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Volume 20, Number 3—March 2014
Research

Comparison of Imported Plasmodium ovale curtisi and P. ovale wallikeri Infections among Patients in Spain, 2005–2011

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Author affiliations: Príncipe de Asturias University Hospital, Madrid, Spain (G. Rojo-Marcos, J. Arévalo-Serrano, J. Cuadros-González,); Instituto de Salud Carlos III, Madrid (J.M. Rubio-Muñoz); Carlos III Hospital, Madrid (G. Ramírez-Olivencia); La Paz University Hospital, Madrid (S García-Bujalance); Doctor Negrín University Hospital, Las Palmas de Gran Canaria, Spain (R. Elcuaz-Romano); Ramón y Cajal Hospital, Madrid (M. Díaz-Menéndez); Gregorio Marañón University Hospital, Madrid (M. Calderón); Getafe University Hospital, Madrid (I. García-Bermejo); University Hospital of Fuenlabrada, Madrid (J. M. Ruiz-Giardín); Severo Ochoa University Hospital, Madrid (F.J. Merino-Fernández); University General Hospital of Alicante, Alicante, Spain (D. Torrús-Tendero); University Hospital Fundación Alcorcón, Madrid (A. Delgado-Iribarren); Hospital General de Granollers, Barcelona, Spain (M. Ribell-Bachs).

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Abstract

Sequencing data from Plasmodium ovale genotypes co-circulating in multiple countries support the hypothesis that P. ovale curtisi and P. ovale wallikeri are 2 separate species. We conducted a multicenter, retrospective, comparative study in Spain of 21 patients who had imported P. ovale curtisi infections and 14 who had imported P. ovale wallikeri infections confirmed by PCR and gene sequencing during June 2005–December 2011. The only significant finding was more severe thrombocytopenia among patients with P. ovale wallikeri infection than among those with P. ovale curtisi infection (p = 0.031). However, we also found nonsignificant trends showing that patients with P. ovale wallikeri infection had shorter time from arrival in Spain to onset of symptoms, lower level of albumin, higher median maximum core temperature, and more markers of hemolysis than did those with P. ovale curtisi infection. Larger, prospective studies are needed to confirm these findings.

 Length: 1:27

Malaria caused by Plasmodium ovale infection has been considered a low-prevalence disease with limited geographic distribution, benign clinical course, and easy treatment; therefore, little attention has been paid to it. Diagnosis of P. ovale malaria can be difficult because of low parasitemia levels, mixed infections with other Plasmodium species, and false negatives from malaria rapid diagnostic tests (RDTs) (1). However, recent epidemiologic studies conducted by using PCR techniques have found P. ovale infections in most of sub-Saharan Africa, Southeast Asia, and the Indian subcontinent (2–5), including prevalence as high as 15% according to results of cross-sectional studies conducted in rural Nigeria (6) and Papua New Guinea (7). In addition, severe complications such as spleen rupture, severe anemia, or acute respiratory distress syndrome (ADRS) (8) may occur in patients with P. ovale malaria. Thus, the global burden of P. ovale infection might have been underestimated.

On the basis of differences in its gene sequences, P. ovale was considered to be dimorphic or to comprise 2 subspecies (2,3,9,10). This difference has hampered molecular diagnosis in some cases because of lack of DNA amplification by PCR with gene-specific primers for the small subunit ribosomal RNA (ssrRNA) (10). These subspecies had been named classic and variant P. ovale, but a comprehensive study recently described differences between these subspecies in at least 6 genes (4). These findings demonstrate that P. ovale actually consists of 2 subspecies that co-circulate in Africa and Asia and that are unable to recombine genetically; the differences seem to be explained by real biological factors, rather than ecologic or geographic factors (11). P. ovale curtisi and P. ovale wallikeri were the names proposed for these species (4).

