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A novel in vitro model reveals distinctive modulatory roles of Plasmodium falciparum and Plasmodium vivax on naïve cell-mediated immunity
Malaria Journal volume 16, Article number: 131 (2017)
To date, human peripheral blood mononuclear cells (PBMCs) have been used mainly in immune stimulation assays and the interpretation of data can be influenced by the previous immunological history of donors and cross reactivity with other infectious agents. Resolving these limitations requires an alternative in vitro model to uncover the primary response profiles.
A novel in vitro model of mononuclear cells (MNCs) generated from haematopoietic stem cells (HSCs) was developed and these cells were then co-cultured with various antigens from Plasmodium falciparum and Plasmodium vivax to investigate the response of naïve immune cells to malaria antigens by flow cytometry.
In vitro stimulation of naïve lymphocytes showed that CD4+ and CD8+ T lymphocytes were significantly reduced (P < 0.01) by exposure to lysates of infected erythrocytes or intact erythrocytes infected with P. falciparum. The depletion was associated with the expression of CD95 (Fas receptor) on the surface of T lymphocytes. Maturation of T lymphocytes was affected differently, showing elevated CD3+CD4+CD8+ and CD3+CD4−CD8− T lymphocytes after stimulation with cell lysates of P. falciparum and P. vivax, respectively. In addition, antigen presenting monocytes and dendritic cells derived from haematopoietic stem cells showed impaired HLA-DR expression as a consequence of exposure to different species of malaria parasites.
These results suggest that naïve mononuclear cells differentiated in vitro from HSCs could provide a valid model for the assessment of immunity. P. falciparum and P. vivax malaria parasites could modulate various populations of immune cells starting from newly differentiated mononuclear cells.
To date, research on adaptive immunity has been restricted to the use of peripheral blood mononuclear cells (PBMCs) as an in vitro model. However, some of these PBMCs are either already committed, or have been primed with unknown epitopes from previously encountered microbes. Given this phenomenon, there might be a number of factors leading to misinterpretation of results, particularly when cross reactivity is concerned [1, 2]. Lymphocytes circulating in the peripheral blood could have already committed to a vast number of non-self-antigens derived mostly from microbial products before being recruited into the experiment. A study in 2004 by Bisset and colleagues  supported this theory, and showed that less than half CD4+ cells, and less than a quarter CD8+ T lymphocytes in the peripheral blood remained naïve. Consequently, several diseases have shown cross reactivity with malaria, i.e. schistosomiasis [4, 5], leishmaniasis, toxoplasmosis, and Chagas’ disease .
Resolving these limitations requires an alternative in vitro model such as newly produced immune cells to uncover primary response profiles. However, there is little information on the in vitro application of mononuclear cells (MNCs) derived from haematopoietic stem cells (HSCs) for research in this area. This study establishes a novel in vitro model focusing on the use of naïve T lymphocytes in stimulation assays. Additionally, the system uses newly differentiated immune cells derived from cord blood-HSCs to verify the modulatory roles of Plasmodium falciparum and Plasmodium vivax in the manipulation of naïve immune cells without the interference of prior donor immunological exposure.
Isolation of cord blood mononuclear cells
Ten samples of umbilical cord blood of normal full-term newborns obtained from Ramathibodi Hospital following informed consent (MURA2014/400 approved by Ethical Committee of Research on Human Beings from Ramathibodi Hospital, Faculty of Medicine, Mahidol University, Bangkok, Thailand) were used to isolate HSCs. Between 50 and 70 ml of cord blood was collected into blood bags containing 30 ml of CPDA-1 anticoagulant [Kawasumi Laboratories (Thailand) Co Ltd]. Cord blood samples were overlaid on Lymphoprep™ solution (Axis Shield PoC, Oslo, Norway) at a 1:1 ratio by volume and centrifuged (Kubota, Tokyo, Japan) at 1200×g, 20 °C for 30 min. The interface layer containing the cord blood mononuclear cells (CBMNs) was collected and washed twice with cold PBS buffer containing 2 mM EDTA. Viability of isolated cells was assessed using the trypan blue exclusion method.
Isolation of CD34+ haematopoietic stem cells (HSCs)
HSCs were isolated from CBMNs with a CD34 isolation kit and Mini-MACS columns (Miltenyi Biotech, Germany) according to the manufacturer’s protocol. Briefly, 1 × 108 CBMCs were suspended in 500 µl cold PBS containing 2 mM EDTA and 0.5% fetal calf serum. The cell suspensions were incubated at 4 °C, for 30 min with 100 µl of each FcR blocking reagent and anti-CD34 antibody-conjugated magnetic microbeads (clone: QBEND/10). Subsequently, the cells were washed with cold PBS buffer to remove unbound anti-CD34 antibodies and loaded onto an LS column (Miltenyi Biotech, Germany). The column was rinsed with PBS buffer to remove non-specific cells. The retained CD34+ cells were eluted from the column with PBS buffer and centrifuged at 800×g for 10 min at 4 °C and the resulting cell pellet was re-suspended in StemlineII™ medium, cells were counted and cultured.
