Journal of Immunology Research

Journal of Immunology Research / 2015 / Article
Special Issue

Cellular Immunity-Pathogen Interactions in Infectious Diseases

View this Special Issue

Research Article | Open Access

Volume 2015 |Article ID 162639 |

James M. Colborn, Joni H. Ylöstalo, Ousmane A. Koita, Ousmane H. Cissé, Donald J. Krogstad, "Human Gene Expression in Uncomplicated Plasmodium falciparum Malaria", Journal of Immunology Research, vol. 2015, Article ID 162639, 10 pages, 2015.

Human Gene Expression in Uncomplicated Plasmodium falciparum Malaria

Academic Editor: Muhammad Abubakar
Received13 Nov 2014
Revised30 Dec 2014
Accepted02 Jan 2015
Published30 Sep 2015


To examine human gene expression during uncomplicated P. falciparum malaria, we obtained three samples (acute illness, treatment, and recovery) from 10 subjects and utilized each subject’s recovery sample as their baseline. At the time of acute illness (day 1), subjects had upregulation of innate immune response, cytokine, and inflammation-related genes (IL-1, IL-6, TNF, and IFN-), which was more frequent with parasitemias 100,000 per L and body temperatures 39C. Apoptosis-related genes (Fas, BAX, and TP53) were upregulated acutely and for several days thereafter (days 1–3). In contrast, the expression of immune-modulatory (transcription factor 7, HLV-DOA, and CD6) and apoptosis inhibitory (c-myc, caspase 8, and Fas Ligand G) genes was downregulated initially and returned to normal with clinical recovery (days 7–10). These results indicate that the innate immune response, cytokine, and apoptosis pathways are upregulated acutely in uncomplicated malaria with concomitant downregulation of immune-modulatory and apoptosis inhibitory genes.

1. Introduction

Malaria is caused by intracellular protozoa of the genus Plasmodium [1]. Each year 300 million to 3 billion people are infected and more than 600,000 die, making malaria the most important vector-borne disease in the world [2]. Of the five parasites that infect humans (P. falciparum, P. vivax, P. malariae, P. ovale, and P. knowlesi), P. falciparum causes the most severe disease and the most morbidity and mortality [3]. Its manifestations range from asymptomatic to fatal infection [4, 5] and there are major gaps in our understanding of its pathogenesis [6] and the changes in gene expression responsible for the host response that are the focus of this study [7, 8].

Previous studies have shown that humans with malaria release proinflammatory mediators, such as tumor necrosis factor (TNF), interferon gamma (IFN-γ), and nitric oxide (NO), which may damage organs such as brain, lung, and kidney [5], and suggest that the levels of these mediators are related to the severity of disease [913]. Potential parasite virulence factors include the glycolipids that anchor parasite proteins to the red cell surface [14, 15], var genes [16, 17], and hybrid sequences in parasite proteins on the surface of parasitized red blood cells (Block 2 region of merozoite surface protein 1 [OA Koita: personal communication]).

However, until now, it has been difficult to study host gene expression in malaria because methods available could examine only a few genes at a time (Northern blots, reverse transcriptase PCR). In contrast, cDNA [18] and oligonucleotide microarrays [19, 20] permit examination of the entire human transcriptome. To examine host gene expression in malaria, it was necessary to examine and resolve (1) effects of ambient temperatures > 45°C on RNA stability, (2) transport of RNA preparations from malarious areas to the U.S., (3) potential confounding by host genomic differences and host variation in gene expression, (4) the effects of antimalarial treatment on host gene expression, and (5) potential false-positive and false-negative microarray results.

2. Methods

2.1. Blood Collection and RNA Isolation

Venous blood samples (3 mL) were drawn from children 3–16 years of age with uncomplicated malaria and transferred to tubes containing Ficoll-Hypaque (CPT Tube 362760, Becton Dickinson). After centrifugation at 1,500 g for 20 min at room temperature, peripheral blood mononuclear cells (PBMCs) formed a 1-2 mm layer 5 mm above the gel separator which was aspirated manually (Samco Pipet 335, San Fernando, CA), mixed with 1.3 mL RNAlater (Ambion, Austin, TX), and stored at 0°C (ice-water bath). Within 2 hours, RNA was isolated from this suspension using the RiboPure-Blood kit (Ambion).

