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Diagnosis of an imported Plasmodium ovale wallikeri infection in Malaysia

Abstract

Plasmodium ovale is rare and not exactly known to be autochthonous in Malaysia. There are two distinct forms of the parasite, namely P. ovale curtisi (classic form) and P. ovale wallikeri (variant form). Here, the first sequence confirmed case of an imported P. ovale wallikeri infection in Malaysia is presented. Microscopy found Plasmodium parasites with morphology similar to P. ovale or Plasmodium vivax in the blood films. Further confirmation using polymerase chain reaction (PCR) targeting the small-subunit rRNA gene of the parasite was unsuccessful. Genus-specific PCR was then performed and the product was sequenced and analysed. Sequence analyses confirmed the aetiological agent as P. ovale wallikeri. New species-specific primers (rOVA1v and rOVA2v) were employed and P. ovale wallikeri was finally confirmed. The findings highlight the need to look out for imported malaria infections in Malaysia and the importance of a constantly updated and validated diagnostic technique.

Background

Malaria is caused by the blood parasite Plasmodium. Plasmodium falciparum, Plasmodium vivax, Plasmodium ovale curtisi, P. ovale wallikeri, Plasmodium knowlesi and Plasmodium malariae are known to infect humans. Current molecular-based diagnostic methods enable sensitive and specific detection of the five human malaria parasites, even in subclinical cases. Improved diagnostic techniques using polymerase chain reaction (PCR) detected a spike in prevalence of overall malaria infections. The relatively insensitive microscopic diagnosis has underestimated the prevalence of this disease, including P. ovale infection, which was once believed to be comparatively rare. Review of a series of studies led to a probable conclusion that a 2 to >10 % prevalence of P. ovale might actually exist in the general population of Africa and Papua New Guinea and among malaria patients in Southeast Asia [1].

Plasmodium ovale infection, a tertian malaria, is difficult to diagnose microscopically, owing to the generally low parasite density in patients and the parasite’s morphology which resembles that of P. vivax. Additionally, it is a relapsing infection, which can occur long after the primary exposure to the parasite, initiated by latent parasites (hypnozoites) residing in the liver [2]. Moreover, dimorphism exists in the small-subunit rRNA (ssrRNA) gene of the parasite, causing some isolates to be undetectable by PCR but microscopically confirmed as P. ovale [3]. Further gene studies demonstrated two distinct, non-recombining sympatric species of the parasite [4]. Subsequently in 2010, Sutherland et al. [4] first coined P. ovale curtisi and P. ovale wallikeri as names for the classic and variant forms of P.ovale, respectively.

Hitherto, cases of P. ovale wallikeri infection have been described in certain countries in Southern Asia (e.g. Bangladesh and India) and almost throughout the whole of Southeast Asia [414]. In Malaysia currently, the most prevalent malaria parasite is P. knowlesi [15], with majority of the cases originating from Malaysian Borneo. Seven known cases of P. ovale were reported so far in Malaysia [1518]. Here, the first sequence confirmed case of an imported P. ovale wallikeri infection in a patient in Malaysia is reported. Microscopy, nested PCR and sequence analyses of the ssrRNA gene confirmed the aetiological agent as P. ovale wallikeri.

Case presentation

A 19-year-old, Nigerian college student presented to Sunway Medical Centre, Selangor, Malaysia with a 4-day history of fever associated with chills, rigors and body ache. Prior to onset of symptoms, he had gone back to Nigeria for 10 days during semester break and became unwell 5 days after returning to Malaysia. He was febrile upon admission with body temperature of 39.8 °C, pulse rate of 126 beats per minute and blood pressure of 128/87 mm Hg. There were no other significant physical findings noted. He recalled to have had three episodes of malaria during childhood, but was uncertain about the causative Plasmodium species. Blood investigation showed thrombocytopaenia with a platelet count of 71,000 per microlitre (normal: 150,000–400,000 per microlitre) and raised C-reactive protein (97 mg/L; normal: <5 mg/L). White blood cell count, haemoglobin and albumin levels were within the normal range. Dengue NS-1Ag, dengue IgM and IgG, Leptospira IgM, Mycoplasma antibody test and Widal-Weil-Felix test were all negative. Blood cultures did not yield any result.

