- Open Access
A lab-on-chip for malaria diagnosis and surveillance
- Brian J Taylor1, 2,
- Anita Howell3,
- Kimberly A Martin1, 2,
- Dammika P Manage4,
- Walter Gordy3,
- Stephanie D Campbell3,
- Samantha Lam1, 2,
- Albert Jin1, 2,
- Spencer D Polley5,
- Roshini A Samuel1, 2,
- Alexey Atrazhev4,
- Alex J Stickel3,
- Josephine Birungi6,
- Anthony K Mbonye7, 8,
- Linda M Pilarski4,
- Jason P Acker3, 9 and
- Stephanie K Yanow1, 2Email author
© Taylor et al.; licensee BioMed Central Ltd. 2014
Received: 13 March 2014
Accepted: 1 May 2014
Published: 9 May 2014
Access to timely and accurate diagnostic tests has a significant impact in the management of diseases of global concern such as malaria. While molecular diagnostics satisfy this need effectively in developed countries, barriers in technology, reagent storage, cost and expertise have hampered the introduction of these methods in developing countries. In this study a simple, lab-on-chip PCR diagnostic was created for malaria that overcomes these challenges.
The platform consists of a disposable plastic chip and a low-cost, portable, real-time PCR machine. The chip contains a desiccated hydrogel with reagents needed for Plasmodium specific PCR. Chips can be stored at room temperature and used on demand by rehydrating the gel with unprocessed blood, avoiding the need for sample preparation. These chips were run on a custom-built instrument containing a Peltier element for thermal cycling and a laser/camera setup for amplicon detection.
This diagnostic was capable of detecting all Plasmodium species with a limit of detection for Plasmodium falciparum of 2 parasites/μL of blood. This exceeds the sensitivity of microscopy, the current standard for diagnosis in the field, by ten to fifty-fold. In a blind panel of 188 patient samples from a hyper-endemic region of malaria transmission in Uganda, the diagnostic had high sensitivity (97.4%) and specificity (93.8%) versus conventional real-time PCR. The test also distinguished the two most prevalent malaria species in mixed infections, P. falciparum and Plasmodium vivax. A second blind panel of 38 patient samples was tested on a streamlined instrument with LED-based excitation, achieving a sensitivity of 96.7% and a specificity of 100%.
These results describe the development of a lab-on-chip PCR diagnostic from initial concept to ready-for-manufacture design. This platform will be useful in front-line malaria diagnosis, elimination programmes, and clinical trials. Furthermore, test chips can be adapted to detect other pathogens for a differential diagnosis in the field. The flexibility, reliability, and robustness of this technology hold much promise for its use as a novel molecular diagnostic platform in developing countries.
Malaria is a blood-borne parasitic disease causing over 660,000 deaths each year, primarily in young children from sub-Saharan Africa . In the past decade, malaria control efforts have focused on scale-up interventions including use of insecticide treated bed nets, indoor residual spraying, rapid diagnostic tests and artemisinin-based combination therapy to reduce morbidity and mortality. Still, in countries bearing the largest malaria burden, access to quality diagnostics is limited [2, 3]. Microscopy, if available, is the gold standard for malaria diagnosis but in health centres with limited resources, malaria is diagnosed presumptively in patients with fever . These practices lead to overtreatment and misdiagnosis of potentially fatal bacterial infections and are becoming less feasible in the face of emerging drug resistance and costly new therapies [2, 5, 6]. As such, new diagnostic practices are urgently needed. Furthermore, as malaria control efforts intensify and countries progress to elimination phases, sensitive diagnostics will play a key role in surveillance to identify sporadic outbreaks and asymptomatic reservoirs of infection . Immunochromatographic rapid diagnostic tests (RDTs) provide an important alternative to microscopy at the point-of-care, but are not without significant limitations, including decreased sensitivity at lower levels of parasitaemia, inhibition at high levels of parasitaemia (prozone effect), inability to quantitate or distinguish malaria species in mixed infections, and failure to detect parasites with mutations in the genes encoding certain target antigens [4, 8, 9]. While strides have been made in improving RDT performance , nucleic acid based diagnostics, including PCR and isothermal amplification, provide superior sensitivity and specificity . However, the need for pre-analytic processing, cold storage, and expensive equipment has precluded the use of nucleic acid diagnostics in the field. Lab-on-chip platforms have shown promise in overcoming these barriers by adapting common laboratory tests to a self-contained, portable, micro-scale format targeted to the point-of-care . In this study, the development of a plastic hydrogel chip and a portable real-time PCR machine for malaria diagnosis is described.
