scholar
  5. Deribew A, Tessema GA, Deribe K, Melaku YA, Lakew Y, Amare AT, et al. Trends, causes, and risk factors of mortality among children under five in Ethiopia, 1990–2013: findings from the Global Burden of Diseases Study 2013. Popul Health Metr. 2016;14:42.View ArticleGoogle Scholar
  6. Nabet C, Doumbo S, Jeddi F, Konaté S, Manciulli T, Fofana B, et al. Genetic diversity of Plasmodium falciparum in human malaria cases in Mali. Malar J. 2016;15:353.View ArticleGoogle Scholar
  7. Nkhoma SC, Nair S, Al-saai S, Ashley E, McGready R, Phyo AP, et al. Population genetics correlates of declining transmission in human pathogen. Mol Ecol. 2013;22:273–85.View ArticleGoogle Scholar
  8. Auburn S, Barry AE. Dissecting malaria biology and epidemiology using population genetics and genomics. Int J Parasitology. 2017;47:77–85.View ArticleGoogle Scholar
  9. Escalante AA, Ferreira MU, Vinetz JM, Volkman SK, Cui L, Gamboa D, et al. Malaria molecular epidemiology: lessons from the International Centers of Excellence for Malaria Research Network. Am J Trop Med Hyg. 2015;93(Suppl 3):79–86.View ArticleGoogle Scholar
  10. Daniels R, Chang HH, Séne PD, Park DC, Neafsey DE, Schaffner SF, et al. Genetic surveillance detects both clonal and epidemic transmission of malaria following enhanced intervention in Senegal. PLoS ONE. 2013;8:e60780.View ArticleGoogle Scholar
  11. Bakhiet AM, Abdel-Muhsin AM, Elzaki SE, Al-Hashami Z, Albarwani HS, Al Qamashoui BA, et al. Plasmodium falciparum population structure in Sudan post artemisinin-based combination therapy. Acta Trop. 2015;148:97–104.View ArticleGoogle Scholar
  12. Mwingira F, Nkwengulila G, Schoepflin S, Sumari D, Beck HP, Snounou G, et al. Plasmodium falciparum msp1, msp2 and glurp allele frequency and diversity in sub-Saharan Africa. Malar J. 2011;10:79.View ArticleGoogle Scholar
  13. Takala SL, Escalante AA, Branch OH, Kariuki S, Biswas S, Chaiyaroj SC, et al. Genetic diversity in the Block 2 region of the merozoite surface protein 1 (MSP-1) of Plasmodium falciparum: additional complexity and selection and convergence in fragment size polymorphism. Infect Genet Evol. 2006;6:417–24.View ArticleGoogle Scholar
  14. Ferreira MU, Hartl DL. Plasmodium falciparum: worldwide sequence diversity and evolution of the malaria vaccine candidate merozoite surface protein-2 (MSP-2). Exp Parasitol. 2007;115:32–40.View ArticleGoogle Scholar
  15. Mohammed H, Mindaye T, Belayneh M, Kassa M, Assefa A, Tadesse M, et al. Genetic diversity of Plasmodium falciparum isolates based on MSP-1 and MSP-2 genes from Kolla-Shele area, Arbaminch Zuria District, southwest Ethiopia. Malar J. 2015;14:73.View ArticleGoogle Scholar
  16. Mohammed H, Kassa M, Assefa A, Tadesse M, Kebede A. Genetic polymorphism of Merozoite Surface Protein-2 (MSP-2) in Plasmodium falciparum isolates from Pawe District, North West Ethiopia. PLoS ONE. 2017;12:e0177559.View ArticleGoogle Scholar
  17. Federal Ministry of Health Ethiopia (FMoH). National Strategic plan for malaria prevention, control and elimination in Ethiopia: 2014–2020. Addis Ababa: FMoH; 2014.Google Scholar
  18. Wezam A. Malaria survey at Humera, northwestern Ethiopia. Ethiop Med J. 1994;32:41–7.PubMedGoogle Scholar
  19. Mengesha T, Tsegaye Y, Hailu Y. The epidemiology of malaria in Humera, Northwest Ethiopia. Ethiop J Health Sci. 2000;10:137–43.Google Scholar
  20. Teklemariam M, Assefa A, Kassa M, Mohammed H, Mamo H. Therapeutic efficacy of artemether-lumefantrine against uncomplicated Plasmodium falciparum malaria in a high transmission area in northwest Ethiopia. PLoS ONE. 2017;12:e0176004.View ArticleGoogle Scholar