After three attempts using BinaxNOW® Malaria Test (USA), a T2 Line appeared, while no T1 Line (specific for P. falciparum infection) was observed, suggesting vivax, malariae or ovale malaria or a mix of these. Microscopy on thick and thin blood films detected the presence of malaria parasites suggesting P. ovale or P. vivax (Fig. 1), with 0.27 % parasitaemia.

Fig. 1
figure1

Microphotographs of giemsa-stained thin blood films of the patient viewed under 1000 ×  magnification. a Developing schizont. b A schizont with eight merozoites. c, d Gametocyte. Infected red blood cell is enlarged, oval in shape with presence of Schuffner’s dots, clearly seen in b and d

DNA was extracted from whole blood collected in EDTA tube using the DNeasy® Blood and Tissue Kit (Qiagen, Germany). Four microlitres of the purified DNA was used in the primary PCR reaction, followed by a secondary PCR amplification using standard nested PCR method [16, 19] (Table 1). The PCR result was negative for all reactions except the reaction using genus-specific primers, rPLU3 and rPLU4. Gel electrophoresis showed a band of 240 bp, corresponding to the product of the genus-specific nest 2 PCR (Fig. 2). At the same time, NM-PCR, a nested multiplex malaria PCR and NG-PCR, a nested PCR for Plasmodium genus amplification were performed (Table 1), as previously described [20]. NG-PCR also successfully amplified a positive product. The positive products of both PCRs were gel purified using QIAquick® Gel Extraction Kit (Qiagen, Germany) and cloned into pGEM®-T vector (Promega, USA). For each PCR product, ten clones were screened and three positive clones were randomly selected for plasmid sequencing. Plasmids were extracted using QIAprep® Spin Miniprep Kit (Qiagen, Germany) and sequenced using BigDye® Terminator v3.1 in ABI PRISM® 3730xl DNA Analyzer (Applied Biosystems). No definitive result was obtained from NM-PCR due to non-specific bands observed on the gel.

Table 1 Description of PCR protocols used in this report
Fig. 2
figure2

2 % agarose gel electrophoresis of Nest 2 PCR showing an amplified product with the genus-specific primers. 1 100 bp DNA ladder; 2 rFAL1/rFAL2 (P. falciparum); 3 rOVA1/rOVA2 (P. ovale); 4 rMAL1/rMAL2 (P. malariae); 5 rVIV1/rVIV2 (P. vivax); 6 Pmk8/Pmkr9 (P. knowlesi); 7 rPLU3/rPLU4 (Plasmodium spp.); 8–13 no template control of P. falciparum, P. ovale, P. malariae, P. vivax, P. knowlesi, and Plasmodium spp., respectively

Sequencing data between clones were similar except for a few nucleotide differences. A consensus sequence was generated from the plasmid sequences of the clones for each PCR product and analysed using NCBI BLAST [21]. The result showed a 99 % identity to the ssrRNA gene of P. ovale wallikeri (GenBank accession number: AB182492.1, KF696360.1, KF018654.1). Subsequently, the full nucleotide sequence (746 bp) of the product from NG-PCR (herein named UM00134; GenBank accession number: KU255080) was compared to those found in the GenBank in a phylogenetic analysis using the MEGA 6.06 program [22]. Sequences were trimmed and aligned using Clustal W [23]. A phylogenetic tree was constructed using the neighbour-joining methods [24] and Jukes-Cantor model [25], with a Bootstrap value of 1000 (Fig. 3). Sequence analyses confirmed that the infecting Plasmodium species was P. ovale wallikeri.

Fig. 3
figure3

Phylogenetic analysis of the NG-PCR product (UM00134). The phylogenetic tree is constructed using the Neighbor-Joining methods and Jukes–Cantor model, with Bootstrap value of 1000. The patient isolate, UM00134 is clustered with P. ovale wallikeri isolates. GenBank accession number is given after each isolate’s name

In light of this finding, primers rOVA1v and rOVA2v which are specific for P. ovale wallikeri [3], were used in the Nest 2 PCR reaction under the same condition as mentioned in Table 1. Primers rOVA1 and rOVA2 were included to exclude P. ovale curtisi infection. Parallel to that, a mixture of primer sets rOVA1/rOVA2 and rOVA1v/rOVA2v, besides primer set rOVA1WC/rOVA2WC [26] which are able to detect both P. ovale forms were also employed. Positive products were obtained from the PCR. The mixture of these primer sets in a single Nest 2 PCR reaction and primer set rOVA1WC/rOVA2WC were able to detect P. ovale wallikeri (Fig. 4).