2.2. RNA Quality

Was assessed by agarose gel (Figure 1) and OD 260/280 ratios in Mali. Samples with distinct 18S and 28S bands on agarose gel and OD 260/280 ratios ≥ 1.7 were stored in sodium acetate : ethanol (0.1 vol 3 M sodium acetate, [pH 5.2] : 2.5 vol 98% ethanol) at −20°C until transport to New Orleans where they were stored at −20°C for ≤ 4 weeks. RNA was purified by ethanol precipitation, followed by cleanup with the RNeasy Kit (Qiagen). RNA was then reexamined using the RNA 6000 Nano Marker Green kit (25–6,000 nt standards, Ambion) and the 2100 Bioanalyzer (Agilent Technologies, Waldbronn, GERMANY) to identify 18S and 28S ribosomal peaks on the electropherogram and estimate the RNA Integrity Number (RIN) [21]. Samples with well-defined 18S and 28S peaks on the electropherogram, ≥1.0 μg RNA, and RINs ≥ 6.5 were converted to biotinylated cRNA and hybridized (Figure 1).

2.3. Conversion of mRNA to Double-Stranded Biotinylated cRNA

Double-stranded cDNA was synthesized using the Superscript system (Invitrogen), purified by phenol : chloroform extraction, and concentrated by ethanol precipitation. In vitro transcription was used to produce biotin-labeled cRNA (GeneChip In Vitro Transcription Labeling Kit, Affymetrix).

2.4. Microarray Hybridization

Biotinylated cRNA was cleaned (RNeasy), fragmented, and hybridized on HG-U133 Plus 2.0 chips (Affymetrix). Each chip had > 54,000 probe sets for > 38,000 human genes [22]. After washing, chips were stained with streptavidin-phycoerythrin, amplified with biotinylated anti-streptavidin (Vector Laboratories), and scanned for fluorescence (GeneChip Scanner 3000) using the GeneChip Operating software, version 1.0 (GCOS).

2.5. Microarray Data Processing

Fluorescence intensities for perfect match (PM) and mismatch (MM) nucleotides were used to determine whether mRNA for specific genes was present (P), marginally present (M) or absent (A). Scanned images were transferred to dChip [2325] and corrected for image discontinuities. To compare results across chips, one array was chosen as baseline (147C, median intensity 167) to which others were normalized by calculating expression values based on PMs and MMs. Negative results were assigned a value of one.

2.6. Filtering

Was performed to identify genes with changes in expression between (1) acute illness (A) and recovery (C), (2) acute illness (A) and treatment (B), or (3) treatment (B) and recovery (C) based on ≥ 90% confidence in a ≥ 1.5-fold change in fluorescence (p < 0.01) and a P-call ≥ 70% for samples with up- or downregulation. Samples were permuted 100 times to estimate the false discovery rate which was 0.0% (median), 90% CI: 16.4–25.2%. The three sets of genes were then combined by removing duplicate genes and genes with redundant probe sets.

2.7. Hierarchical Clustering in dChip

Expression values were standardized by adjusting samples linearly to a mean of zero with a standard deviation of one and by determining correlation coefficients ( values) for normalized expression (intergenic distances defined as ). Genes with the shortest distances between them were merged into supergenes, connected in dendrograms using lengths proportional to genetic distance (centroid-linkage), and repeated times to cluster all genes. A similar algorithm was used to cluster the samples [26, 27].

2.8. Gene Ontologies

Five patterns of expression on the heat maps were examined for Gene Ontology (GO) term enrichment [28] across the entire microarray by using the exact hypergeometric distribution (significant values < 0.01).

2.9. Filtering Based on Parasitemia and Temperature (Table 1)

Age (years) Sex (M, F) Temperature (°C) Parasitemia (per μL)

11M 40.029,525

Uninfected controls
6M36.20 (Neg)
4M37.20 (Neg)
7F36.70 (Neg
7F36.80 (Neg)
2M36.00 (Neg)

Was based on acute illness samples and used analysis of variance ( values ≤ 0.01 and P-calls ≥ 20%); hierarchical clustering was used to identify patterns of expression and to test for GO term enrichment.

2.10. Pathway Analysis and Filtering

Identified genes with differences in expression between acute illness and recovery based on (1) ≥ 90% confidence in ≥ 2-fold changes in expression (up or down) and (2) P-calls of 100% for the samples in which genes were up- or downregulated.