Scant information is available on differences in clinical and analytical features, relapse profile, or accuracy of RDT results between these proposed species. Relatively high parasitemia levels were found in some patients with P. ovale wallikeri infection in Thailand (12), Vietnam (13), and Flores Island (14). A study published from a disease-endemic area of Bangladesh reported on the clinical features and degree of parasitemia in 13 patients with P. ovale wallikeri infection and 10 with P. ovale curtisi infection (5). These infections were diagnosed by PCR; only 4 of the 23 patients were symptomatic. Another recent study compared parasitemia levels, RDT results, and patient country of origin for 31 patients from Côte d’Ivoire and the Comoros Islands with imported P. ovale wallikeri infection and 59 with P. ovale curtisi infection, but no clinical data were provided (15). Clearly, information on these infections is limited.

Growth in international travel and migration has increased the incidence of imported malaria in industrialized countries. P. ovale infection may represent up to 8% of imported malaria cases, according to some published series of patients primarily from West Africa (16,17), where the proportion of sub-Saharan immigrants is high and PCR has been systematically performed. Yet, it is difficult to gather a substantial number of cases with clinico-epidemiologic correlation and molecular data. To identify clinical or analytical differences between P. ovale wallikeri and P. ovale curtisi infections and expand data on these infections, we conducted a multicenter, retrospective, comparative study of imported P. ovale infections diagnosed in Spain during 2005–2011.

Methods

Sample Selection

During June 2005–December 2011, blood samples from all patients with positive PCR results for imported infection with P. ovale were sent from public hospitals in Spain to the reference Malaria & Emerging Parasitic Diseases Laboratory of the National Centre of Microbiology in Madrid. The samples were shipped to the laboratory 1) to confirm the diagnosis of malaria and the species or 2) to study fever, anemia, or suspected malaria in patients with negative results on thick and/or thin smears and RDTs who were considered at high risk for malaria (i.e., immigrants and travelers to malaria-endemic areas).

Microbiological Diagnosis

The initial diagnosis of imported Plasmodium spp. infection was made by thick and/or thin smears and/or by using the second-generation RDT NOW Malaria Test Kit (Binax Inc., Scarborough, ME, USA) for histidine-rich protein 2 antigen of P. falciparum and aldolase enzyme common to all Plasmodium spp. Blood smears were stained by a standard technique with Giemsa solution for 30 min and were reviewed by an expert microbiologist. Parasite count was measured by determining the proportion of parasitized erythrocytes or the number of trophozoites per microliter.

Isolation of Parasite DNA and Molecular Diagnosis Confirmation

DNA isolation from whole blood was performed by using the QIAamp DNA Blood Mini Kit (QIAGEN, Hilden, Germany), according to the manufacturer’s protocol. P. ovale molecular diagnosis was confirmed by using seminested multiplex malaria PCR (18), which enables the discernment of the 4 most prevalent human malaria species by amplified fragments of DNA in 2 sequential PCRs.

P. ovale Subtype Characterization and Confirmation

Partial sequencing of the ssrRNA gene was used to differentiate P. ovale curtisi from P. ovale wallikeri. ssrRNA amplification was performed by using a nested PCR specific for Plasmodium. The first reaction included UNR (5′-GACGGT ATCTGATCGTCTTC-3′) and PLF (5′- AGTGTGTATCCAATCGAGTTTC-3′) primers, which correspond to the first reaction of the seminested multiplex malaria PCR. The second reaction incorporated the products of the first reaction, along with NewPLFsh (5′-CTATCAGCTTTTGATGTTAG-3′) and NewRevsh (5′-CCTTAACTTTCGTTCTTG-3′) primers. Infection with different malaria species yielded products of 710–740 bp.