Fig. 4
figure4

Detection of P. ovale wallikeri using primer sets rOVA1/rOVA2, rOVA1v/rOVA2v, mixture of both primer sets and rOVA1WC/rOVA2WC. A 2 % agarose gel electrophoresis was performed. Parasite DNA purified from patient blood is used as template of PCR. 1 100 bp DNA ladder; 2 rOVA1/rOVA2 (P. ovale curtisi); 3 rOVA1v/rOVA2v (P. ovale wallikeri); 4 Mixture of primer sets rOVA1/rOVA2 and rOVA1v/rOVA2v (both forms of P. ovale); 5 rOVA1WC/rOVA2WC (both forms of P. ovale)

The patient was immediately treated with a course of Riamet® (artemether/lumefantrine) following detection of malaria parasites. His symptoms improved within 24 h of treatment but blood film for malaria became negative only after 36 h of treatment. However his platelet count seems to be slow to recover while C-reactive protein, which is known as a marker for severity in malaria [27], improved steadily following treatment. Primaquine 30 mg base daily was added 2 days after Riamet. He requested for discharge and agreed to complete the two-week course of primaquine at home. He continued to improve clinically post-discharge but could not afford to repeat his blood tests and dropped out from subsequent out-patient follow up visit.

Consent

The study was approved by the University of Malaya Medical Centre Medical Ethics Committee (MEC Ref. No: 817.18).

Discussion

In Malaysia, two of the seven ovale malaria were reported to be caused by P. ovale curtisi [18]. No known ovale infection in the country was sequence-confirmed to be caused by P. ovale wallikeri, up till now. Diagnosis of ovale malaria is a challenge, due to the parasite’s low density and close morphological resemblance to P. vivax. Both the classic and variant forms of P. ovale are also morphologically indistinguishable from each other [26]. Rapid diagnostic tests (RDT) have aided in the rapid diagnosis of malaria and other infectious diseases. Nonetheless, their apparent ineffectiveness in detecting P. ovale turns out to be well documented [28, 29]. In this case, the result of the RDT, BinaxNOW® Malaria Test was negative twice before a faint line indicating Plasmodium species infection appeared on the third attempt.

Nested PCR for molecular detection of Plasmodium spp. [30] has emerged as a standard molecular method for malaria diagnosis. However, the primers for P. ovale detection (rOVA1/rOVA2) were unable to identify the variant form of the parasite, until a new set of primers (rOVA1v/rOVA2v) specific for P. ovale wallikeri and a set of primers (rOVA1WC/rOVA2WC) to detect both forms were introduced [3, 26]. The initial negative PCR result using the species-specific primers and subsequent sequencing analyses were indicative of P. ovale wallikeri infection, prompting the use of these new primers. Besides, primer sets rOVA1/rOVA2 and rOVA1v/rOVA2v were mixed to detect both P. ovale wallikeri and P. ovale curtisi in a single Nest 2 duplex PCR reaction. The mixed primers and primer set rOVA1WC/rOVA2WC in the PCR reaction appeared to be a mean for quick and cost-efficient detection of both species of P. ovale [26], and therefore should replace primers rOVA1/rOVA2 for routine diagnosis of malaria.

The accurate diagnosis of P. ovale infection, in fact of all malaria infection, is crucial to avoid the delay of treatment and clinical complications. Though ovale malaria is thought to be rather benign, associated severe complications such as acute respiratory distress syndrome (ARDS) [31, 32], splenic complication [33], acute renal failure and ultimately, death [18, 34] have been reported. There are certain clinical features slightly distinctive of the two different forms of P. ovale. The latency periods of P. ovale curtisi and P. ovale wallikeri infection are reported to be 66.1–111.1 days and 28.9–57 days, respectively, with one case of P. ovale curtisi infection displaying an extraordinarily long latency period of 1083 days [35]. This shorter latency period may lead to higher relapse rate of P. ovale wallikeri infection. A trend toward a shorter stay in Africa and shorter period of time between onset of symptoms and diagnosis was found among patients with P. ovale wallikeri infection, possibly reflecting easier transmission, shorter latency or higher relapse rates [6]. In addition, patients with P. ovale wallikeri infection have significantly more severe thrombocytopaenia and relatively higher parasitaemia than those with P. ovale curtisi infection. Other non-significant, differentiating features include shorter pre-patent period, lower albumin level, higher body temperature and more markers of haemolysis in P. ovale wallikeri infection compared to that of P. ovale curtisi [6]. Taken together, it may seem that management of P. ovale wallikeri could be slightly more complicated than P. ovale curtisi.