2.11. Samples from Uninfected Controls

Included 4 subjects who received chloroquine and one who received placebo (5% dextrose in saline). After normalization based on sample 2405A (median intensity 153), cRNA from these subjects was analyzed similarly using dChip.

2.12. Microarray Target Validation

Was performed with TaqMan low density arrays using cDNA prepared from total RNA (iScript kit, Bio-Rad), loaded in low density cards, and run on an ABI 7900 HT real-time thermocycler using 50–100 ng cDNA per well. Data were normalized using endogenous 18S cDNA as the control to calculate fold changes between samples with 95% CIs for genes with valid threshold cycle data for 3 or more of 4 replicates (based on acute illness or recovery samples). Genes with changes in expression that overlapped the baseline sample (based on the 95% CI) were excluded from the subsequent analyses.

2.13. Subject Identification, Informed Consent, and Study Design

Identification of infected subjects was performed at the Banconi Clinic in Bamako using Giemsa-stained thick blood smears, a positive parasite antigen test, and PCR for the polymorphic Block 2 region of msp1 [29]. Informed consent was obtained before enrollment from the parents or guardians of children with uncomplicated P. falciparum malaria using a protocol approved by the Mali IRB in Bamako and the Tulane IRB in New Orleans. To control for host genomic variation and variation in gene expression, three samples were obtained from each subject (Figure 1): (1) an acute sample at the time of diagnosis on day 1 before beginning treatment (A), (2) a treatment sample on day 3 or 4 after completion of the 3-day course of treatment (B), and (3) a recovery sample 7–10 days after treatment (C, no signs or symptoms of malaria, no asexual parasites on the thick smear). The recovery sample served as the baseline to which the other samples were compared to identify changes from baseline (normal) gene expression. Relevant clinical data, including parasitemia and temperature (Table 1), were obtained at the time of diagnosis and during follow-up visits.

To control for the effects of antimalarials on gene expression, uninfected healthy controls were identified in the village of Missira in the Kolokani District (160 km NW of Bamako) based on a negative Giemsa-stained thick smear, negative parasite antigen test, and the absence of symptoms or signs of malaria. After obtaining consent, these subjects were enrolled in the study and randomized to receive either chloroquine or placebo (5% dextrose in saline).

3. Results

3.1. Examination of Gene Expression Profiles

Identified three sets of genes with ≥1.5-fold changes between (1) acute illness and treatment (), (2) acute illness and recovery (), or (3) treatment and recovery (). These three sets of genes () contained 219 unique genes, which were reduced to 182 by removing redundant probes. Conversely, when these criteria were used with samples from uninfected controls, only one gene was identified, indicating that antimalarial treatment produced no identifiable changes in gene expression. Gene expression patterns in the treatment and recovery groups (B and C) clustered closest to each other, with the acute illness group (A) being most distant. However, those patterns were not observed with the uninfected controls. Hierarchical clustering indicated that the uninfected controls were most similar to the recovery samples (C) and thus the recovery samples provided an accurate profile of gene expression in healthy subjects.

Hierarchical clustering of these 182 genes identified five expression profiles, four of which were linked to Gene Ontology (GO) categories such as host immune response or apoptosis (Figure 2). These four profiles included (1) genes upregulated during acute illness (A), (2) genes upregulated during both acute illness and treatment (AB), (3) genes upregulated during both treatment and recovery (BC) and (4) genes upregulated only at the time of recovery (C). The fifth profile (B), which contained genes upregulated only during treatment, was not included in the subsequent analyses because those genes were scattered across Gene Ontology categories.

Expression profile A (79 upregulated genes, 65 in 41 GO categories) included genes involved in the innate immune response, effector cell activation, and chemotaxis: leukocyte immunoglobulin-like receptor (LIR) family, neutrophil/monocyte/macrophage chemotactic chemokine receptor-like 2 (CCRL2), toll-like receptor 5 (TLR-5), aquaporin 9, complement component receptor C3AR1, acute-phase cytokine IL-6, and the IL-1β receptor antagonist.

Expression profile AB (44 upregulated genes, 41 in 25 GO categories) included genes involved in the immune response, apoptosis, and cell death. Immune response genes included complement components C1qA, C1qB, C1qG, and C2, chemokine ligand CXCL16, and Fc III γ-receptors CD16a and CD16b. Upregulated apoptosis- and cell death-related genes included BCL2-related X-protein (BAX), BH3 interacting domain death agonist (BID), baculoviral IAP repeat-containing 5 (survivin), and caspase 5.