Patient samples and controls
Archived, frozen samples from malaria patients with a positive diagnosis by PCR were acquired from the Provincial Laboratory for Public Health (ProvLab) in Edmonton, Alberta. The blind panel run on the Gelcycler was generated from samples collected in 2011–2012 in Uganda from consenting pregnant women participating in a study to genotype parasite resistance  (during antenatal care, at delivery and those with fever attending outpatient clinics). Blood (4 mL) was sampled by venipuncture, stored in EDTA vacutainers, and transferred to the Uganda Virus Research Institute for storage at −20°C. Thick smears were stained by Giemsa and malaria parasites counted against 200 leukocytes and expressed as number of parasites per μL of blood assuming a standard leukocyte count of 8,000/μL of blood. A smear was considered negative after examining a minimum of 100 high power fields with no parasites seen. Microscopy was performed by a laboratory technician at one of two health facilities in Mukono district. Coded samples were aliquoted and shipped frozen for testing in Alberta. Ethical approval was granted by the review boards at the Uganda Virus Research Institute and Uganda National Council for Science and Technology (Reference HS 747). Use of samples from ProvLab and the Ugandan study was approved by the Health Research Ethics Board at the University of Alberta.
The blind panel run on the Accutas comprised randomly chosen EDTA samples as positive and negative for malaria DNA that were submitted during the first seven months of 2011 for routine malaria diagnosis at the Department of Clinical Parasitology, Hospital for Tropical Diseases .
A nested PCR reaction  to amplify malarial DNA was performed on all these samples in addition to routine diagnosis by microscopy. All PCR positive samples were further characterized against the WHO International Standard for Plasmodium falciparum by a real-time PCR reaction . Once a definitive malaria diagnosis had been made for each sample the remainder were anonymized and stored as surplus to diagnostic requirements for use in ethically approved research projects. The panel consisted of positive samples infected with the following species: P. falciparum (n = 25), Plasmodium vivax (n = 2), Plasmodium ovale (n = 2), and Plasmodium malariae (n = 1). Parasitemia ranged from <5 to >1,000 parasites/μL blood. The panel also included eight negative samples.
Plasmodium knowlesi purified genomic DNA (Malaria Research and Reference Reagent Resource Center (MR4), Manassas, VA) was diluted to 2 ng/mL in non-infected blood to serve as a reference for this species. The negative control used in this study was a hemoglobin tri-level control, level 2 (Stanbio, Boerne, TX) diluted 1:10 in water. The positive control had the same composition as the negative, with the addition of a consensus PCR product to a final concentration of 105 copies/μL for hydrogel wax chips and 102 copies/μL for hydrogel plastic chips.
Plasmodium falciparum parasites were grown in human erythrocytes at 3-5% haematocrit as described . Ring stage parasites were enriched by sorbitol lysis , counted, and diluted in whole blood. The diluted parasites were frozen until use.