Plasmodium ovale is not exactly known to be autochthonous in Malaysia. It is absolutely undesirable for P. ovale to be transmitting within the country, especially when Malaysia is progressing towards elimination of malaria by 2020. Relapsing ovale infection is often asymptomatic, detected only by continued examination of blood films [2]. In other words, human reservoir of P. ovale may stay under the radar. This poses a threat to the public health because natural transmission of ovale malaria in Malaysia is possible in view of the availability of two vectors, Anopheles maculatus [36] and Anopheles dirus [37] which have been shown to be good experimental vectors for P. ovale. Nolder et al. [35] also found that, compared to other human malaria, ovale malaria is less likely to be prevented by chemoprophylaxis. Furthermore, as pointed out by Mellon et al. [38], with non-specific clinical signs as well as long latency period of P. ovale infection [2, 6, 35], what then should the maximum exclusion period be for blood donors who had travelled to endemic areas? Transfusion-transmitted P. ovale infection had been reported and can be severe [39].

It was not discernable if the patient was experiencing a relapse or acute malaria. Prepatent period (time between sporozoite inoculation and the first detection of parasites in blood) for ovale malaria is reported to be 12–20 days [2]. Lastly, a similar case was reported by Li et al. [29], whereby P. ovale wallikeri infection was diagnosed in a Chinese worker returning from West Africa. This and other increasing worldwide reports of P. ovale infections [4043] and misdiagnosed cases [7] urge the health and research sectors to devise and utilise accurate techniques to diagnose this infectious disease.

Conclusions

The current findings highlight the need for continuously updating and validating diagnostic techniques for malaria. Complete history taking is of utmost importance in patients as it aids diagnosis, especially in the case of P. ovale infection where it can remain latent and asymptomatic for a long period of time. Imported cases of malaria are a concern for public health, especially in countries where malaria is non-existent or has been eliminated. With Malaysia’s open policy and the ease of travel, healthcare personnel should be made aware of the possible imported infections entering the country.

References

  1. 1.

    Mueller I, Zimmerman PA, Reeder JC. Plasmodium malariae and Plasmodium ovale–the “bashful” malaria parasites. Trends Parasitol. 2007;23:278–83. doi:10.1016/j.pt.2007.04.009.

    PubMed  CAS  PubMed Central  Article  Google Scholar 

  2. 2.

    Collins WE, Jeffery GM. Plasmodium ovale: parasite and disease. Clin Microbiol Rev. 2005;18:570–81. doi:10.1128/cmr.18.3.570-581.2005.

    PubMed  PubMed Central  Article  Google Scholar 

  3. 3.

    Calderaro A, Piccolo G, Perandin F, Gorrini C, Peruzzi S, Zuelli C, et al. Genetic polymorphisms influence Plasmodium ovale PCR detection accuracy. J Clin Microbiol. 2007;45:1624–7. doi:10.1128/jcm.02316-06.

    PubMed  CAS  PubMed Central  Article  Google Scholar 

  4. 4.

    Sutherland CJ, Tanomsing N, Nolder D, Oguike M, Jennison C, Pukrittayakamee S, et al. Two nonrecombining sympatric forms of the human malaria parasite Plasmodium ovale occur globally. J Infect Dis. 2010;201:1544–50. doi:10.1086/652240.

    PubMed  CAS  Article  Google Scholar 

  5. 5.

    Fuehrer HP, Habler VE, Fally MA, Harl J, Starzengruber P, Swoboda P, et al. Plasmodium ovale in Bangladesh: genetic diversity and the first known evidence of the sympatric distribution of Plasmodium ovale curtisi and Plasmodium ovale wallikeri in southern Asia. Int J Parasitol. 2012;42:693–9. doi:10.1016/j.ijpara.2012.04.015.

    PubMed  Article  Google Scholar 

  6. 6.

    Rojo-Marcos G, Rubio-Muñoz Jé M, Ramírez-Olivencia G, García-Bujalance S, Elcuaz-Romano R, Díaz-Menéndez M, et al. Comparison of imported Plasmodium ovale curtisi and P. ovale wallikeri infections among patients in Spain, 2005–2011. Emerg Infect Dis. 2014;20:409–16. doi:10.3201/eid2003.130745.