The PCR mixture in both reactions consisted of 75 mmol/L Tris-HCl (pH 9.0), 2 mmol/L MgCl2, 50 mmol/L KCl, 20 mmol/L (NH4)2SO4, 200 μmol/L dNTP, 0.075 μmol/L of the corresponding PCR primers, 1.25 units Taq DNA polymerase (Biotools B&M Labs, S.A., Madrid, Spain), and the template DNA in a reaction volume of 50 μL. The amount of template was 5 μL of DNA extracted by using a QIAamp DNA Blood Mini Kit (QIAGEN). For the second reaction mixture, 2 μL of the PCR product of the first reaction was used as template. For both reactions, a GeneAmp PCR System 2700 thermal cycler (Applied Biosystems, Foster City, CA, USA) was used, beginning with 7 min at 94°C, followed by 40 cycles of 20 s at 94°C, 20 s at 62°C, and 30 s at 72°C for the first round; or 35 cycles of 20 s at 94°C, 20 s at 53°C, and 20 s at 72°C for the second round. The final cycle was followed by an extension time of 10 min at 72°C.

The amplified products were purified by using Illustra DNA and Gel Band Purification Kit (GE Healthcare, Buckinghamshire, UK) and sequenced by using the Big Dye Terminator v3.1 Cycle Sequencing Kit and ABI PRISM 3700 DNA Analyzer (Applied Biosystems). All amplified products were sequenced in both directions twice. To confirm P. ovale subtyping, a nested PCR amplification plus sequencing targeting cytochrome (Cyt) b was performed (3) in 3 samples of each group, by using a unique second amplification (nested) reaction with primers Cyt b 2F and Cyt b 2R.

Data Collection

Hospitals that submitted PCR-confirmed and P. ovale subtype–identified samples were invited to collaborate in the study. A database was designed and completed after the retrospective review of medical reports and laboratory registries. Patient data collected included sex, age, ethnicity, underlying diseases, time living in non–malaria-endemic countries, dates and purpose of travel, countries visited, malaria chemoprophylaxis, date of admission and diagnosis, symptoms and clinical signs, physical examinations, and complications of severe malaria according to World Health Organization criteria (19). The closest possible date of infection was defined as the day of departure from a malaria-endemic area. The time between date of arrival in Spain and onset of illness or diagnosis was calculated once asymptomatic patients were excluded. Patients were classified as early immigrant if they had stayed in a country without malaria for <1 year before diagnosis and as visiting friends and relatives if they had traveled to a malaria-endemic country after 1 year living in a non–malaria-endemic area. Recent Plasmodium infection was defined as probable or definite malaria infection in the 3 months before P. ovale infection was diagnosed.

Recorded laboratory results included microbiological data; complete blood count with leukocytes, hemoglobin, and platelet levels; levels ​​of creatinine, albumin, transaminases, lactate dehydrogenase, and direct bilirubin in plasma; and glucose-6-phosphate dehydrogenase activity in erythrocytes. Abdominal ultrasonography and serologic studies to detect infection with HIV and hepatitis A, B, and C viruses were reviewed. Recorded treatments and compliance, clinical and microbiological evolution, and duration of hospital stay for those admitted were included.

Statistical Analysis

Differences of proportions were evaluated by χ2 test or Fisher exact test, as appropriate for sample size. Means between groups were calculated by using the Student t-test for independent samples if the normal distribution could be assumed; we used the Levene test for homogeneity of variances. If normality was not valid, we used the Mann-Whitney U test for nonparametric variables.

To test for normality, we used either the Shapiro-Wilks test for small samples or the Kolmogorov-Smirnov test with the Lilliefors correction for large samples. Values were reported as means and SDs or, for nonparametric distributions, medians and interquartile ranges (IQRs). A 2-sided p value of <0.05 was considered to indicate statistical significance. Statistical analyses were performed by using SPSS version 15 (SPSS Inc., Chicago, IL, USA).

Results

During June 2005–December 2011, a total of 102 samples positive by PCR for P. ovale were analyzed at the reference laboratory; of these, we were able to amplify and genotype 55 samples. Poor quality of long-term stored DNA prevented amplification of the other samples. Genetic analyses of the cytb gene identified P. ovale curtisi in 31 samples from 28 patients and P. ovale wallikeri in 24 samples from to 22 patients.

