Application of magnetic cytosmear for the estimation of Plasmodium falciparum gametocyte density and detection of asexual stages in asymptomatic children
© Sumari et al. 2016
Received: 12 November 2015
Accepted: 12 February 2016
Published: 24 February 2016
Conventional malaria parasite detection methods, such as rapid diagnostic tests (RDT) and light microscopy (LM), are not sensitive enough to detect low level parasites and identification of gametocytes in the peripheral blood. A modified and sensitive laboratory prototype, Magnetic Deposition Microscopy (MDM) was developed to increase the detection of sub-microscopic parasitaemia and estimation of gametocytes density in asymptomatic school children.
Blood samples were collected from 303 asymptomatic school children from seven villages in Bagamoyo district in Tanzania. Participants were screened for presence of malaria parasites in the field using RDT and MDM whereas further examination of malaria parasites was done in the laboratory by LM. LM and MDM readings were used to calculate densities and estimate prevalence of asexual and sexual stages of the parasite.
Plasmodium falciparum parasites (asexual and sexual stages) were detected in 23 (7.6 %), 52 (17.2 %), and 59 (19.5 %) out of 303 samples by LM, RDT and MDM respectively. Gametocytes were detected in 4 (1.3 %) and 12 (4.0 %) out of the same numbers of samples by LM, and MDM, respectively. Likewise, in vitro results conducted on two laboratory strains of P. falciparum, 3D7 and NF54 to assess MDM sensitivity on gametocytes detection and its application on concentrating gametocytes indicated that gametocytes were enriched by MDM by 10-fold higher than LM. Late stages of the parasite strains, 3D7 and NF54 were enriched by MDM by a factor of 20.5 and 35.6, respectively. MDM was more specific than LM and RDT by 87.5 % (95 %, CI 71.2–89.6 %) and 89.0 % (95 % CI 82.9–91.4) respectively. It was also found that MDM sensitivity was 62.5 % (95 % CI 49.5–71.8) when compared with RDT while with LM was 36.5 % (95 % CI 32.2–60.5).
These findings provide strong evidence that MDM enhanced detection of sub-microscopic P. falciparum infections and estimation of gametocyte density compared to current malaria diagnostic tools. In addition, MDM is superior to LM in detecting sub-microscopic gametocytaemia. Therefore, MDM is a potential tool for low-level parasitaemia identification and quantification with possible application in malaria transmission research.
Diagnosis of malaria especially in resource poor settings relies heavily on clinical symptoms or confirmation of Plasmodium falciparum parasites in blood by microscopic examination, or by detection of circulating parasite antigens using immunological methods, such as Rapid Diagnostic Test (RDT) . In Tanzania, about 95 % of the communities living at the coast possess mosquito nets and more than half of the households use insecticide-treated nets (ITNs) . Recent malaria survey conducted in Tanzania indicated that interventions have contributed dramatically to a general decline of clinical malaria in Pwani region [12, 13]. This has made it more difficult to diagnose P. falciparum at very low levels, hence prompting a shift from focusing only on clinical malaria to identifying and treating asymptomatic malaria infections [14, 15] that sustain transmission.
Malaria transmission depends on several factors, such as presence of mosquito vectors and infectious gametocytes in the peripheral human blood [16–18]. Plasmodium falciparum gametocytes circulate in the blood stream for longer period of time than gametocytes of other Plasmodium species, and they frequently occur at densities below microscopic detection . Gametocyte detection in the peripheral blood is a good indicator for characterizing the level of transmission . Sub-microscopic infections, especially gametocytaemia, constitute an important parasite reservoir in endemic populations  and has become a focus of interest for successful malaria elimination and eradication . A number of studies have been conducted focusing on treating asexual parasites responsible for clinical manifestation of the disease. Little attention has been directed on gametocytes, which are the parasite stage responsible for transmission of the disease even when present at low densities. This study focused on identifying and quantifying infectious reservoirs that sustain malaria transmission and investigated the usefulness of the MDM when used singly or in combination with conventional diagnostic methods in detecting P. falciparum gametocytaemia and asymptomatic infections in school-aged children in Bagamoyo district in Pwani region. The MDM device was evaluated firstly, for sensitivity to gametocytaemia and secondly, for ease of use in field operation. This is the first study in Tanzania reporting sensitivity and specificity of MDM for field detection of sub-microscopic infections of P. falciparum.