Expression profile BC (7 upregulated genes, 7 in 13 GO categories) included genesinvolved in cellular development and the response to injury such as myosin regulatory protein MYL9, bone morphogenic protein 6, thrombospondin 1, and the oxytocin receptor.

Expression profile C (31 upregulated genes, 27 in 7 GO categories) includedgenes upregulated at recovery (10–14 days after acute illness) such as human leukocyte antigens HLA-DOA and HLA-DOB, transcription factor 7, CD6, CD1C antigen, and the Fc IgE receptor, FCER1A.

3.2. Pathways (Gene Networks) Involved in Uncomplicated P. falciparum Malaria

Based on pathway analyses, a number of cytokine and inflammatory response genes were upregulated, including IL-6, IL-10, IL-1β, and TNF (Figure 3). Examination of the apoptosis pathway (Figure 4) demonstrated simultaneous upregulation of genes that facilitate apoptosis (BAX, NF-κ1B, TNF SF10, Gzm B, and TNF) and concomitant downregulation of genes that inhibit apoptosis (c-Myc, TNF R SF25, IRF4, KBBKG, caspase 8, and Fas Ligand G).

3.3. Pathway Analyses Based on Parasitemia and Temperature

Identified 55 genes based on parasitemia and 21 based on temperature. GenMAPP analyses revealed differences in the inflammatory and apoptosis pathways between subjects with low parasitemias and subjects with medium or high parasitemias. Within the inflammatory, immune response, and host response pathways, the differences were most striking for acute phase mediators such as IFN-γ, IL-1α, IL-1β, IL-6, IL-7, IL-10, IL-15, and TNF (Figures 3(a)-3(b)). Within the apoptosis pathway, the differences were most striking for TP53 (p53), Fas, Fas Ligand, MCL1, caspases 6, 8, and 10, TNF, and TNFSF10B and 25 (Figures 4(a)-4(b)). Similar results were obtained with increasing body temperature (data not shown).

3.4. Upregulation of the Inflammatory and Apoptosis Pathways with Higher Parasitemias

Was identified with ANOVA using Kruskal-Wallis. Similar upregulation was observed in subjects with elevated temperatures (< 39°C versus ≥39°C, data not shown).

3.5. Microarray Validation Using Low Density Arrays

Quantitative real-time PCR using TaqMan low density arrays demonstrated excellent correlations between the changes observed in the microarrays and low density arrays. The magnitudes of changes (fold increase or decrease) in gene expression in the inflammatory response and apoptosis pathways varied similarly with parasitemia in both the microarrays (Figures 3-4) and the low density arrays (data not shown).

4. Discussion

4.1. Study Design, Obstacles, and Potential Confounders

The effects of ambient temperatures > 45°C in Mali on RNA quality were addressed by rapid sample processing, by storage of PBMC preparations at 0°C in RNAlater until the time of RNA extraction, and by the evaluation of RNA quality on-site in Bamako and again in New Orleans. Confounding by individual variation in gene expression was addressed by using the recovery samples from each subject as their control. This study design also permitted the study of changes in expression over time in pathways that were initially up- or downregulated. Confounding by antimalarial treatment was addressed by demonstrating that antimalarial treatment alone had no effect on gene expression.

4.2. Comparison with Previous Reports

These results provide the first information of which we are aware for upregulation of the apoptosis pathway with concomitant downregulation of apoptosis inhibitory genes during acute malaria (Figure 4). In contrast, the upregulation of inflammatory, host response, and proinflammatory cytokine genes observed (TNF, IFN-γ) is consistent with previous reports (Figure 3) [5, 7, 9, 10, 15, 23, 24] and there was no upregulation of immune response genes in the uninfected controls (data not shown). Although some immune-related genes were downregulated, those downregulated genes had immune-modulatory functions (Figure 2, profile BC).

4.3. Pathway Analyses

Revealed upregulation of cytokine, immune response, inflammatory response, complement activation (Figure 3), apoptosis (Figure 4), and Fas pathways [3032] in subjects with higher parasitemias (25,000–100,000 per μL and >100,000 per μL, Figures 3-4) and higher temperatures (≥39°C, data not shown).