The hydrogel mastermix contains reagents described previously for direct amplification of DNA targets from blood  and reagents for forming a polyacrylamide gel. This mastermix was prepared with 1X Klentaq Buffer (containing 3.5 mM Mg2+; DNA Polymerase Technology, St. Louis, Mo), 40X SYBR Green I (Life Technologies, Grand Island, NY), 1X PCR Enhancer Cocktail (PEC-1) (DNA Polymerase Technology), 200 nM forward and reverse primers, 200 μM dNTPs, 0.03% BSA, 4% acrylamide (Sigma St. Louis, Mo), 0.4% bis-acrylamide aqueous solution (BioRad, Hercules, CA), 0.06% azobis (Wako, Richmond, VA), and 0.1% TEMED (Sigma). For a 100 μL mastermix volume, 3 μL of Omni KlenTaq enzyme was added (DNA Polymerase Technology). Both consensus PCR primers [15, 20], and species-specific primers [21, 22] target regions of the 18S rRNA gene of Plasmodium.
Hydrogel wax chips
A prototype consisting of a wax cassette in a 23.5 × 32 mm aluminum pan was created wherein the hydrogel is polymerized and desiccated on a coverslip above a wax-bound “trench”. A polydimethylsiloxane (PDMS) stamp was used to imprint 4 trenches in the wax. Three coverslips (20 mm × 5 mm) were placed equally spaced on top of the wax, perpendicular to the trenches, creating 12 covered slots for hydrogels. Coverslips were sealed onto the wax by briefly heating the surface of the coverslip between each trench with a soldering iron, allowing the wax underneath to melt slightly. A 13 μL aliquot of mastermix was added to each slot, creating a “gel strip”. The gel strip was photopolymerized at room temperature under UV light (367 nm) for 30 minutes. Polymerized gels were desiccated under vacuum (23 inHg) for 1 hour at room temperature and used within seven days. Chips were stored in dark conditions to prevent photo-bleaching of SYBR green dye. Coverslips were treated with 3-(trimethoxysilyl)propyl methacrylate to promote adherence to the gel strip as described . On desiccation, the gel shrinks away from the trench and stays attached to the coverslip, creating a channel underneath the strip where the sample can diffuse in. Whole blood was diluted 1:10 with water, then 8.5 μL of this sample mixture was applied underneath the coverslip/gel-strip. After the addition of samples and controls, the wax cassette was incubated for 10 minutes at room temperature then placed directly on the Peltier element within the Gelcycler for thermocycling.
Hydrogel plastic chips
Plastic chips were manufactured by miniFAB (Scoresby, Australia) by injection molding of cyclic olefin polymer (COP1420R) into top (27 × 27 mm) and bottom pieces (27 × 42 mm). To form the hydrogels, a 15 μL aliquot of mastermix was first added to the wells in the top piece. Next, the top piece was placed in a customized UV illumination chamber and flooded with nitrogen for 2 minutes. The gel was photopolymerized at room temperature under UV light (405 nm) for 30 minutes. The chamber was flooded with nitrogen a second time for 2 minutes, halfway into the UV treatment. This sustained nitrogen overlay was needed to prevent oxygen from inhibiting gel polymerization. The polymerized gels were desiccated under vacuum (23 inHg) at least 20 hours at room temperature. To complete the process of making a chip, a 10 μL aliquot of wax was added to each reservoir in the bottom piece, and the top and bottom pieces were fitted together. Wax in the bottom reservoir melts during thermocycling to cover the gel and sample ports, preventing evaporation and further cross-contamination that may occur at high denaturation temperatures. A two-sided tape adhesive on the bottom piece seals the chip upon assembly and prevents cross-contamination between gel chambers. The assembled plastic chips were used within 24 hours of preparation, or vacuum-sealed in plastic, stored at room temperature (22°C) in the dark, and tested within one month. With this design, sample added via the sample port in the top piece enters the lower reservoir and rehydrates the gel in the well. However, to ensure efficient loading of the sample in the validation experiments presented here, 8.5 μL of whole blood diluted 1:10 in water was added directly to the gel in the well before assembly of the chip. Samples were incubated prior to thermocycling as described above. As opposed to the wax chips, which sit freely on the Gelcycler Peltier element, the plastic chips were secured onto the Peltier with a gantry to ensure evenly distributed thermal transfer.