This was a cross-sectional study conducted in primary school children selected from five schools in two wards in Bagamoyo district, Tanzania. The study was carried out during a high malaria transmission seasons from May to June and from October to December 2014. Prior to commencement of the study, sensitization meetings were held in selected communities and their respective schools. School-teachers helped to distribute consent forms to the participants and arrange meetings with the children’s parents and/or guardians.
A total of 500 school children aged 6–14 years (whose malaria status was unknown) were enrolled of which 303 consented and were recruited for study. Out of the 303 children, 40 were recruited from Kongo primary school in Yombo ward (approximately 25 km from the laboratory) and 136, 49, 43 and 35 children were recruited, respectively from Kidomole, Fukayosi, Mwavi and Msinune primary schools in Kiwangwa ward (approximately 45 km from the laboratory). All 303 children whose parents consented were screened for malaria using RDT and MDM on the spot at the school premises. At the end of screening, the remaining blood was taken to the laboratory for microscopy on the same day. Both symptomatic and asymptomatic malaria cases were referred and offered appropriate treatment at nearby health facilities, according to the national malaria treatment guidelines [23, 24]. The inclusion criteria were child’s asymptomatic status, age between 6–14 years and parent’s consent.
This study received ethical approval from Institutional Review Board (No.IHI/IRB/No: 34-2013) of Ifakara Health Institute and Medical Research Coordinating Committee of the National Institute for Medical Research No. (NIMR/HQ/R.8a/Vol. IX/1705). Regional, district and community authorities in the study area were contacted and granted approval of the study. Prior to participation, a written consent of each respondent was obtained based on Informed Consent Forms (ICFs) designed for the study. Each parent or guardian was given the form that explained risks, benefits and confidentiality that would have been taken. Additionally, the confidentiality of all participants was assured by using unique identity study numbers. The parents and/or guardians, who consented, signed the ICFs and returned back to the study team through head teachers of the schools under study.
Blood sampling procedures and malaria screening
Three millilitres of venous blood from each participant were collected into heparin vacutainer tubes (Greiner Bio-One GmbH, Kremsmuenster, Austria) for RDT, LM and MDM. The RDT (ICT Malaria Dual Cassette Test; ICT Diagnostics, Cape Town, South Africa) was performed in the field for quick malaria screening as described elsewhere . A volume of 6 and 3 µL of blood were used for thick and thin blood smears immediately after collection respectively. Parasites were counted in accordance to World Health Organization (WHO) standards to detect and quantify parasites and their stages . Fifty microliter of whole blood was diluted 10× with warm phosphate buffered saline (PBS) (37 °C) to final volume of 0.5 mL and used for the MDM. The tubes containing a mixture of blood sample and buffer were kept at 37 °C before running into the prototype. All samples and buffers were maintained at 37 °C.
As a quality control measure two microscopists examined slides independently. Slides with high discordance were reexamined by a third microscopist. Samples were considered negative if no parasites were detected in 100 high-power fields of Giemsa-stained thick blood smears. Both, asexual and sexual stages of the parasites were assessed in thick smears by comparing ratio of infected red blood cells to uninfected ones. Thin smears were examined for parasite quantification. Gametocytes and asexual stage parasites were counted against 500 and 200 white blood cells (WBCs), respectively and densities (parasite per microlitre) were estimated using a factor of 8000 leukocytes/µL.
In vitro cultivation of malaria parasites
Prior to deployment of MDM for field-testing, its performance was validated and proven using P. falciparum laboratory strains, NF54 and 3D7. In vitro cultivation of these two strains was done at Case Western Reserve University, USA. The asynchronous parasite culture was set up at 0.5 % parasitaemia, 4 % haematocrit and maintained using complete malaria culture media [7, 27]. To obtain gametocytes, the cultures were left undisturbed for 4 days to allow induction of gametocytes. The young gametocytes were left to mature by changing the media daily while maintaining 1 % haematocrit. Mature gametocytes developed 15 days later. From the parasite culture stock solution of 1:10, MDM working solution was prepared by 1:10 serial dilution using 1× phosphate buffered saline (PBS) to obtain a working concentration of 1: 1000 dilutions for easy cell examination. The slides were Giemsa-stained and quantified under the microscope by counting 2000 total red blood cells (RBCs) according to WHO guidelines and distinguishing the number of infected and uninfected cells to determine parasitaemia. The slide reading results were recorded on an Excel sheet for further analysis.