4.4. The Role of the Innate Immune System in Uncomplicated P. falciparum Malaria [3335]

Is supported by the upregulation of Toll-like receptors (TLR 5) [36, 37], NK cell receptors (LILRs, KIRs), and chemokines during the acute illness (day 1). Indeed, several studies have suggested that the glycosylphosphatidylinositol (GPI) lipopolysaccharide which anchors P. falciparum proteins to parasite and red cell surfaces may stimulate the production of proinflammatory cytokines such as TNF, and Zhu et al. [15] have shown that GPI induction of IL-6, IL-12, and TNF is dependent on TLR activation via the p38- and NF-κB pathways. In these studies, IL-1β, IL-6, and TNF were upregulated more frequently in subjects with higher parasitemias (Figures 3-4) and higher temperatures (data not shown). In addition, studies in Uganda suggest that individuals heterozygous for the TLR 2 22 polymorphism may be protected from cerebral malaria [38].

4.5. Apoptosis in Malaria

The data reported here are likewise consistent with previous studies suggesting that apoptosis plays an important role in the pathogenesis of uncomplicated falciparum malaria [32, 3941]. Because they indicate that genes involved in apoptosis, such as Fas, BAX, and TP53, are upregulated during uncomplicated P. falciparum malaria in vivo (Figure 4), they suggest that apoptosis may be initiated through several different pathways in uncomplicated malaria, including TNF binding to TNFRSF, Fas (which can be induced by TNF), TNF binding to FasL, and possibly HMOX in response to oxidative stress. In these studies, upregulation of apoptosis-related genes correlated with higher parasitemias (>100,000 per μL, Figure 4) and higher body temperatures (≥39°C, data not shown). These results are also consistent with the findings of Wassmer et al. [42] who suggested that TGF-β1 from activated platelets may stimulate endothelial cell apoptosis and death in cerebral malaria. Despite the evidence from these and other studies for apoptosis in P. falciparum infection, the actual role(s) of apoptosis in malaria remains unclear although a number of studies have reported that this pathway is upregulated in severe malaria [6, 43, 44].

5. Conclusions

The data reported here indicate that the immune response, proinflammatory, and apoptosis pathways are upregulated at the time of acute illness in uncomplicated P. falciparum malaria. The apoptosis pathway remains upregulated for several days (days 1–3) before returning to normal. In contrast, immune-modulatory and apoptosis inhibitory genes are downregulated initially (days 1–3) and return to normal by the time of clinical recovery 7–10 days later.


BAX:BCL2 associated X-protein
CI:Confidence interval
GCOS:Gene chip operating system
GO:Gene Ontology
HG-U133 Plus 2.0:Gene chip for the study of human gene expression
ID:Identification (as in Gene ID Number)
msp1:Merozoite surface protein 1
PM:Perfect match
RIN:RNA integrity number
TNF:Tumor necrosis factor
TP53:Tumor protein 53 (p53).


This work was presented in part at the International Congress of Immunogenomics in Budapest, Hungary, in October 2006 (Abstract SY12-O-09), and at the 55th annual meeting of the American Society of Tropical Medicine in Atlanta, GA, in November 2006 (Abstract 304).

Conflict of Interests

The authors of this paper state that they have no commercial or other associations which might pose a conflict of interests.

Authors’ Contribution

James M. Colborn and Joni H. Ylöstalo contributed equally to this work.


The authors thank Fawaz Mzayek for his help in planning and performing the statistical analyses and Barbara Beckman, Frank B. Cogswell, Kaushal Deepak, Elizabeth Didier, Marcelo Kuroda, Michelle Lacey, Frances J. Mather, Tunika I. Okatcha, Sudesh Srivastav, and Young Hong for their thoughtful reviews of the paper. These studies were supported by the Emerging Infectious Diseases Program of the Centers for Disease Control and Prevention (Cooperative Agreements CCU/UR3 418652 and U01 CI 000211) and by a Tulane University Research Enhancement Award to DJK.