Twelve hospitals agreed to participate in the study and provided complete epidemiologic, microbiological, biochemical, clinical, and therapeutic information for 35 of the 50 patients for which P. ovale genetic characterization was available. Of these, 21 patients had P. ovale curtisi infection and 14 had P. ovale wallikeri infection. Table 1 shows the demographic and epidemiologic data for these 35 patients. Patient age and sex were virtually the same for patients with P. ovale curtisi and P. ovale wallikeri infections and corresponded mostly to young persons from Africa who traveled to visit their friends and relatives for a long period or immigrants who had recently arrived.

The lapses between time of arrival in Spain, onset of illness, and diagnosis were longer for patients with P. ovale curtisi infection than for those with P. ovale wallikeri infection, but not significantly. Most travelers did not take any malaria prophylaxis or did not adhere to the full regimen. All but 2 infections were acquired in West Africa, and both Plasmodium species were found in patients from Nigeria, Equatorial Guinea, Ghana, and Guinea-Conakry. A high rate of underlying disease was found among patients in both parasite groups; the P. ovale curtisi group included 3 early immigrants who were chronically infected with HIV, hepatitis B virus, and hepatitis C virus and carried filarial and intestinal parasites.

Microbiological and laboratory data for the patients are shown in Table 2. Statistically significant worse levels of thrombocytopenia were found among patients with P. ovale wallikeri infection compared with those who had P. ovale curtisi infection, but no other significant difference was found. One mixed infection with P. falciparum was found among each patient group. The RDT technique used showed a low sensitivity (<30%) for detecting P. ovale once mixed infections were excluded.

Clinical and therapeutic data for the patients are shown in Table 3. All 3 asymptomatic patients had P. ovale curtisi infection; 1 infection was detected as an incidental finding in a blood smear for sickle cell disease, and the other 2 were found during studies of anemia after negative results were found by thick film examination and RDT results. The remaining 7 patients with negative thick smear and positive PCR results reported at least fever. Symptomatic patients showed no difference in clinical signs and symptoms, but those with P. ovale wallikeri did have a higher mean number of symptoms (3.5 per patient) than did those with P. ovale curtisi (2.7). The number of complications was similar in both groups; 3 cases of severe anemia occurred, 2 of them related to sickle cell disease, and 1 case of ADRS occurred in a patient with P. ovale wallikeri infection.

Most patients were admitted to a hospital and received inpatient treatment. Roughly half the patients in each group received chloroquine alone. Almost all patients showed good tolerance to treatment and favorable clinical evolution. More than a quarter (33.3% of P. ovale curtisi and 28.6% of P. ovale wallikeri) did not receive primaquine for radical cure, 2 because of glucose-6-phosphate dehydrogenase deficiency. One patient was lost to follow-up and did not receive any treatment or monitoring.

Discussion

Our comparative study of the epidemiologic and clinical characteristics of patients with P. ovale curtisi and P. ovale wallikeri infection found only 1 statistically significant result, a higher rate of severe thrombocytopenia among patients with P. ovale wallikeri infection (p = 0.031). Nevertheless, we noted nonsignificant results, including a shorter time from arrival to onset of symptoms in travelers who acquired P. ovale wallikeri infection (p = 0.077). This finding fits with findings from a recently published larger series from the United Kingdom in which a significantly shorter latency was found for P. ovale wallikeri compared with P. ovale curtisi infection (20). We also found a trend toward a shorter stay in Africa and shorter interval between onset of symptoms and diagnosis among patients with P. ovale wallikeri infection, which could reflect easier transmission, shorter latency, or higher relapse rates. This finding might also mean that slightly more severe illness, including higher median fever (39.7°C vs. 38.4°C) and a greater number of symptoms (3.5 vs. 2.7 per symptomatic patient), led more patients with P. ovale wallikeri infection than those with P. ovale curtisi infection to seek medical attention earlier. However, the higher percentage of travelers who took at least partial prophylaxis among the P. ovale curtisi group (19.2%) might also explain a longer time of onset. A high frequency of nausea and vomiting was found among those with P. ovale wallikeri infection, a symptom that was absent among those with P. ovale curtisi infection. However, because most cases were asymptomatic or had mild to moderate clinical features, finding significant differences within this narrow clinical spectrum may be especially difficult and might require a much larger study.