Magnetic deposition microscopy (MDM)
Briefly, blood samples were diluted using PBS (pH = 7.2) in a ratio of 1:10 before pumping 500 µL of each test sample through the flow channels. Infected RBCs were collected and concentrated on a 0.13 mm-thick Mylar sheet (also known as polyester slide) by the magnet to ensure maximum late parasitic stage enrichment from five samples obtained from the five different flow channels. The blood samples for the MDM analysis were prepared and processed freshly in the field. Cells captured on the Mylar slide were fixed by 100 % methanol for 30 s and stained with 10 % Giemsa for 30 min. Once the slides dried, they were observed and analyzed under a light microscope at 100× magnification.
In vitro results
Three methods, LM, MDM and RDT were compared to detect P. falciparum infections in 303 school children. Amongst the P. falciparum positive individuals as detected by LM, RDT and MDM, 88.2, 93 and 89.8 %, respectively, had body temperature below 37.5 °C. However, body temperature had no statistical significant influence on the proportion of P. falciparum infections among the asymptomatic individuals.
Prevalence of Plasmodium falciparum all stages as determined by three diagnostic tests (LM, RDT and MDM) and gametocytes prevalence determined by LM and MDM only, in both cases n = 303
95 % CI
95 % CI
95 % CI
Comparison of sensitivity and specificity for the parasite detection between MDM, LM (part A1) and RDT (part A2) and comparison of sensitivity and specificity of gametocytes detection between MDM and LM (part B)
The prevalence of P. falciparum gametocytes was 1.3 % (4/303 95 % CI 0.4–3.3) by LM but was considerably higher and equal to 4 % (12/303 95 % CI 2.1–6.8) by the MDM (Table 1). The difference between the two methods in detection of gametocytes was statistically significant (p = 0.008). The sensitivity of the MDM to gametocyte detection was low 26.7 %, (95 % CI 0.6–80.5) but its specificity was high, 96.5 % (95 % CI 93.7–99.1) indicating that both tests do not differ significantly in specificity of gametocyte detection (Table 2B).
This study demonstrates that MDM could successfully detect sub-microscopic parasitaemia from asymptomatic school children. Overall, MDM showed an improved detection rate for the gametocytes by threefold compared to LM, important in areas where malaria is declining and gametocyte density has become a variable of interest . Sub-Saharan Africa has experienced a marked reduction of P. falciparum infection rates and parasitaemia levels, a situation that poses a serious challenge to the conventional malaria diagnostic tools, such as LM, to clearly estimate malaria burden . The MDM device from this study improved detection of parasitaemia and gametocytaemia compared to LM. This is not surprising as the MDM device used in this study was a modified version of the previous one used in PNG [8, 9], by using two-directional flow across the magnet for increased capture of iRBCs and it offers a convenient way on set up and operation for a day-to-day use.
The increased rate of gametocyte detection by MDM compared to LM is related to two factors: depletion of uninfected RBCs from the slide by the fluid flow and concentration of the infected RBCs (iRBCs) by the magnetic field in a small area of the slide covered by only a few microscope fields of view. In comparison, the LM preparation is smeared over a substantial part of the microscope slide surface and the iRBCs are diluted by the uninfected cells in the microscope field of view. This MDM deposition pattern can assist microscopists in locating iRBCs on the slide, hence contribute to more rapid evaluation of blood slides and reduction of slide reading time. Interestingly, the gametocyte enrichment rate (relative to LM) in vitro, 10× was higher than that determined for the asymptomatic children (3×). The responsible mechanism could be higher viscosity of the diluted blood from human subjects compared to the viscosity of the iRBCs culture media (not measured) increasing the loss of iRBCs from MDM slides. As MDM provides mature gametocyte counts in a given blood volume (50 µL), this enumeration strategy may help in studying the relationship between gametocyte density and mosquito infectivity. A number of field studies suggested that microscopic and sub-microscopic gametocytes from humans are infectious to mosquitoes [16, 29, 30]. Additionally, because MDM captures intact iRBCs on the microscope slide, it provides a convenient platform for cytochemical differentiation of species, species identification and stage-specific morphologic features analysis of the parasite.
This study involving asymptomatic school children from a low malaria transmission setting confirmed preliminary results from in vitro work showing that late stage parasites, microscopic and sub-microscopic gametocytes were susceptible to MDM capture. The results show that MDM increased detection of P. falciparum infection by 2.5-fold (19.5 % vs 7.6 %) and was more specific (87.5 %) over LM and RDT (89.0 %), although its sensitivity was almost similar to RDT. Comparable findings were reported in other studies [6, 8, 9, 31] although blood samples used in this study were from asymptomatic school children who are potentially reservoirs of gametocytes something which differs from other studies. Similarly, MDM detected three times more gametocytes compared to LM what indicate that P. falciparum gametocytes were usually underestimated by the current diagnostic tool, LM. Malaria infection underestimation by current diagnostic tools was also observed by the studies conducted in southeast Tanzania . Moreover, several other studies emphasized on the importance of detecting sub-microscopic gametocytes that occur below the detection limit as they perpetuate transmission when ingested by a female mosquito [17, 30, 33].