Instrumentation: Gelcycler and Accutas
The Gelcycler features a Peltier element for sample heating, components for stringent thermal regulation, a laser and CCD camera for capturing fluorescence . Consensus PCR reactions for the hydrogel wax chip were performed with a 10 minute initial denaturation step at 94°C, followed by 40 cycles of 94°C for 20 seconds, 58°C for 30 seconds, 72°C for 30 seconds, and a 2 minute final extension of 72°C. Reaction conditions for the hydrogel plastic chips were the same as above, except the consensus PCR annealing temperature was 60°C, and the species-specific annealing temperature was 64°C. MCA from 70-90°C was performed immediately after PCR. Fluorescent images were obtained and analysed as described  to generate real-time PCR and MCA curves using in-house software that requires manual analysis. A five-parameter sigmoid curve-fitting method using the first derivative was created to calculate cycle threshold (Ct) values. Samples were considered positive if they had a Ct value of less than 40 and the expected MCA peak profile. Conventional real-time PCR confirmation was performed on panel samples as described in Taylor et al. . The Accutas system refines the Gelcycler and brings many improvements. The modular design incorporates Design for Manufacturing principles to enable low cost, high volume manufacturing of the system. The Accutas system includes an LED light source rather than a laser-based system, allowing lower power and safer operation. The temperature-controlled environment allows the Accutas to be run in a wider window of temperatures. The temperature control of the Accutas was optimized and is easily adaptable to new designs. The new aluminum framed enclosure is more rugged for transport in the field. The PC control software was rewritten as well to provide an easier, step-by-step user interface with automated reporting at the end of each experiment.
Analyses were performed using SAS/STAT 9.1. Confidence intervals (95%) were calculated using the Wilson score interval method.
Test performance in prototype hydrogel chips
Manufactured plastic chips for hydrogel PCR
In the next phase of chip development, an enclosed plastic chip was designed that retained the key features of the prototype wax chip and could be manufactured on a large scale for use in the field (Figure 1C). The thermal properties and auto-fluorescence of several types of plastics were assessed and cyclic olefin polymer (COP1420R) proved most compatible with real-time PCR. The top piece of the chip was molded with 10 individual wells: eight test wells and two controls. Two ports for sample delivery are present on either side of each well. The hydrogel mixture was added to each well, polymerized and desiccated. A bottom piece of plastic was created with reservoirs that align with the sample ports and wells of the top piece. When the two pieces are adhered, they form an enclosed chip with channels for sample delivery, similar in concept to the hydrogel wax chip. The assembled plastic chips are easily packaged and stored. Blood samples were simply diluted in water for lysis (2 μL of blood added to 18 μL of water) and 8.5 μL was added to the hydrogel on the chip. This corresponds to approximately 0.85 μL of the original blood sample. To ensure accuracy in the current study, samples were added to each hydrogel prior to chip assembly. Positive and negative controls were included in each chip to ensure on-board quality control for the reagents and amplification reactions (Additional file 2).
Test performance in plastic chips
Validation of plastic chips
Demographic and clinical characteristics of patients included in the blind panel from Uganda (n = 188)
Median age [range]
20 years [14 – 42]
Asymptomatic (n [%])
Clinical malaria (n [%])
In antenatal care (n [%])
At delivery (n [%])
Median parasitemia [range]
440 parasites/μL [1 – 94800]
Performance characteristics of the hydrogel plastic chip compared with microscopy and conventional real-time PCR
Sensitivity* (95% CI)
Specificity* (95% CI)
Kappa (95% CI)
96.5% (92.0 – 98.5)
63.0% (48.6 – 75.5)
0.653 (0.521 – 0.785)
Conventional real-time PCR
97.4% (93.5 – 99.0)
93.8% (79.9 – 98.3)
0.890 (0.803 – 0.976)
Malaria speciation on plastic chips
Development and validation of a field-ready device
Third party assessment of the Accutas (n = 38)
Sensitivity (95% CI)
Specificity (95% CI)
Kappa (95% CI)
96.7% (83.3 – 99.4)
100% (67.6 – 100.0)
0.924 (0.778 – 1.000)
Accessible, quality diagnostics with low infrastructure requirements are expected to profoundly impact public health and child mortality from malaria . They also support new ‘test-before-treat’ policies to curb the emergence of drug-resistant parasites and discourage presumptive diagnosis based on fever [27, 28]. Highly sensitive molecular technologies exist with the potential to meet this critical need [8, 11], yet few have overcome the barriers of sample preparation, cold storage, cost, complexity and infrastructure requirements for use in low-resource settings . The recent clinical evaluation of a commercial loop-mediated isothermal amplification (LAMP) kit that amplifies parasite DNA with minimal extraction steps addresses many of these issues and demonstrates that molecular testing in the field is feasible [14, 30, 31]. However, while the innovations present in field-ready LAMP kits are commendable, a separate sample preparation process is still a necessary part of the procedure. This step, even in streamlined self-contained form provided by commercial kits, can be a significant barrier to implementation of a diagnostic test in resource-limited areas.