Because the time of infection is more likely to be accurately known, patients with imported malaria might make a better group for study of the epidemiologic and clinical characteristics of different Plasmodium species than those living in malaria-endemic countries. Moreover, signs or symptoms may be less affected by other tropical infections, including mixed Plasmodium infections, or by patient immunity; imported malaria occurs among a larger number of nonimmune patients and patients who are visiting friends and relatives. Differentiation among primary infection or relapse continues to be practically impossible, but the longer the time of latency, the more probable a relapse.

Although criteria for admission to each hospital involved in the study were different, P. ovale wallikeri patients were admitted more frequently. The number of complications was similar in both groups; 3 cases of severe anemia were reported, 2 related to sickle cell disease, and 1 case of ADRS occurred in a patient infected with P. ovale wallikeri (8). Sickle cell trait was described as a risk factor for infection with P. ovale in Senegal (21), and a recent series showed 3 of 16 patients with P. ovale infection were homozygous for sickle cell disease (22), a clearly disproportionate number.

Regarding symptomatic patients, the Bangladesh study (5) showed a trend toward a larger number of asymptomatic P. ovale curtisi infections (90% vs. 75% for P. ovale wallikeri), which would be consistent with our results. In that study, all 13 mixed infections of P. ovale with other Plasmodium species were asymptomatic; in our study, the 2 patients who had mixed infections with P. falciparum had at least fever. The number of P. ovale monoinfections in our study confirmed by PCR is high, unlike the number in malaria-endemic areas, where most infections are mixed (5,7,23) and a high rate of submicroscopic carriage occurs (24). In part, our finding may result from previous antimalarial treatment or prophylaxis in a number of patients, which could have minimized the number of Plasmodium parasites in the blood.

Among the laboratory results, the only significant difference was found in platelet count, with more severe thrombocytopenia seen among patients with P. ovale wallikeri infection than among those with P. ovale curtisi infection. Thrombocytopenia is a common finding in patients with malaria; a previous series found 10 (66.6%) of 15 patients with imported P. ovale infection had platelet counts of <140,000/μL (22). The mechanisms that produce thrombocytopenia in malaria are not known but seem related to a greater severity of illness (25). Some studies also suggest an inverse correlation between the level of parasitemia and platelet count (26).

We found that indirect parameters of hemolysis, such as hemoglobin, lactate dehydrogenase, and bilirubin levels, were less impaired among patients with P. ovale curtisi infection than those with P. ovale wallikeri infection, even including 2 patients with sickle cell disease, who had more severe anemia. Albumin values, diminished by other multiple types of infections, ​​also tend to be lower in patients with P. ovale wallikeri infection. For transaminases, if we were to exclude a patient with chronic hepatitis B and hypertransaminasemia, we would also find higher values ​​for patients with P. ovale wallikeri infection. These data collectively raise the hypothesis that P. ovale wallikeri is slightly more pathogenic, which warrants further investigation.

Parasitemia levels were not significantly different between the 2 groups (p = 0.699). In 2 recent studies of P. ovale infection that included determination of parasitemia levels and genetic analysis (5,15), no differences were described. Case reports of high parasitemia levels in patients with P. ovale wallikeri infection in Southeast Asia are isolated and noncomparative (12–14).

Sooner and better access to health care in industrialized countries might provide a broader range of diagnostic tools for malaria, including RDT, thick and thin film examination, or PCR. Current techniques of RDT still show a low sensitivity for detecting P. ovale (27,28). This problem is usually explained by the genetic variability of the 2 subspecies and the low levels of parasitemia detected. After discarding mixed infections, in our study, the aldolase-based RDT used as a common antigen of Plasmodium obtained 20% sensitivity for detection of P. ovale curtisi and 27.27% for P. ovale wallikeri. Results are poorer than those recently published by Bauffe et al., who found a higher false-negative rate of infection for P. ovale curtisi than for P. ovale wallikeri (60% vs. 43%, respectively) and no significant differences in parasitemia levels (15).

