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ABSTRACT |
 TOP ABSTRACT INTRODUCTIONSUBJECTS AND METHODSRESULTSDISCUSSIONREFERENCES |
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INTRODUCTION |
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TOPABSTRACTINTRODUCTIONSUBJECTS AND METHODSRESULTSDISCUSSIONREFERENCES |
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Detection of low parasitemia with P. falciparum is a challenge. Although diagnostic methods have improved greatly over the past decade, for malaria diagnosis the classic thick blood smear method still remains the standard in clinical malaria diagnosis. Rapid diagnostic tests (RDTs) are a fast and easy-to-perform alternative method of diagnosis, but they show decreased sensitivity at lower parasitemia.8 Most of these tests are based on detection of several proteins, including histidine-rich protein 2 (HRP-2), which is the most sensitive antigen marker for P. falciparum.9 Because of its long half-life, detection of this protein does not always correlate with the presence of viable parasites, thus leading to false-positive results and lower specificity.10 Parasite-specific aldolase (panmalarial antigen) is used as a complementary antigen in second-generation HRP-2 tests being produced for use with the four Plasmodium species that infect humans.9 Polymerase chain reaction (PCR) techniques detect parasites at densities less than one parasite per microliter. The subtelomeric variable open reading frame (stevor) gene sequences are unique to P. falciparum and can be used for highly sensitive PCR assays. With this method, 10 parasites can be detected in 1 mL of blood.11
In this study, using three different methods for parasite detection, we report the prevalence of asymptomatic P. falciparum infection in adults living near Lambaréné, Gabon.
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SUBJECTS AND METHODS |
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During an epidemiologic survey, we enrolled 497 male 18–51-year-old individuals (mean ± SD age = 30 ± 8 years) in the study. All participants were healthy volunteers without clinical signs and symptoms of malaria from villages located 
50 km from Lambaréné. Written informed consent was obtained before screening for P. falciparum parasitemia. Demographic data and dates of sampling were documented. For each individual only one finger prick was performed. We immediately prepared a thick blood smear for an RDT and dotted blood on Whatman (Brentford, United Kingdom) filter paper for analysis by a stevor-PCR. Samples were collected by a fieldworker team from March 2005 to April 2006. In Plasmodium spp.–positive cases diagnosed from blood smear or by RDT, subjects were examined by a physician in our clinical trial unit. If symptoms of malaria developed, individuals were treated orally with artesunate (Arsumax®, 50 mg; Sanofi-Aventis, Gentilly, France) for five days. Ethical clearance was obtained from the ethics committee of the International Foundation Albert Schweitzer Hospital.
Malaria blood smear. In this study, the Lambaréné method for thick film preparation and reading was applied as described elsewhere.14 Blood smears were stained with a 20% Giemsa solution. Two experienced technicians individually examined the microscopic slides. The main objective was to find P. falciparum. The technicians read at least 100 microscopic high-power fields with oil-immersion (CH30 microscope; Olympus, Tokyo, Japan). Parasitemia was calculated as parasites per microliter (counted parasites/no. of microscopic fields) x 600.14 The final result was obtained by calculating the arithmetic mean from parasite count of the first and second readings. If different results for parasitemia were obtained, a third experienced technician read the slides to obtain a final result. A third reading was also conducted if the ratio of results between higher and lower parasitemias was > 1.5 or if both results for parasitemia were less than 300 parasites/µL and had a difference of more than 100 parasites/µL.
Rapid diagnostic test Immunochromatographic antigen detection. We used an RDT (NOW® ICT Malaria Test; Binax, Inc., Portland, ME), which detects markers for all four human pathogenic Plasmodium species. For each individual, 15 µL of EDTA-whole blood was applied to the test strip. The reagent, which contained buffer solution and detecting antibody against HRP-2 or parasite-specific aldolase labeled with colloidal gold, was then applied. All of tests were performed in accordance with the manufacturer’s instructions and showed a well-visible control line. Tests were performed within five minutes after finger prick blood sampling. Interpretation of results was done after 15 minutes. Results were noted and the used test cards were archived.
PCR technique (stevor genes amplification). Thirty microliters of capillary blood of each individual, collected from the same finger prick, was applied onto filter paper (Whatman). The filter papers were dried and stored individually in sealed plastic bags. The DNA from dried blood spots was purified using a purification kit (Qiamp DNA mini kit; Qiagen, Valencia, CA).
A nested PCR was conducted according to the modified protocol of Cheng and others for detection of plasmodial DNA.11 The PCR was conducted in a thermocycler (PTC-200; MJ Research, Watertown, MA). For the first-round PCR, we used four primers: P5, 5'-gggaattcTTTATTTGAT-GAAGATG-3' (lowercase bases are not part of the stevor sequence); P18, 5'-TTTCA(C)TCACCAAACATTTCTT-'3; P19, 5'-AATCCACATTATCACAATGA-3'; and P20, 5'-CCGATTTTAACATAATATGA-3'. Ten microliters (5.0–25 ng) of DNA was added to 3 µL of P5, P18, P19, and P20 (10 µM), 10 µL of 10x buffer, 20 µL of MgCl2 (25 mM), 0.8 µL of dNTP (25 mM), 0.5 µL of Taq polymerase (5 U/µL), and 46.7 µL of distilled water. A total of 22 cycles (93°C for 30 seconds, 50°C for 50 seconds, and 72°C for 30 seconds) were performed. For the second-round PCR, primers P17, 5'-ACATTATCATAATGAC(T)CCAGAACT-3' and P24, 5'-GTTTCCAATAATTCTTTTTCTATC-3' were used. Two microliters of first-round PCR products were added to 2 µL of P17 and P24 (10 µM), 5 µL of 10x buffer, 5 µL of MgCl2 (25 mM), 0.8 µL of dNTP (25 mM), 0.25 µL of Taq polymerase (5 U/µL), and 33 µL of distilled water and 35 cycles (93°C for 30 seconds, 55°C for 50 seconds, and 72°C for 30 seconds) were performed. Five microliters of this PCR product was added to 1 µL of Sybr Green (Biozym Scientific, Hessisch Oldendorf, Germany), 2 µL of 5x buffer, and 2 µL of distilled water and analyzed by electrophoresis on a 2% agarose gel (Peqlab, Erlangen, Germany). Positive and negative controls were run in parallel with each test sample. The presence of DNA fragments was interpreted as a positive test result.