A significant challenge on management of malaria disease is an easy way of obtaining a reliable, simple and sensitive diagnosis. In many endemic areas LM remains the most available method  while in Tanzania, LM and RDT are the widely used as standards for malaria parasite confirmation and detection methods respectively. However, RDT has been used as a quick diagnostic test although its detection capacity is limited to ≥200 parasites per microlitres  and it is incapable of distinguishing sexual and asexual forms of the parasites. The familiarity with the LM use in the field, the higher sensitivity of MDM to gametocytaemia detection than that of LM (although operating on the same principle of microscopic examination) together with its ability to distinguish between sexual and asexual forms makes it an interesting potential addition tool in detecting sub-microscopic parasitaemia and accurately estimating the malaria burden in low malaria transmission settings. Moreover, the estimated equipment cost could be reduced to that of a commercial, high gradient magnetic separation (HGMS) column system in multiple column configuration but with significant savings on disposables as the material cost of MDM slides is cheaper compared to multiple US dollars for one HGMS column .
The MDM instrument used in this study was a laboratory prototype and, therefore, lacking the user-friendly features of operation. The study served an important purpose of identifying those features that would require simplification before the MDM device could be adopted for wider use in field studies. The other important consideration is that it relies on the presence of haemozoin to magnetically concentrate iRBCs on the slide leaving out uninfected RBCs, therefore absence of uninfected RBCs on the slide, increases detection of iRBCs.
The current instrument requires AC power for the syringe pump operation, conveniently supplied by DC-AC inverter or 12 V automobile battery. These could be miniaturized by taking advantage of increasing availability of small pumps for point of care laboratory medicine, including USB powered pumps (powered by laptop computer batteries) and solar panels or completely eliminated by redesigning the flow path for gravity-fed operation. The combination of magnetic separation and microfluidics of the MDM prototype coupled with its ability to distinguish low-level parasite stages, particularly gametocytes, makes it an ideal candidate for miniaturization to further reduce size, weight and minimize or eliminate power consumption. This improvement could make the instrument more user-friendly, cost-effective and hence attractive as a tool for malaria transmission in the laboratory and in the field.
MDM enhanced detection of sub-microscopic P. falciparum infections and estimation of gametocyte density compared to LM and the results were comparable to those determined by RDT. Gametocyte enrichment by MDM was threefold higher than LM, offering improvements in results turn-around time and detection of sub-microscopic gametocytes, a feature which cannot be accorded by RDTs. Rather than depending on blood smears alone, the reliable, simple and field-adaptable MDM system could be useful to investigators and clinical researchers working on transmission studies as well as routine diagnosis after modification and miniaturization. On the other hand, these findings could further provide information on gametocytes density levels from asymptomatic individuals that become infectious to mosquitoes in settings where malaria transmission is substantially decreasing.
MZ and KM conceived and designed the study. BTG contributed on the experimental design and supervised the in vitro part of the study. DS carried out data collection, laboratory experiments and performed the analysis of data. DB contributed to the preparation and conduct of in vitro part of the study. PG and JM supervised the work. MZ and LM designed the MDM device and assisted on the technical aspect of the study. DS, KM and PG drafted the manuscript, with assistance from other authors. All authors read and approved the final manuscript.
The authors are grateful to the community of Bagamoyo villages where the study was conducted, school-teachers, parents/guardians and the school children who participated in the study. In addition, we recognize the assistance from the Ifakara Heath Institute (IHI) team on field trips. We are also thankful to the clinicians for their support during the conduct of the study. We recognize the financial support from The Tanzania Commission for Science and Technology (COSTECH) through The Nelson Mandela African Institution for Science and Technology (NM-AIST) for the PhD study and highly appreciate additional resources from IHI and partial grant support from the US National Institutes of Health (NIH CA062349 through the Cleveland Clinic, Lerner Research Institute and Case Western Reserve University. The early input in developing the study from Dr. Georgina Humphreys, Dr. Peter A. Zimmerman, and helpful suggestions from Dr. Stefan Karl are greatly appreciated. Finally, we are grateful to ethical committees for permission to conduct this study.