    PubMed  CAS  PubMed Central  Article  Google Scholar 

  7. 7.

    Chavatte J-M, Tan S, Snounou G, Lin R. Molecular characterization of misidentified Plasmodium ovale imported cases in Singapore. Malar J. 2015;14:454.

    PubMed  PubMed Central  Article  Google Scholar 

  8. 8.

    Incardona S, Chy S, Chiv L, Nhem S, Sem R, Hewitt S, et al. Large sequence heterogeneity of the small subunit ribosomal RNA gene of Plasmodium ovale in Cambodia. Am J Trop Med Hyg. 2005;72:719–24.

    PubMed  CAS  Google Scholar 

  9. 9.

    Toma H, Kobayashi J, Vannachone B, Arakawa T, Sato Y, Nambanya S, et al. Plasmodium ovale infections detected by PCR assay in Lao PDR. Southeast Asian J Trop Med Public Health. 1999;30:620–2.

    PubMed  CAS  Google Scholar 

  10. 10.

    Wickremasinghe R, Galapaththy GN, Fernando WA, de Monbrison F, Wijesinghe RS, Mendis KN, et al. An indigenous case of Plasmodium ovale infection in Sri Lanka. Am J Trop Med Hyg. 2008;78:206–7.

    PubMed  Google Scholar 

  11. 11.

    Win TT, Lin K, Mizuno S, Zhou M, Liu Q, Ferreira MU, et al. Wide distribution of Plasmodium ovale in Myanmar. Trop Med Int Health. 2002;7:231–9.

    PubMed  CAS  Article  Google Scholar 

  12. 12.

    Zhou M, Liu Q, Wongsrichanalai C, Suwonkerd W, Panart K, Prajakwong S, et al. High prevalence of Plasmodium malariae and Plasmodium ovale in malaria patients along the Thai-Myanmar border, as revealed by acridine orange staining and PCR-based diagnoses. Trop Med Int Health. 1998;3:304–12.

    PubMed  CAS  Article  Google Scholar 

  13. 13.

    Baird JK. Purnomo, Masbar S. Plasmodium ovale in Indonesia. Southeast Asian J Trop Med Public Health. 1990;21:541–4.

    PubMed  CAS  Google Scholar 

  14. 14.

    Cabrera BD, Arambulo PV 3rd. Malaria in the Republic of the Philippines: a review. Acta Trop. 1977;34:265–79.

    PubMed  CAS  Google Scholar 

  15. 15.

    Yusof R, Lau YL, Mahmud R, Fong MY, Jelip J, Ngian HU, et al. High proportion of knowlesi malaria in recent malaria cases in Malaysia. Malar J. 2014;13:168.

    PubMed  PubMed Central  Article  Google Scholar 

  16. 16.

    Singh B, Lee KS, Matusop A, Radhakrishnan A, Shamsul SSG, Cox-Singh J, et al. A large focus of naturally acquired Plasmodium knowlesi infections in human beings. Lancet. 2004;363:1017–24.

    PubMed  Article  Google Scholar 

  17. 17.

    Lim YAL, Mahmud R, Chew CH, T T, Chua KH. Plasmodium ovale infection in Malaysia: first imported case. Malar J. 2010;9:272. doi:10.1186/1475-2875-9-272.

    PubMed  PubMed Central  Article  Google Scholar 

  18. 18.

    Lau YL, Lee WC, Tan LH, Kamarulzaman A, Syed Omar SF, Fong MY, et al. Acute respiratory distress syndrome and acute renal failure from Plasmodium ovale infection with fatal outcome. Malar J. 2013;12:389. doi:10.1186/1475-2875-12-389.

    PubMed  PubMed Central  Article  Google Scholar 

  19. 19.

    Singh B, Bobogare A, Cox-Singh J, Snounou G, Abdullah MS, Rahman HA. A genus- and species-specific nested polymerase chain reaction malaria detection assay for epidemiologic studies. Am J Trop Med Hyg. 1999;60:687–92.

    PubMed  CAS  Google Scholar 

  20. 20.

    Ta TH, Hisam S, Lanza M, Jiram AI, Ismail N, Rubio JM. First case of a naturally acquired human infection with Plasmodium cynomolgi. Malar J. 2014;13:68. doi:10.1186/1475-2875-13-68.