Statistical analysis. Results of 497 individuals were used for the assessment of data quality on the basis of descriptive statistics, including means and standard deviations, medians and interquartile ranges, and proportions. Data of 466 individuals with results for each test method were analyzed for stratification of parasitemia and comparison of the diagnostic methods by calculating the coefficient of agreement. Sample size calculation was not done. Data analyses were performed using SAS JMP version 5 (SAS Institute, Inc., Cary, NC) and Excel® 2002 Microsoft (Redmond, WA).
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RESULTS |
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Results of RDT in the absence of clinical symptoms.
Histidine-rich protein 2 was detected in 132 (27%) (95% CI = 23–31%) of 496 RDTs (Table 1
). In 17 of these tests with positive results, there was also a line for the parasite specific aldolase, which indicated a P. falciparum or mixed infection.
Screening for P. falciparum by PCR.
Overall, 244 (52%) (95% CI = 47–56%) of 470 samples were positive in the stevor PCR (Table 1).
Comparison of diagnostic test results.
A total of 466 samples for which results of all three tests were available were analyzed (Tables 2–4). Although 114 of 466 tests results were positive in the PCR and in either one or both of the other tests, 128 of 466 test results were positive only in the PCR. The coefficients of agreement (Cohen’s kappa) were 0.22 for thick blood smear and stevor PCR, 0.30 for RDT and stevor PCR, and 0.81 for RDT and thick blood smear. When we used the PCR as the gold standard, the sensitivity and specificity were 22% and 100% for the blood smear and 46% and 93% for the RDT. The positive predictive values and negative predictive values were 100% and 54% for the blood smear and 88% and 62% for the RDT.
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DISCUSSION |
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Although sensitivity for the thick blood smear was not high, the advantages of this procedure were high specificity, quantification of parasitemia, and easy handling. Not sufficiently screening blood transfusions that contain low parasite densities and administered to non-immune individuals, such as children, can be a concern because of transfusion-malaria. Detection of parasites depends on the amount of blood processed. Even the most sensitive PCR method may not be successful because only a small amount of blood is usually examined.
During the last century, efforts were made to control vectors of malaria. Attempts were made either to eradicate mosquitoes or to protect individuals from mosquito bites. However, less attention was paid to the human reservoir of P. falciparum. A study in Brazil underlines the importance of asymptomatic carriers with low-level parasitemias for malaria transmission. Persons with PCR-detectable parasitemia may serve as a reservoir for transmissible parasites.18 Therefore, treatment may be useful for malaria control. However, persistent low-level parasitemia seems to be a prerequisite for enduring semi-immunity in African adults. Thus, asymptomatic P. falciparum parasitemia in adults living in a malaria-endemic country seems to be common.
Received October 22, 2006. Accepted for publication February 28, 2007.
Acknowledgments: We thank all persons from villages near Lambaréné for participating in the study; Philemon Koumba-Koumba and Leonce Massoussa Mbadinga for assistance during sample collection; Judith Kammer, Marcel Nkeyi, Anselme Ndzengue, Brigitte Migombet, and Ariane Ntseyi for microscopic examination of the thick blood smears; and Andrea Weierich for conducting the stevor-PCR analysis.
* Address correspondence to Matthias P. Dal-Bianco, Medical Research Unit, Albert Schweitzer Hospital, BP 118 Lambaréné, Gabon and Department of Parasitology, Institute of Tropical Medicine University of Tübingen, Wilhelmstrasse 27, 72074, Tübingen, Germany. E-mail:matthiasdalbianco{at}yahoo.com 
Authors’ addresses: Matthias P. Dal-Bianco, Pierre B. Matsiegui, Michel A. Missinou, Saadou Issifou, Bertrand Lell, and Peter Kremsner, Medical Research Unit, Albert Schweitzer Hospital, BP 118 Lambaréné, Gabon and Department of Parasitology, Institute of Tropical Medicine University of Tübingen, Wilhelmstrasse 27, 72074, Tübingen, Germany. Kai B. Köster, Ulrich D. Kombila, Ghyslain Mombo Ngoma, Christian Supan, and Carmen L. Ospina Salazar, Medical Research Unit, Albert Schweitzer Hospital, BP 118 Lambaréné, Gabon. Jürgen F. J. Kun, Department of Parasitology, Institute of Tropical Medicine University of Tübingen, Wilhelmstrasse 27, 72074, Tübingen, Germany. Martin P. Grobusch, Infectious Diseases Unit, Division of Clinical Microbiology and Infectious Diseases, National Health Laboratory Service and School of Pathology, Faculty of Health Sciences University of the Witwatersrand, 7 York Road, Parktown 2196, Johannesburg, South Africa and Medical Research Unit, Albert Schweitzer Hospital, BP 118 Lambaréné, Gabon.
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