The authors declare that they have no competing interests.
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- Zborowski M, Fuh CB, Green R, Baldwin NJ, Reddy S, Douglas T, et al. Immunomagnetic isolation of magnetoferritin-labeled cells in a modified ferrograph. Cytometry. 1996;24:251–9.View ArticlePubMedGoogle Scholar
- Ribaut C, Berry A, Chevalley S, Reybier K, Morlais I, Parzy D, et al. Concentration and purification by magnetic separation of the erythrocytic stages of all human Plasmodium species. Malar J. 2008;7:45.PubMed CentralView ArticlePubMedGoogle Scholar
- Ito A, Shinkai M, Honda H, Kobayashi T. Medical application of functionalized magnetic nanoparticles. J Biosci Bioeng. 2005;100:1–11.View ArticlePubMedGoogle Scholar
- Mornet S, Vasseur S, Grasset F, Veverka P, Goglio G, Demourgues A, et al. Magnetic nanoparticle design for medical applications. Prog Solid State Chem. 2006;34:237–47.View ArticleGoogle Scholar
- Butykai A, Orbán A, Kocsis V, Szaller D, Bordács S, Tátrai-Szekeres E, et al. Malaria pigment crystals as magnetic micro-rotors: key for high-sensitivity diagnosis. Sci Rep. 2013;3:1431.PubMed CentralView ArticlePubMedGoogle Scholar
- Zimmerman PA, Thomson JM, Fujioka H, Collins WE, Zborowski M. Diagnosis of malaria by magnetic deposition microscopy. Am J Trop Med Hyg. 2006;74:568–72.PubMed CentralPubMedGoogle Scholar
- Moore LR, Fujioka H, Williams PS, Chalmers JJ, Grimberg B, Zimmerman PA, et al. Hemoglobin degradation in malaria-infected erythrocytes determined from live cell magnetophoresis. FASEB J. 2006;20:747–9.PubMed CentralPubMedGoogle Scholar
- Karl S, David M, Moore L, Grimberg BT, Michon P, Mueller I, et al. Enhanced detection of gametocytes by magnetic deposition microscopy predicts higher potential for Plasmodium falciparum transmission. Malar J. 2008;7:66.PubMed CentralView ArticlePubMedGoogle Scholar
- Karl S, Davis TME, St-Pierre TG. A comparison of the sensitivities of detection of Plasmodium falciparum gametocytes by magnetic fractionation, thick blood film microscopy, and RT-PCR. Malar J. 2009;8:98.PubMed CentralView ArticlePubMedGoogle Scholar
- Moody A. Rapid diagnostic tests for malaria parasites. Clin Microbiol Rev. 2002;5:66–78.View ArticleGoogle Scholar
- Khatib RA, Killeen GF, Abdulla SMK, Kahigwa E, McElroy PD, Gerrets RPM, et al. Markets, voucher subsidies and free nets combine to achieve high bed net coverage in rural Tanzania. Malar J. 2008;7:98.PubMed CentralView ArticlePubMedGoogle Scholar
- Tacaids: Tanzania HIV/AIDS and Malaria Indicator Survey 2007–2008. TACAIDS, ZAC, NBS,OCGS, ICF Int. 2008;71–80.Google Scholar
- Tacaids: Tanzania HIV/AIDS and Malaria Indicator Survey 2011–12. TACAIDS, ZAC, NBS,OCGS, ICF Int. 2012.Google Scholar
- Babiker HA, Gadalla AA, Rantford-Cartwright LC. The role of asymptomatic P. falciparum parasitaemia in the evolution of antimalarial drug resistance in areas of seasonal transmission. Drug Resist Updat. 2013;16:1–9.View ArticlePubMedGoogle Scholar
- Geiger C, Agustar HK, Compaoré G, Coulibaly B, Sié A, Becher H, et al. Declining malaria parasite prevalence and trends of asymptomatic parasitaemia in a seasonal transmission setting in North-Western Burkina Faso between 2000 and 2009–2012. Malar J. 2013;12:27.PubMed CentralView ArticlePubMedGoogle Scholar
- Bousema T, Okell L, Felger I, Drakeley C. Asymptomatic malaria infections: detectability, transmissibility and public health relevance. Nat Rev Microbiol. 2014;12:833–40.View ArticlePubMedGoogle Scholar
- Lin JT, Saunders DL, Meshnick SR. The role of submicroscopic parasitemia in malaria transmission: what is the evidence? Trends Parasitol. 2014;30:183–90.PubMed CentralView ArticlePubMedGoogle Scholar