  1. P. C. C. Garnham, Malaria Parasites and Other Haemosporidia, Blackwell Scientific, Oxford, UK, 1966.
  2. Global Health Observatory, “Malaria,” 2015, View at: Google Scholar
  3. Centers for Disease Control and Prevention, “Malaria,” January 2015, View at: Google Scholar
  4. B. Greenwood, K. Marsh, and R. Snow, “Why do some African children develop severe malaria?” Parasitology Today, vol. 7, no. 10, pp. 277–281, 1991. View at: Publisher Site | Google Scholar
  5. L. H. Miller, D. I. Baruch, K. Marsh, and O. K. Doumbo, “The pathogenic basis of malaria,” Nature, vol. 415, no. 6872, pp. 673–679, 2002. View at: Publisher Site | Google Scholar
  6. N. H. Hunt, J. Golenser, T. Chan-Ling et al., “Immunopathogenesis of cerebral malaria,” International Journal for Parasitology, vol. 36, no. 5, pp. 569–582, 2006. View at: Publisher Site | Google Scholar
  7. L. Schofield and G. E. Grau, “Immunological processes in malaria pathogenesis,” Nature Reviews Immunology, vol. 5, no. 9, pp. 722–735, 2005. View at: Publisher Site | Google Scholar
  8. M. J. Griffiths, M. J. Shafi, S. J. Popper et al., “Genomewide analysis of the host response to malaria in Kenyan children,” Journal of Infectious Diseases, vol. 191, no. 10, pp. 1599–1611, 2005. View at: Publisher Site | Google Scholar
  9. B. G. Mordmüller, W. G. Metzger, P. Juillard et al., “Tumor necrosis factor in Plasmodium falciparum malaria: high plasma level is associated with fever, but high production capacity is associated with rapid fever clearance,” European Cytokine Network, vol. 8, no. 1, pp. 29–35, 1997. View at: Google Scholar
  10. P. H. Jakobsen, R. Moon, R. G. Ridley et al., “Tumour necrosis factor and interleukin-6 production induced by components associated with merozoite proteins of Plasmodium falciparum,” Parasite Immunology, vol. 15, no. 4, pp. 229–237, 1993. View at: Publisher Site | Google Scholar
  11. D. Kwiatkowski, J. G. Cannon, K. R. Manogue, A. Cerami, C. A. Dinarello, and B. M. Greenwood, “Tumour necrosis factor production in Falciparum malaria and its association with schizont rupture,” Clinical & Experimental Immunology, vol. 77, no. 3, pp. 361–366, 1989. View at: Google Scholar
  12. C. A. W. Bate, J. Taverne, E. Roman, C. Moreno, and J. H. L. Playfair, “Tumour necrosis factor induction by malaria exoantigens depends upon phospholipid,” Immunology, vol. 75, no. 1, pp. 129–135, 1992. View at: Google Scholar
  13. W. McGuire, A. V. S. Hill, C. E. M. Allsopp, B. M. Greenwood, and D. Kwiatkowski, “Variation in the TNF-alpha promoter region associated with susceptibility to cerebral malaria,” Nature, vol. 371, no. 6497, pp. 508–511, 1994. View at: Publisher Site | Google Scholar
  14. L. Schofield, M. C. Hewittt, K. Evans, M. A. Slomos, and P. H. Seeberger, “Synthetic GPI as a candidate anti-toxic vaccine in a model of malaria,” Nature, vol. 418, no. 6899, pp. 785–789, 2002. View at: Publisher Site | Google Scholar
  15. J. Zhu, G. Krishnegowda, and D. C. Gowda, “Induction of proinflammatory responses in macrophages by the glycosylphosphatidylinositols of Plasmodium falciparum: the requirement of extracellular signal-regulated kinase, p38, c-Jun N-terminal kinase and NF-kappaB pathways for the expression of proinflammatory cytokines and nitric oxide,” The Journal of Biological Chemistry, vol. 280, no. 9, pp. 8617–8627, 2005. View at: Publisher Site | Google Scholar
  16. X. Z. Su, V. M. Heatwole, S. P. Wertheimer et al., “The large diverse gene family var encodes proteins involved in cytoadherence and antigenic variation of Plasmodium falciparum-infected erythrocytes,” Cell, vol. 82, no. 1, pp. 89–100, 1995. View at: Publisher Site | Google Scholar