    PubMed  PubMed Central  Article  Google Scholar 

  21. 21.

    Altschul SF, Gish W, Miller W, Myers EW, Lipman DJ. Basic local alignment search tool. J Mol Biol. 1990;215:403–10. doi:10.1016/s0022-2836(05)80360-2.

    PubMed  CAS  Article  Google Scholar 

  22. 22.

    Tamura K, Stecher G, Peterson D, Filipski A, Kumar S. MEGA6: molecular evolutionary genetics analysis version 6.0. Mol Biol Evol. 2013;30:2725–9. doi:10.1093/molbev/mst197.

    PubMed  CAS  PubMed Central  Article  Google Scholar 

  23. 23.

    Thompson JD, Higgins DG, Gibson TJ, Clustal W. Improving the sensitivity of progressive multiple sequence alignment through sequence weighting, position-specific gap penalties and weight matrix choice. Nucleic Acids Res. 1994;22:4673–80.

    PubMed  CAS  PubMed Central  Article  Google Scholar 

  24. 24.

    Saitou N, Nei M. The neighbor-joining method: a new method for reconstructing phylogenetic trees. Mol Biol Evol. 1987;4:406–25.

    PubMed  CAS  Google Scholar 

  25. 25.

    Jukes TH, Cantor CR. Evolution of protein molecules. In: Munro HN, editor. Mammalian protein metabolism III. New York: Academic Press; 1969. p. 21–132.

    Chapter  Google Scholar 

  26. 26.

    Fuehrer HP, Stadler MT, Buczolich K, Bloeschl I, Noedl H. Two techniques for simultaneous identification of Plasmodium ovale curtisi and Plasmodium ovale wallikeri by use of the small-subunit rRNA gene. J Clin Microbiol. 2012;50:4100–2. doi:10.1128/jcm.02180-12.

    PubMed  CAS  PubMed Central  Article  Google Scholar 

  27. 27.

    Paul R, Sinha PK, Bhattacharya R, Banerjee AK, Raychaudhuri P, Mondal J. Study of C reactive protein as a prognostic marker in malaria from Eastern India. Adv Biomed Res. 2012;1:41. doi:10.4103/2277-9175.100140.

    PubMed  PubMed Central  Article  Google Scholar 

  28. 28.

    Bauffe F, Desplans J, Fraisier C, Parzy D. Real-time PCR assay for discrimination of Plasmodium ovale curtisi and Plasmodium ovale wallikeri in the Ivory Coast and in the Comoros Islands. Malar J. 2012;11:307. doi:10.1186/1475-2875-11-307.

    PubMed  PubMed Central  Article  Google Scholar 

  29. 29.

    Li Y, Wang G, Sun D, Meng F, Lin S, Hu X, et al. A case of Plasmodium ovale wallikeri infection in a Chinese worker returning from West Africa. Korean J Parasitol. 2013;51:557–62. doi:10.3347/kjp.2013.51.5.557.

    PubMed  PubMed Central  Article  Google Scholar 

  30. 30.

    Snounou G, Viriyakosol S, Zhu XP, Jarra W, Pinheiro L, do Rosario VE, et al. High sensitivity of detection of human malaria parasites by the use of nested polymerase chain reaction. Mol Biochem Parasitol. 1993;61:315–20.

    PubMed  CAS  Article  Google Scholar 

  31. 31.

    Lee EY, Maguire JH. Acute pulmonary edema complicating ovale malaria. Clin Infect Dis. 1999;29:697–8.

    PubMed  CAS  Article  Google Scholar 

  32. 32.

    Rojo-Marcos G, Cuadros-Gonzalez J, Mesa-Latorre JM, Culebras-Lopez AM, de Pablo-Sanchez R. Acute respiratory distress syndrome in a case of Plasmodium ovale malaria. Am J Trop Med Hyg. 2008;79:391–3.

    PubMed  Google Scholar 

  33. 33.

    Cinquetti G, Banal F, Rondel C, Plancade D, de Saint Roman C, Adriamanantena D, et al. Splenic infarction during Plasmodium ovale acute malaria: first case reported. Malar J. 2010;9:288. doi:10.1186/1475-2875-9-288.

    PubMed  PubMed Central  Article  Google Scholar 

  34. 34.