Although circulation of P. ovale was known in these countries, our study provides PCR confirmation for P. ovale curtisi infections from Guinea-Conakry, Ethiopia, and Liberia and P. ovale wallikeri infections from Mozambique. Both species have been described as sympatric in time and space in Equatorial Guinea, Republic of Congo, Uganda, Bangladesh, and Angola (5,11,29), maintaining genetic differentiation, which supports the hypothesis of 2 distinct subspecies. Moreover, 2 cases of P. ovale curtisi and P. ovale wallikeri co-infection have been reported (5,29).

We found a high rate of underlying chronic diseases among the patients in this study, especially homozygous sickle cell anemia and diabetes mellitus. Previous studies have shown that carriage of the sickle cell trait confers increased susceptibility to P. ovale infection (20) and that diabetes and HIV infection confer increased susceptibility to P. falciparum infection (30).

In industrialized countries, improved clinical and microbiological control after treatment and radical cure with primaquine can be achieved for malaria. P. ovale seems to remain sensitivity to chloroquine and other antimalarial drugs. Patients in our study showed good clinical response that could be followed up without any relapse, including among those who had complications. The treatment differences reflect the different hospital managing protocols, patient age and pregnancy status, or difficulty in identifying P. ovale initially.

Our study has limitations. First, the small number of patients may lack sufficient statistical power to show differences between infections with different Plasmodium species. Second, the low performance of genetic amplification may have caused some sample selection bias (e.g., a higher number of samples that were stored short term or came from patients with higher parasitemia levels). Third, patient selection was not systematically planned but was done on the basis of decisions of physicians from many hospitals who sent samples to the reference laboratory and subsequently agreed to participate in this study. Fourth, the study’s retrospective design led to gaps in the information collected. Fifth, only strains of P. ovale from Africa were analyzed, and patients were from Africa and Europe; a study of infections and patients from Asia or Oceania might show different results. Last, more diversity in the geographic origin of the strains and a mix of nonimmune and semiimmune patients would lead to more heterogeneous study groups.

In summary, after comparing epidemiologic, clinical, and analytic data for patients with P. ovale wallikeri and P. ovale curtisi infections, we found significantly more marked thrombocytopenia among patients with P. ovale wallikeri infection, but we found no other significant differences. However, some trends toward slightly greater pathogenicity were observed for P. ovale wallikeri infection. The description of both genotypes occurring in sympatry without hybrid forms in an increasing number of countries supports the idea of ​​2 well-defined species. Larger prospective studies should be conducted to more fully explore this hypothesis.

Dr Rojo-Marcos is a consultant in tropical and travel medicine with the Department of Internal Medicine, Príncipe de Asturias University Hospital, Alcalá de Henares, Madrid, Spain. His research interests include malaria, leishmaniasis, schistosomiasis, imported tropical diseases, and social and health problems of immigration.

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Acknowledgment

We thank Francisco Javier Vilar Izquierdo for his assistance in the translation and critical review of this manuscript.