In this work a PCR-based diagnostic for malaria intended for use at or near the point-of-care is presented. The platform consists of hydrogel chips run on a customized portable real-time PCR machine. The hydrogel chips are disposable, do not require a cold-chain, and can be stored and used on demand for a result in less than two hours. PCR performed directly with unprocessed blood eliminates a major obstacle to adopting this technology outside of reference or research labs, and simplifies the testing for unskilled users. The entire system was designed to be low-cost for use in developing countries. The chips use small volumes of master mix (15 μL per test), and the material cost for the chips will be further reduced to under $1 USD per test with scaled production. Through innovative engineering and with mass production, the real-time PCR instrument can be manufactured for less than $2,000 USD. Quality optics constitutes the major share of component costs, but is essential to maintain sensitive fluorescence detection. The instrument is designed to operate on 12 V which can be supplied by a variety of power sources include the grid, dry cells, generators or photovoltaic systems. The amount of power required to run the device is equivalent to a car battery, which can be used to power the device in field settings where the supply of electricity is unstable. In the next generation of the platform, direct loading of the chip and a battery-operated instrument that provides a result within an hour will fully adapt the technology to the constraints of the field.
The technology described in this study has the potential to make major inroads by supporting key areas of malaria control: as a diagnostic for acute malaria, for surveillance in elimination settings, and as a tool in clinical evaluations of new drugs and vaccines. Importantly, there are numerous applications of this technology beyond malaria. The platform has the inherent flexibility to detect any molecular target simply by using different PCR primers in the hydrogel mix. This marks an important advantage over other approaches, such as LAMP, that require extensive primer validation. Tests for other disease targets in different specimen types are readily adapted to our platform, for example, sexually transmitted infections (STI) detected from urine and genital swabs . Furthermore, as shown here with malaria species, and separately for STI targets , a single patient sample could be tested for multiple targets simultaneously, providing a rapid differential diagnosis. Chips can be tailored to test for different pathogens, species, or genetic markers (including drug resistance markers), depending on the clinical or public health need. In summary, this work showcases a novel molecular technology that can make an important contribution to the diagnosis and surveillance of infectious diseases in low-resource settings.
This work was funded by an Interdisciplinary Team Grant from Alberta Innovates - Health Solutions and a Phase I Rising Stars Award from Grand Challenges Canada.