  17. H. M. Kyriacou, G. N. Stone, R. J. Challis et al., “Differential var gene transcription in Plasmodium falciparum isolates from patients with cerebral malaria compared to hyperparasitaemia,” Molecular and Biochemical Parasitology, vol. 150, no. 2, pp. 211–218, 2006. View at: Publisher Site | Google Scholar
  18. M. Schena, D. Shalon, R. W. Davis, and P. O. Brown, “Quantitative monitoring of gene expression patterns with a complementary DNA microarray,” Science, vol. 270, no. 5235, pp. 467–470, 1995. View at: Publisher Site | Google Scholar
  19. R. J. Lipshutz, S. P. A. Fodor, T. R. Gingeras, and D. J. Lockhart, “High density synthetic oligonucleotide arrays,” Nature Genetics, vol. 21, no. 1, pp. 20–24, 1999. View at: Publisher Site | Google Scholar
  20. D. J. Lockhart, H. Dong, M. C. Byrne et al., “Expression monitoring by hybridization to high-density oligonucleotide arrays,” Nature Biotechnology, vol. 14, no. 13, pp. 1675–1680, 1996. View at: Publisher Site | Google Scholar
  21. A. Schroeder, O. Mueller, S. Stocker et al., “The RIN: an RNA integrity number for assigning integrity values to RNA measurements,” BMC Molecular Biology, vol. 7, article 3, 2006. View at: Publisher Site | Google Scholar
  22. R. J. Lipshutz, S. P. A. Fodor, T. R. Gingeras, and D. J. Lockhart, “High density synthetic oligonucleotide arrays,” Nature Genetics, vol. 21, supplement 1, pp. 20–24, 1999. View at: Publisher Site | Google Scholar
  23. C. Li and W. H. Wong, “Model-based analysis of oligonucleotide arrays: expression index computation and outlier detection,” Proceedings of the National Academy of Sciences of the United States of America, vol. 98, no. 1, pp. 31–36, 2001. View at: Google Scholar
  24. S. Zhong, C. Li, and W. H. Wong, “ChipInfo: software for extracting gene annotation and gene ontology information for microarray analysis,” Nucleic Acids Research, vol. 31, no. 13, pp. 3483–3486, 2003. View at: Publisher Site | Google Scholar
  25. C. Li and W. H. Wong, “DNA-chip analyzer (dChip),” in The Analysis of Gene Expression Data: Methods and Software, G. Parmigiani, E. S. Garrett, R. A. Irizarry, and S. L. Zeger, Eds., pp. 1–446, Springer, New York, NY, USA, 2003. View at: Google Scholar
  26. T. R. Golub, D. K. Slonim, P. Tamayo et al., “Molecular classification of cancer: class discovery and class prediction by gene expression monitoring,” Science, vol. 286, no. 5439, pp. 531–527, 1999. View at: Publisher Site | Google Scholar
  27. M. B. Eisen, P. T. Spellman, P. O. Brown, and D. Botstein, “Cluster analysis and display of genome-wide expression patterns,” Proceedings of the National Academy of Sciences of the United States of America, vol. 95, no. 25, pp. 14863–14868, 1998. View at: Publisher Site | Google Scholar
  28. M. Ashburner, C. A. Ball, J. A. Blake et al., “Gene ontology: tool for the unification of biology,” Nature Genetics, vol. 25, no. 1, pp. 25–29, 2000. View at: Publisher Site | Google Scholar
  29. J. M. Colborn, O. A. Koita, O. Cissé, M. W. Bagayoko, E. J. Guthrie, and D. J. Krogstad, “Identifying and quantifying genotypes in polyclonal infections due to single species,” Emerging Infectious Diseases, vol. 12, no. 3, pp. 475–482, 2006. View at: Publisher Site | Google Scholar
  30. K. D. Dahlquist, N. Salomonis, K. Vranizan, S. C. Lawlor, and B. R. Conklin, “GenMAPP, a new tool for viewing and analyzing microarray data on biological pathways,” Nature Genetics, vol. 31, no. 1, pp. 19–20, 2002. View at: Publisher Site | Google Scholar
  31. S. W. Doniger, N. Salomonis, K. D. Dahlquist, K. Vranizan, S. C. Lawlor, and B. R. Conklin, “MAPPFinder: using gene ontology and GenMAPP to create a global gene-expression profile from microarray data,” Genome Biology, vol. 4, article R7, 2003. View at: Publisher Site | Google Scholar
  32. P. Kern, M. Dietrich, C. Hemmer, and N. Wellinghausen, “Increased levels of soluble Fas ligand in serum in Plasmodium falciparum malaria,” Infection and Immunity, vol. 68, no. 5, pp. 3061–3063, 2000. View at: Publisher Site | Google Scholar