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References

  1. Mueller  I, Zimmerman  PA, Reeder  JC. Plasmodium malariae and Plasmodium ovale—the “bashful” malaria parasites. Trends Parasitol. 2007;23:278–83. DOIPubMedGoogle Scholar
  2. Tachibana  M, Tsuboi  T, Kaneko  O, Khuntirat  B, Torii  M. Two types of Plasmodium ovale defined by SSU rRNA have distinct sequences for ookinete surface proteins. Mol Biochem Parasitol. 2002;122:223–6. DOIPubMedGoogle Scholar
  3. Win  TT, Jalloh  A, Tantular  IS, Tsuboi  T, Ferreira  MU, Kimura  M, Molecular analysis of Plasmodium ovale variants. Emerg Infect Dis. 2004;10:1235–40 . DOIPubMedGoogle Scholar
  4. Sutherland  CJ, Tanomsing  N, Nolder  D, Oguike  M, Jennison  C, Pukrittayakamee  S, Two non-recombining sympatric forms of the human malaria parasite Plasmodium ovale occur globally. J Infect Dis. 2010;201:1544–50 . DOIPubMedGoogle Scholar
  5. Fuehrer  H-P, Habler  VE, Fally  MA, Harl  J, Starzengruber  P, Swoboda  P, 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 . DOIPubMedGoogle Scholar
  6. May  J, Mockenhaupt  FP, Ademowo  OG, Falusi  AG, Olumese  PE, Bienzle  U, High rate of mixed and subpatent malarial infections in southwest Nigeria. Am J Trop Med Hyg. 1999;61:339–43 .PubMedGoogle Scholar
  7. Mehlotra  RK, Lorry  K, Kastens  W, Miller  SM, Alpers  MP, Bockarie  M, Random distribution of mixed species malaria infections in Papua New Guinea. Am J Trop Med Hyg. 2000;62:225–31 .PubMedGoogle Scholar
  8. Rojo-Marcos  G, Cuadros-González  J, Mesa-Latorre  JM, Culebras-López  AM, de Pablo-Sánchez  R. Acute respiratory distress syndrome in a case of Plasmodium ovale malaria. Am J Trop Med Hyg. 2008;79:391–3 .PubMedGoogle Scholar
  9. Li  J, Wirtz  RA, McConkey  GA, Sattabongkot  J, Waters  AP, Rogers  MJ, Plasmodium: genus-conserved primers for species identification and quantitation. Exp Parasitol. 1995;81:182–90. DOIPubMedGoogle Scholar
  10. Calderaro  A, Piccolo  G, Perandin  F, Gorrini  C, Peruzzi  S, Zuelli  C, Genetic polymorphisms influence Plasmodium ovale PCR detection accuracy. J Clin Microbiol. 2007;45:1624–7 . DOIPubMedGoogle Scholar
  11. Oguike  MC, Betson  M, Burke  M, Nolder  D, Stothard  JR, Kleinschmidt  I, Plasmodium ovale curtisi and Plasmodium ovale wallikeri circulate simultaneously in African communities. Int J Parasitol. 2011;41:677–83 . DOIPubMedGoogle Scholar
  12. Win  TT, Lin  K, Mizuno  S, Zhou  M, Liu  Q, Ferreira  MU, Wide distribution of Plasmodium ovale in Myanmar. Trop Med Int Health. 2002;7:231–9. DOIPubMedGoogle Scholar
  13. Kawamoto  F, Miyake  H, Kaneko  O, Kimura  M, Nguyen  TD, Nguyen  TD, Sequence variation in the 18S rRNA gene, a target for PCR-based malaria diagnosis in Plasmodium ovale from southern Vietnam. J Clin Microbiol. 1996;34:2287–9 .PubMedGoogle Scholar
  14. Win  TT, Tantular  IS, Pusarawati  S, Kerong  H, Lin  K, Matsuoka  H, Detection of Plasmodium ovale by the ICT Malaria P.f/P.v. immunochromatographic test. Acta Trop. 2001;80:283–4. DOIPubMedGoogle Scholar
  15. 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 . DOIPubMedGoogle Scholar
  16. Rojo-Marcos  G, Cuadros-González  J, Gete-García  L, Prieto-Ríos  B, Arcos-Pereda  P. Imported malaria in a general hospital in Madrid [in Spanish.]. Enferm Infecc Microbiol Clin. 2007;25:168–71. DOIPubMedGoogle Scholar
  17. Calderaro  A, Gorrini  C, Peruzzi  S, Piccolo  G, Dettori  G, Chezzi  C. An 8-year survey on the occurrence of imported malaria in a nonendemic area by microscopy and molecular assays. Diagn Microbiol Infect Dis. 2008;61:434–9. DOIPubMedGoogle Scholar