- WHO: World Malaria Report. 2012, Geneva: World Health Organization, 1-195.Google Scholar
- Amexo M, Tolhurst R, Barnish G, Bates I: Malaria misdiagnosis: effects on the poor and vulnerable. Lancet. 2004, 364: 1896-1898.View ArticlePubMedGoogle Scholar
- Rafael ME, Taylor T, Magill A, Lim YW, Girosi F, Allan R: Reducing the burden of childhood malaria in Africa: the role of improved. Nature. 2006, 444 (Suppl 1): 39-48.View ArticlePubMedGoogle Scholar
- Murray CK, Gasser RA, Magill AJ, Miller RS: Update on rapid diagnostic testing for malaria. Clin Microbiol Rev. 2008, 21: 97-110.PubMed CentralView ArticlePubMedGoogle Scholar
- Breman JG, Alilio MS, Mills A: Conquering the intolerable burden of malaria: what's new, what's needed: a summary. Am J Trop Med Hyg. 2004, 71: 1-15.PubMedGoogle Scholar
- O'Dempsey TJ, McArdle TF, Laurence BE, Lamont AC, Todd JE, Greenwood BM: Overlap in the clinical features of pneumonia and malaria in African children. Trans R Soc Trop Med Hyg. 1993, 87: 662-665.View ArticlePubMedGoogle Scholar
- mal ERACGoD, Diagnostics: A research agenda for malaria eradication: diagnoses and diagnostics. PLoS Med. 2011, 8: e1000396-View ArticleGoogle Scholar
- Erdman LK, Kain KC: Molecular diagnostic and surveillance tools for global malaria control. Travel Med Infect Dis. 2008, 6: 82-99.View ArticlePubMedGoogle Scholar
- Maltha J, Gillet P, Jacobs J: Malaria rapid diagnostic tests in endemic settings. Clin Microbiol Infect. 2013, 19: 399-407.View ArticlePubMedGoogle Scholar
- WHO: Malaria Rapid Diagnostic Test Performance. Results of the WHO Product Testing of Malaria RDTs: Round 4. 2012, Geneva: World Health Organization, 140-Google Scholar
- Cordray MS, Richards-Kortum RR: Emerging nucleic acid-based tests for point-of-care detection of malaria. Am J Trop Med Hyg. 2012, 87: 223-230.PubMed CentralView ArticlePubMedGoogle Scholar
- Chin CD, Linder V, Sia SK: Lab-on-a-chip devices for global health: past studies and future opportunities. Lab Chip. 2007, 7: 41-57.View ArticlePubMedGoogle Scholar
- Mbonye AK, Birungi J, Yanow S, Magnussen P: Prescription patterns and drug use among pregnant women with febrile Illnesses in Uganda: a survey in out-patient clinics. BMC Infect Dis. 2013, 13: 237-PubMed CentralView ArticlePubMedGoogle Scholar
- Polley SD, Gonzalez IJ, Mohamed D, Daly R, Bowers K, Watson J, Mewse E, Armstrong M, Gray C, Perkins MD, Bell D, Kanda H, Tomita N, Kubota Y, Mori Y, Chiodini PL, Sutherland CJ: Clinical evaluation of a loop-mediated amplification kit for diagnosis of imported malaria. J Infect Dis. 2013, 208: 637-644.PubMed CentralView ArticlePubMedGoogle Scholar
- Snounou G, Viriyakosol S, Zhu XP, Jarra W, Pinheiro L, do Rosario VE, Thaithong S, Brown KN: High sensitivity of detection of human malaria parasites by the use of nested polymerase chain reaction. Mol Biochem Parasitol. 1993, 61: 315-320.View ArticlePubMedGoogle Scholar
- Shokoples SE, Ndao M, Kowalewska-Grochowska K, Yanow SK: Multiplexed real-time PCR assay for discrimination of Plasmodium species with improved sensitivity for mixed infections. J Clin Microbiol. 2009, 47: 975-980.PubMed CentralView ArticlePubMedGoogle Scholar
- Trager W, Jensen JB: Human malaria parasites in continuous culture. Science. 1976, 193: 673-675.View ArticlePubMedGoogle Scholar
- Lambros C, Vanderberg JP: Synchronization of Plasmodium falciparum erythrocytic stages in culture. J Parasitol. 1979, 65: 418-420.View ArticlePubMedGoogle Scholar