  21. Plowe CV, Djimde A, Bouare M, Doumbo O, Wellems TE. Pyrimethamine and proguanil resistance-conferring mutations in Plasmodium falciparum dihydrofolate reductase: polymerase chain reaction methods for surveillance in Africa. Am J Trop Med Hyg. 1995;52:565–8.View ArticleGoogle Scholar
  22. Snounou G. Genotyping of Plasmodium spp. Nested PCR. Methods Mol Med. 2002;72:103–16.PubMedGoogle Scholar
  23. Ntoumi F, Ngoundou-Landji J, Lekoulou F, Luty A, Deloron P, Ringwald P. Site based study on polymorphism of Plasmodium falciparum msp-1 and msp-2 genes in isolates from two villages in Central Africa. Parasitology. 2000;42:197–203.Google Scholar
  24. Gosi P, Lanteri CA, Tyner SD, Se Y, Lon C, Spring M, et al. Evaluation of parasite subpopulations and genetic diversity of msp1, msp2 and glurp genes during and following artesunate mono therapy treatment of Plasmodium falciparum malaria in Western Cambodia. Malar J. 2013;12:403.View ArticleGoogle Scholar
  25. Kiwuwa MS, Ribacke U, Moll K, Byarugaba J, Lundblom K, Farnert A, et al. Genetic diversity of Plasmodium falciparum infections in mild and severe malaria of children from Kampala, Uganda. Parasitol Res. 2013;112:169–70.View ArticleGoogle Scholar
  26. Mayengue PL, Ndounga M, Malonga FV, Bitemo M, Ntoumi F. Genetic polymorphism of merozoite surface protein-1 and merozoite surface polymorphism of merozoite surface protein-1 and merozoite surface protein-2 in Plasmodium falciparum isolates from Brazzaville, Republic of Congo. Malar J. 2011;10:276.View ArticleGoogle Scholar
  27. Nei M. Estimation of average heterozygosity and genetic distance from a small number of individuals. Genetics. 1978;89:583–90.PubMedPubMed CentralGoogle Scholar
  28. Bogreau H, Renaud F, Bouchiba H, Durand P, Assi S, Henry M, et al. Genetic diversity and structure of Africa Plasmodium falciparum in urban and rural areas. Am J Trop Hyg. 2006;74:953–9.View ArticleGoogle Scholar
  29. Mobegi VA, Loua KM, Ahouidi AD, Satoguina J, Nwanma DC, Amambua-Ngwa A, et al. Population genetic structure of Plasmodium falciparum across a region of diverse endemicity in West Africa. Malar J. 2012;11:223.View ArticleGoogle Scholar
  30. Congpuong K, Sukaram R, Prompan Y, Dornae A. Genetic diversity of the msp1, msp2 and glurp genes of Plasmodium falciparum isolates along the Thai-Myanmar borders. Asia Pac J Trop Biomed. 2014;4:598–602.View ArticleGoogle Scholar
  31. Soe TN, Wu Y, Tun MW, Xu X, Hu Y, Ruan Y, et al. Genetic diversity of Plasmodium falciparum populations in southeast and western Myanmar. Parasit Vectors. 2017;10:322.View ArticleGoogle Scholar
  32. Sorontou Y, Pakpahan A. Genetic diversity in MSP-1 gene of Plasmodium falciparum and its association with malaria severity, parasite density, and host factors of asymptomatic and symptomatic patients in Papua, Indonesia. Int J Med Pub Health. 2015;4:1584.View ArticleGoogle Scholar
  33. Mohd Abd Razak MR, Sastu UR, Norahmad NA, Abdul-Karim A, Muhammad A, Muniandy PK, et al. Genetic diversity of Plasmodium falciparum populations in malaria declining areas of Sabah, East Malaysia. PLoS ONE. 2016;11:e0152415.View ArticleGoogle Scholar
  34. Hamid MMA, Elamin AF, Albsheer MM, Abdella AA, Mustafa SO, Muneer MS, et al. Multiplicity of infection and genetic diversity of Plasmodium falciparum isolates from patients with uncomplicated and sever malaria in Gezira State, Sudan. Parasit Vectors. 2016;9:362.View ArticleGoogle Scholar
  35. Yavo W, Konaté A, Mawili-Mboumba DP, Kassi FK, Tshibola-Mbuyi ML, Angora EK, et al. Genetic polymorphism of msp1 and msp2 in Plasmodium falciparum isolates from Côte d’Ivoire versus Gabon. J Parasitol Res. 2016;2016:3074803.View ArticleGoogle Scholar