  18. Rubio  JM, Post  RJ, van Leeuwen  WM, Henry  MC, Lindergard  G, Hommel  M. Alternative polymerase chain reaction method to identify Plasmodium species in human blood samples: the seminested multiplex malaria PCR (SnM-PCR). Trans R Soc Trop Med Hyg. 2002;96(Suppl 1):S199–204 . DOIPubMedGoogle Scholar
  19. World Health Organization. Severe and complicated malaria. Trans R Soc Trop Med Hyg. 1990;84(Suppl 2):1–65 . DOIPubMedGoogle Scholar
  20. Nolder  D, Oguike  MC, Maxwell-Scott  H, Niyazi  HA, Smith  V, Chiodini  PL, 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:e002711.
  21. Faye  FB, Spiegel  A, Tall  A, Sokhna  C, Fontenille  D, Rogier  C, Diagnostic criteria and risk factors for Plasmodium ovale malaria. J Infect Dis. 2002;186:690–5. DOIPubMedGoogle Scholar
  22. Rojo-Marcos  G, Cuadros-González  J, Gete-García  L, Gómez-Herruz  P, López-Rubio  M, Esteban-Gutierrez  G. Plasmodium ovale infection: description of 16 cases and a review [in Spanish.]. Enferm Infecc Microbiol Clin. 2011;29:204–8 . DOIPubMedGoogle Scholar
  23. Kawamoto  F, Liu  Q, Ferreira  MU, Tantular  IS. How prevalent are Plasmodium ovale and P. malariae in East Asia? Parasitol Today. 1999;15:422–6 . DOIPubMedGoogle Scholar
  24. Bruce  MC, Macheso  A, Kelly-Hope  LA, Nkhoma  S, McConnachie  A, Molyneux  ME. Effect of transmission setting and mixed species infections on clinical measures of malaria in Malawi. PLoS ONE. 2008;3:e2775 . DOIPubMedGoogle Scholar
  25. Lacerda  MV, Mourão  MP, Coelho  HC, Santos  JB. Thrombocytopenia in malaria: who cares? Mem Inst Oswaldo Cruz. 2011;106(Suppl 1):52–63 . DOIPubMedGoogle Scholar
  26. Saravu  K, Docherla  M, Vasudev  A, Shastry  BA. Thrombocytopenia in vivax and falciparum malaria: an observational study of 131 patients in Karnataka, India. Ann Trop Med Parasitol. 2011;105:593–8 . DOIPubMedGoogle Scholar
  27. Moody  A. Rapid diagnostic tests for malaria parasites. Clin Microbiol Rev. 2002;15:66–78 . DOIPubMedGoogle Scholar
  28. Bigaillon  C, Fontan  E, Cavallo  JD, Hernandez  E, Spiegel  A. Ineffectiveness of the Binax NOW malaria test for diagnosis of Plasmodium ovale malaria. J Clin Microbiol. 2005;43:1011 . DOIPubMedGoogle Scholar
  29. Fançony  C, Gamboa  D, Sebastião  Y, Hallett  R, Sutherland  C, Sousa-Figueiredo  JC, Various pfcrt and pfmdr1 genotypes of Plasmodium falciparum cocirculate with P. malariae, P. ovale spp., and P. vivax in northern Angola. Antimicrob Agents Chemother. 2012;56:5271–7 . DOIPubMedGoogle Scholar
  30. Danquah  I, Bedu-Addo  G, Mockenhaupt  FP. Type 2 diabetes mellitus and increased risk for malaria infection. Emerg Infect Dis. 2010;16:1601–4 . DOIPubMedGoogle Scholar

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DOI: 10.3201/eid2003.130745

Table of Contents – Volume 20, Number 3—March 2014

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Gerardo Rojo-Marcos, Department of Internal Medicine, Príncipe de Asturias University Hospital, Ctra de Meco s/n, 28805 Alcalá de Henares, Madrid, SpainGerardo Rojo-Marcos, Department of Internal Medicine, Príncipe de Asturias University Hospital, Ctra de Meco s/n, 28805 Alcalá de Henares, Madrid, Spain

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Page created: February 19, 2014
Page updated: February 19, 2014
Page reviewed: February 19, 2014
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