- Taylor BJ, Martin KA, Arango E, Agudelo OM, Maestre A, Yanow SK: Real-time PCR detection of Plasmodium directly from whole blood and filter paper samples. Malar J. 2011, 10: 244-PubMed CentralView ArticlePubMedGoogle Scholar
- Kamau E, Tolbert LS, Kortepeter L, Pratt M, Nyakoe N, Muringo L, Ogutu B, Waitumbi JN, Ockenhouse CF: Development of a highly sensitive genus-specific quantitative reverse transcriptase real-time PCR assay for detection and quantitation of Plasmodium by amplifying RNA and DNA of the 18S rRNA genes. J Clin Microbiol. 2011, 49: 2946-2953.PubMed CentralView ArticlePubMedGoogle Scholar
- de Monbrison F, Angei C, Staal A, Kaiser K, Picot S: Simultaneous identification of the four human Plasmodium species and quantification of Plasmodium DNA load in human blood by real-time polymerase chain reaction. Trans R Soc Trop Med Hyg. 2003, 97: 387-390.View ArticlePubMedGoogle Scholar
- Arango EM, Samuel R, Agudelo OM, Carmona-Fonseca J, Maestre A, Yanow SK: Molecular detection of malaria at delivery reveals a high frequency of submicroscopic infections and associated placental damage in pregnant women from Northwest Colombia. Am J Trop Med Hyg. 2013, 89: 178-183.PubMed CentralView ArticlePubMedGoogle Scholar
- Atrazhev A, Manage DP, Stickel AJ, Crabtree HJ, Pilarski LM, Acker JP: In-gel technology for PCR genotyping and pathogen detection. Anal Chem. 2010, 82: 8079-8087.View ArticlePubMedGoogle Scholar
- Manage DP, Lauzon J, Atrazev A, Chavali R, Samuel RA, Chan B, Morrissey YC, Gordy W, Edwards AL, Larison K, Yanow SK, Acker JP, Zahariadis G, Pilarski LM: An enclosed in-gel PCR amplification cassette with multi-target, multi-sample detection for platform molecular diagnostics. Lab Chip. 2013, 13: 2576-2584.View ArticlePubMedGoogle Scholar
- Manage DP, Lauzon J, Atrazhev A, Pang X, Pilarski LM: A novel method for sample delivery and testing of whole blood: gel strip PCR for point of care (POC) molecular diagnostics. Lab Chip. 2013, 13: 4011-4014.View ArticlePubMedGoogle Scholar
- Hall N, Gardner M: Malaria Parasites: Genomes and Molecular Biology. 2004, Norfolk, England: Caister Academic PressGoogle Scholar
- WHO: Guidelines for the Treatment of Malaria. 2010, Geneva: World Health Organization, 2Google Scholar
- Perkins MD, Bell DR: Working without a blindfold: the critical role of diagnostics in malaria control. Malar J. 2008, 7 (Suppl 1): S5-PubMed CentralView ArticlePubMedGoogle Scholar
- Yager P, Domingo GJ, Gerdes J: Point-of-care diagnostics for global health. Annu Rev Biomed Eng. 2008, 10: 107-144.View ArticlePubMedGoogle Scholar
- Hopkins H, Gonzalez IJ, Polley SD, Angutoko P, Ategeka J, Asiimwe C, Agaba B, Kyabayinze DJ, Sutherland CJ, Perkins MD, Bell D: Highly sensitive detection of malaria parasitemia in an endemic setting: Performance of a new LAMP kit in a remote clinic in Uganda. J Infect Dis. 2013, 208: 645-652.PubMed CentralView ArticlePubMedGoogle Scholar
- Sirichaisinthop J, Buates S, Watanabe R, Han ET, Suktawonjaroenpon W, Krasaesub S, Takeo S, Tsuboi T, Sattabongkot J: Evaluation of loop-mediated isothermal amplification (LAMP) for malaria diagnosis in a field setting. Am J Trop Med Hyg. 2011, 85: 594-596.PubMed CentralView ArticlePubMedGoogle Scholar
This article is published under license to BioMed Central Ltd. This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/4.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly credited. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.