  33. M. Baratin, S. Roetynck, C. Lépolard et al., “Natural killer cell and macrophage cooperation in MyD88-dependent innate responses to Plasmodium falciparum,” Proceedings of the National Academy of Sciences of the United States of America, vol. 102, no. 41, pp. 14747–14752, 2005. View at: Publisher Site | Google Scholar
  34. D. S. Hansen, K. J. Evans, M. C. D'Ombrain et al., “The natural killer complex regulates severe malarial pathogenesis and influences acquired immune responses to Plasmodium berghei ANKA,” Infection and Immunity, vol. 73, no. 4, pp. 2288–2297, 2005. View at: Publisher Site | Google Scholar
  35. B. Beutler, “Innate immunity: an overview,” Molecular Immunology, vol. 40, no. 12, pp. 845–859, 2004. View at: Publisher Site | Google Scholar
  36. H. Häcker, V. Redecke, B. Blagoev et al., “Specificity in Toll-like receptor signalling through distinct effector functions of TRAF3 and TRAF6,” Nature, vol. 439, no. 7073, pp. 204–207, 2006. View at: Publisher Site | Google Scholar
  37. B. Beutler, “Inferences, questions and possibilities in Toll-like receptor signalling,” Nature, vol. 430, no. 6996, pp. 257–263, 2004. View at: Publisher Site | Google Scholar
  38. J. A. Greene, N. Sam-Agudu, C. C. John, R. O. Opoka, P. A. Zimmerman, and J. W. Kazura, “Toll-like receptor polymorphisms and cerebral malaria: TLR2 Δ22 polymorphism is associated with protection from cerebral malaria in a case control study,” Malaria Journal, vol. 11, article 47, 2012. View at: Google Scholar
  39. A. T. Baldé, J. L. Sarthou, and C. Roussilhon, “Acute Plasmodium falciparum infection is associated with increased percentages of apoptotic cells,” Immunology Letters, vol. 46, no. 1-2, pp. 59–62, 1995. View at: Publisher Site | Google Scholar
  40. A. T. Balde, G. Aribot, A. Tall, A. Spiegel, and C. Roussilhon, “Apoptosis modulation in mononuclear cells recovered from individuals exposed to Plasmodium falciparum infection,” Parasite Immunology, vol. 22, no. 6, pp. 307–318, 2000. View at: Publisher Site | Google Scholar
  41. C. J. Hemmer, H. A. Lehr, K. Westphal, M. Unverricht, M. Kratzius, and E. C. Reisinger, “Plasmodium falciparum malaria: reduction of endothelial cell apoptosis in vitro,” Infection and Immunity, vol. 73, no. 3, pp. 1764–1770, 2005. View at: Publisher Site | Google Scholar
  42. S. C. Wassmer, J. B. de Souza, C. Frère, F. J. Candal, I. Juhan-Vague, and G. E. Grau, “TGF-beta1 released from activated platelets can induce TNF-stimulated human brain endothelium apoptosis: A new mechanism for microvascular lesion during cerebral malaria,” Journal of Immunology, vol. 176, no. 2, pp. 1180–1184, 2006. View at: Publisher Site | Google Scholar
  43. F. S. Touré, O. Ouwe-Missi-Oukem-Boyer, U. Bisvigou et al., “Apoptosis: a potential triggering mechanism of neurological manifestation in Plasmodium falciparum malaria,” Parasite Immunology, vol. 30, no. 1, pp. 47–51, 2008. View at: Publisher Site | Google Scholar
  44. C. Punsawad, Y. Maneerat, U. Chaisri, K. Nantavisai, and P. Viriyavejakul, “Nuclear factor kappa B modulates apoptosis in the brain endothelial cells and intravascular leukocytes of fatal cerebral malaria,” Malaria Journal, vol. 12, article 260, 2013. View at: Publisher Site | Google Scholar

Copyright © 2015 James M. Colborn et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

Related articles

No related content is available yet for this article.
 PDF Download Citation Citation
 Download other formatsMore
 Order printed copiesOrder

Related articles

No related content is available yet for this article.

Article of the Year Award: Outstanding research contributions of 2021, as selected by our Chief Editors. Read the winning articles.