    Hachimi MA, Hatim EA, Moudden MK, Elkartouti A, Errami M, Louzi L, et al. The acute respiratory distress syndrome in malaria: is it always the prerogative of Plasmodium falciparum? Rev Pneumol Clin. 2013;69:283–6. doi:10.1016/j.pneumo.2013.03.001.

    PubMed  CAS  Article  Google Scholar 

  35. 35.

    Nolder D, Oguike MC, Maxwell-Scott H, Niyazi HA, Smith V, Chiodini PL, et al. An observational study of malaria in British travellers: Plasmodium ovale wallikeri and Plasmodium ovale curtisi differ significantly in the duration of latency. BMJ Open. 2013;3:5. doi:10.1136/bmjopen-2013-002711.

  36. 36.

    Chin W, Contacos PG, Buxbaum JN. The transmission of a West African strain of Plasmodium ovale by Anopheles freeborni and Anopheles maculatus. Am J Trop Med Hyg. 1966;15:690–3.

    PubMed  CAS  Google Scholar 

  37. 37.

    Coatney GR, Collins WE, Warren M, Contacos PG. The primate malarias. Atlanta: CDC; 1971.

    Google Scholar 

  38. 38.

    Mellon G, Ficko C, Thellier M, Kendjo E, Aoun O, Adriamanantena D, et al. Two cases of late Plasmodium ovale presentation in military personnel. J Travel Med. 2014;21:52–4. doi:10.1111/jtm.12077.

    PubMed  Article  Google Scholar 

  39. 39.

    Haydoura S, Mazboudi O, Charafeddine K, Bouakl I, Baban TA, Taher AT, et al. Transfusion-related Plasmodium ovale malaria complicated by acute respiratory distress syndrome (ARDS) in a non-endemic country. Parasitol Int. 2011;60:114–6. doi:10.1016/j.parint.2010.10.005.

    PubMed  Article  Google Scholar 

  40. 40.

    de Laval F, Simon F, Bogreau H, Rapp C, Wurtz N, Oliver M, et al. Emergence of Plasmodium ovale malaria among the French armed forces in the Republic of Ivory Coast: 20 years of clinical and biological experience. Clin Infect Dis. 2014;58:e122–8. doi:10.1093/cid/ciu021.

    PubMed  Article  Google Scholar 

  41. 41.

    Li M, Xia Z, Yan H. New type of SSUrDNA sequence was detected from both Plasmodium ovale curtisi and Plasmodium ovale wallikeri samples. Malar J. 2014;13:216.

    PubMed  PubMed Central  Article  Google Scholar 

  42. 42.

    Castellanos Mí E, Díaz S, Parsons E, Peruski LF, Enríquez F, Ramírez JL, et al. First imported Plasmodium ovale malaria in Central America: case report of a Guatemalan soldier and a call to improve its accurate diagnosis. Mil Med Res. 2015;2:3. doi:10.1186/s40779-015-0030-9.

    Article  Google Scholar 

  43. 43.

    Chaturvedi N, Bhandari S, Bharti PK, Basak SK, Singh MP, Singh N. Sympatric distribution of Plasmodium ovale curtisi and P. ovale wallikeri in India: implication for the diagnosis of malaria and its control. Trans R Soc Trop Med Hyg. 2015;109:352–4. doi:10.1093/trstmh/trv015.

    PubMed  Article  Google Scholar 

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Authors’ contributions

JWKL performed the molecular biology techniques and drafted the manuscript. RM performed the microscopy. LHT presented the patient’s history and clinical symptoms. YLL conceptualize the manuscript. All authors read and approved the final manuscript.

Acknowledgements

This work was supported by University of Malaya High Impact Research Grant (UM.C/625/1/HIR/MOHE/CHAN/14/3) from the Ministry of Higher Education, Malaysia. The authors would like to thank the Parasites: South East Asian Diagnostic (PARA:SEAD) Laboratory, Kuala Lumpur, Malaysia for the assistance during diagnosis.

Competing interests

The authors declare that they have no competing interests.

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Correspondence to Yee Ling Lau.

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Liew, J.W.K., Mahmud, R., Tan, L.H. et al. Diagnosis of an imported Plasmodium ovale wallikeri infection in Malaysia. Malar J 15, 8 (2016). https://doi.org/10.1186/s12936-015-1070-z

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Keywords

  • Plasmodium ovale wallikeri
  • PCR
  • Diagnosis
  • Malaysia
  • Southeast Asia