  36. Farnert A, Lebbad M, Faraja L, Rooth I. Extensive dynamics of Plasmodium falciparum densities, stages and genotyping profiles. Malar J. 2008;7:241.View ArticleGoogle Scholar
  37. Bharti PK, Shukla MM, Sharma YD, Singh N. Genetic diversity in the block 2 region of the merozoite surface protein 1 of Plasmodium falciparum in central India. Malar J. 2012;11:78.View ArticleGoogle Scholar
  38. Funwei RI, Thomas BN, Falade CO, Ojurongbe O. Extensive diversity in the allelic frequency of Plasmodium falciparum merozoite surface proteins and glutamate-rich protein in rural and urban settings of southwestern Nigeria. Malar J. 2018;17:1.View ArticleGoogle Scholar
  39. Khaireh BA, Assefa A, Guessod HH, Basco LK, Khaireh MA, Pasqual A, et al. Population genetics analysis during the elimination process of Plasmodium falciparum in Djibouti. Malar J. 2013;12:201.View ArticleGoogle Scholar
  40. Basco LK, Ringwald P. Molecular epidemiology of malaria in Yaounde, Cameroon. VIII. Multiple Plasmodium falciparum infections in symptomatic patients. Am J Trop Med Hyg. 2001;65:798–803.View ArticleGoogle Scholar
  41. Magesa SM, Mdira KY, Babiker HA, Alifrangis M, Farnert A, Simonsen PE, et al. Diversity of Plasmodium falciparum clones infecting children living in a holoendemic area in north-eastern Tanzania. Acta Trop. 2002;84:83–92.View ArticleGoogle Scholar
  42. Vardo-Zalik AM, Zhou G, Zhong D, Afrane YA, Githeko AK, Yan G. Alteration in Plasmodium falciparum genetic structure two years after increased malaria control efforts in western Kenya. Am J Trop Med Hyg. 2013;88:29–36.View ArticleGoogle Scholar
  43. Yuan L, Zhao H, Wu L, Li X, Parker D, Xu S, et al. Plasmodium falciparum populations from northeastern Myanmar display high levels of genetic diversity at multiple antigenic loci. Acta Trop. 2013;125:53–9.View ArticleGoogle Scholar
  44. Peyerl-Hoffmann G, Jelinek T, Kilian A, Kabagambe G, Metzger WG, von Sonnenburg F. Genetic diversity of Plasmodium falciparum and its relationship to parasite density in an area with different malaria endemicities in West Uganda. Trop Med Int Health. 2001;6:607–13.View ArticleGoogle Scholar
  45. Ogouye’mi-Hounto A, Gazard DK, Ndam N, Topanou E, Garba O, Elegbe P, et al. Genetic polymorphism of merozoite surface protein-1 and merozoite surface protein-2 in Plasmodium falciparum isolates from children in South of Benin. Parasite. 2013;20:37.View ArticleGoogle Scholar
  46. Vafa M, Troye-Blomberg A, Anchang J, Garcia A, Migot-Nabias F. Multiplicity of Plasmodium falciparum infection in asymptomatic in children in Senegal in relation to transmission, age and erythrocyte variants. Malar J. 2008;7:17.View ArticleGoogle Scholar
  47. Hamid MM, Mohammed SB, El Hassan IM. Genetic diversity of Plasmodium falciparum field isolates in Central Sudan inferred by PCR genotyping of merozoite surface protein 1 and 2. N Am J Med Sci. 2013;5:95–101.View ArticleGoogle Scholar
  48. Ntoumi F, Contamin H, Rogier C, Bonnefoy S, Trape JF, Mercereau-Puijalon O. Age-dependent carriage of multiple Plasmodium falciparum merozoite surface antigen-2 alleles in asymptomatic malaria infections. Am J Trop Med Hyg. 1995;52:81–8.View ArticleGoogle Scholar
  49. Baird JK. Host age as a determinant of naturally acquired immunity to Plasmodium falciparum. Parasitol Today. 1995;11:105–11.View ArticleGoogle Scholar
  50. Schultz L, Wapling J, Mueller I, Ntsuke PO, Senn N, Nale J, et al. Multilocus haplotypes reveal variable levels of diversity and population structure of Plasmodium falciparum in Papua New Guinea, a region of intense perennial transmission. Malar J. 2010;9:336.View ArticleGoogle Scholar

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