- Bousema T, Okell L, Shekalaghe S, Griffin JT, Omar S, Sawa P, et al. Revisiting the circulation time of Plasmodium falciparum gametocytes: molecular detection methods to estimate the duration of gametocyte carriage and the effect of gametocytocidal drugs. Malar J. 2010;9:136.PubMed CentralView ArticlePubMedGoogle Scholar
- Drakeley C, Sutherland C, Bousema JT, Sauerwein RW, Targett GAT. The epidemiology of Plasmodium falciparum gametocytes: weapons of mass dispersion. Trends Parasitol. 2006;22:424–30.View ArticlePubMedGoogle Scholar
- Bousema T, Drakeley C. Epidemiology and infectivity of Plasmodium falciparum and Plasmodium vivax gametocytes in relation to malaria control and elimination. Clin Microbiol Rev. 2011;24:377–410.PubMed CentralView ArticlePubMedGoogle Scholar
- Okell LC, Bousema T, Griffin JT, Ouédraogo AL, Ghani AC, Drakeley CJ. Factors determining the occurrence of submicroscopic malaria infections and their relevance for control. Nat Commun. 2012;3:1237.PubMed CentralView ArticlePubMedGoogle Scholar
- Ghani RA, Basco LK, Beier JC, Mahdy MAK. Inclusion of gametocyte parameters in anti - malarial drug efficacy studies : filling a neglected gap needed for malaria elimination. Malar J. 2015;14:413.PubMed CentralView ArticlePubMedGoogle Scholar
- MOHSW. National Malaria Control Program; Medium Term malaria Strategic Plan 2014–2020. 2014.Google Scholar
- WHO. Guidelines for the treatment of Malaria. Geneva: World Health Organization; 2015.Google Scholar
- WHO. Malaria Rapid Diagnostic Test Performance. Geneva: World Health Organization; 2012.Google Scholar
- WHO. Bench Aids for the diagnosis of malaria infections. Geneva: World Health Organization; 2000.Google Scholar
- Grimberg BT, Erickson JJ, Sramkoski RM, Jacobberger JW, Zimmerman PA. Monitoring Plasmodium falciparum growth and development by UV flow cytometry using an optimized Hoechst-thiazole orange staining strategy. Cytometry A. 2008;73:546–54.PubMed CentralView ArticlePubMedGoogle Scholar
- Bhatt S, Weiss DJ, Cameron E, Bisanzio D, Mappin B, Dalrymple U, et al. The effect of malaria control on Plasmodium falciparum in Africa between 2000 and 2015. Nature. 2015;526:207–15.View ArticlePubMedGoogle Scholar
- Churcher TS, Bousema T, Walker M, Drakeley C, Schneider P, Ouédraogo AL, et al. Predicting mosquito infection from Plasmodium falciparum gametocyte density and estimating the reservoir of infection. Elife. 2013;2013:1–12.Google Scholar
- Schneider P, Bousema JT, Gouagna LC, Otieno S, Van De Vegte-Bolmer M, Omar SA, et al. Submicroscopic Plasmodium falciparum gametocyte densities frequently result in mosquito infection. Am J Trop Med Hyg. 2007;76:470–4.PubMedGoogle Scholar
- Karl S, Laman M, Koleala T, Ibam C, Kasian B, N’Drewei N, et al. Comparison of three methods for detection of gametocytes in Melanesian children treated for uncomplicated malaria. Malar J. 2014;13:319.PubMed CentralView ArticlePubMedGoogle Scholar
- Mwingira F, Genton B, Kabanywanyi AM, Felger I. Comparison of detection methods to estimate asexual Plasmodium falciparum parasite prevalence and gametocyte carriage in a community survey in Tanzania. Malar J. 2014;13:433.PubMed CentralView ArticlePubMedGoogle Scholar
- Shekalaghe SA, Teun Bousema J, Kunei KK, Lushino P, Masokoto A, Wolters LR, et al. Submicroscopic Plasmodium falciparum gametocyte carriage is common in an area of low and seasonal transmission in Tanzania. Trop Med Int Health. 2007;12:547–53.View ArticlePubMedGoogle Scholar
- Karl S, Gurarie D, Zimmerman PA, King CH, St. Pierre TG, Davis TME. A sub-microscopic gametocyte reservoir can sustain malaria transmission. PLoS ONE. 2011;6:e20805.PubMed CentralView ArticlePubMedGoogle Scholar