Cultivation and differentiation of HSCs derived from CBMNs (HSC-derived MNCs)
The isolated CD34+ haematopoietic stem cells were cultured according to an established protocol . Briefly, 5 × 105 cell/ml of CD34+ cells were cultured in 12-well tissue culture plates (Costar®, Corning Inc, NY, USA) using StemlineII™ medium (Sigma-Aldrich Corp, MI, USA) supplemented with 50 ng/ml of stem cell factor (Sigma-Aldrich Corp), 10 ng/ml of IL-3 (PeproTech Asia, Rehovot, Israel), 100 µg/ml transferrin (Sigma-Aldrich Corp) and 100 µg/ml of humulin (Sigma-Aldrich Corp). CD34+ HSCs were incubated at 37 °C in a humidified atmosphere with 5% CO2 and half volumes of medium were replaced with fresh complete medium every three days. Cell number and viability were assessed after five and ten days of cultivation by the trypan blue exclusion method. On day 10 of cultivation, cell surface markers of all mononuclear cells were determined by flow cytometric analysis (FACScan, Becton–Dickinson, Oxford, UK) and cells were morphologically examined after Giemsa staining. Ten days old HSC-derived MNCs were used in co-cultivation with malaria antigens in all assays.
Cultivation of parasites and antigen preparations
Antigens used in this study were prepared from two sources of human malaria parasites. Plasmodium falciparum parasites were obtained from in vitro cultivation of TM267 laboratory strain maintained in group O human erythrocytes from healthy donors by in vitro cultivation, using RPMI-1640 medium (Gibco, Carlsbad, CA. USA) supplemented with 10% human serum. The parasites were incubated at 37 °C in a humidified atmosphere with 5% CO2 in air, starting from ring stages until most of the P. falciparum parasites entered mature schizont stages.
Plasmodium vivax parasites were isolated from blood of 10 P. vivax-infected patients (Ethical Approvals WRAIR#1308, MU-IRB 2009/346.2711). Briefly, blood samples were filtered through Plasmodipur® filters (Euro-Diagnostic B.V., The Netherlands) to deplete leukocytes. The resulting P. vivax-infected blood were washed twice with McCoy 5A medium (Gibco) by centrifugation at 800×g, 4 °C for 5 min and cultured at 5% haematocrit in McCoy’s 5A medium supplemented with 25% human AB-serum. The parasites were kept at 37 °C in a humidified atmosphere with 5% CO2 in air for 24–30 h (depending on the age of the starting parasites) until most of the P. vivax parasites entered mature schizont stages.
Two types of antigen preparations, intact infected erythrocytes and parasitized cell lysates, were prepared from both species. Schizont stage parasites were isolated by gradient centrifugation at 1200×g, 4 °C for 30 min with 60% Percoll® for P. falciparum infected erythrocytes, and 45% Percoll® for P. vivax infected erythrocytes to enrich the parasite. Plasmodium falciparum-infected erythrocytes (PfIEs) and P. vivax-infected erythrocytes (PvIEs) in the interface layer between medium and Percoll® were collected and washed twice by centrifugation at 800×g, 4 °C for 5 min with cold RPMI-1640. The resulting PfIEs and PvIEs were counted and used to stimulate the HSC-derived MNCs as described below. For the parasite lysates, the same batch pellets of the PfIEs and PvIEs were stored at −70 °C without any cryopreservative agent and twice freeze–thawed for use as whole malaria infected erythrocyte lysates. Uninfected erythrocyte controls were prepared from erythrocytes of healthy donor used in the P. falciparum parasite culture by repeating the same protocol as that used for infected erythrocytes as described above.
Stimulation of HSC-derived MNCs with malaria antigens
On day 10 of cultivation, HSC-derived MNCs from each cord blood sample were individually co-cultured with the different malaria antigens, i.e. intact infected erythrocytes and whole parasite infected erythrocyte lysates from both P. falciparum and P. vivax (MNCs: antigens = 1:5). Stimulation with intact uninfected erythrocyte (1:5) and whole uninfected erythrocyte lysate (1:5) were used as baseline controls for the leukocyte response. Phytohemagglutinin-A (PHA) (5 µg/ml) was used for validating the activity of T lymphocytes for mitogenic response. On day 2 or day 4 after stimulation, the HSC-derived MNCs were harvested for phenotypic characterization by flow cytometry (FACScan).
Phenotypic characterization and expression of death receptor (CD95)
Phenotyping of the cells was performed by three-colour flow cytometry (FACScan). Stimulated HSC-derived MNCs (1 × 105 cell) from each condition were labeled with fluorescent, dye-conjugated monoclonal antibodies to define various populations of cells including T lymphocytes (anti-CD3-PECy5, CD4-PE and CD8-FITC), monocytes (anti-CD14-PE and HLA-DR-PECy5), dendritic cells (anti-CD40-FITC, and HLA-DR-PECy5), B lymphocytes (anti-CD19-FITC), NK and NKT cells (anti-CD3-PE and CD56-FITC), HSCs (anti-CD34-PE and Lin-FITC) and expression of death receptor (anti-CD3-PE, anti-CD4-FITC, anti-CD8-FITC and anti-CD95- PECy5) (eBioscience, San Diego, CA, USA; and Miltenyi Biotech, Germany for anti-CD34-PE) (details of antibodies used can be found in Additional file 1). After staining, the cells were washed with PBS pH 7.4 and fixed with 1% paraformaldehyde in PBS. The analysis was performed using the CellQuest software (Becton–Dickinson, San Jose, CA, USA). The mononuclear cells were gated by that excludes those events with low FSC and high SSC, for exclusion of debris and dead cells from the analysis.
The data are represented as fold change of population and analysed by the GraphPad Prism (version 6.0, San Diego, CA, USA) and SPSS (version 18.0, Chicago, IL, USA) programs. Statistical significance was determined by one-way analysis of variance (ANOVA). The Mann–Whitney U test for nonparametric data was used for statistical analysis between the fold changes of population of each condition. The results were considered significant at P < 0.05.
Analysis of leukocyte populations obtained from HSC culture
HSC cultures were started with highly purified CD34+ Lin− cells (95–98%) and maintained for 10 days. The expansion of total nucleated cells ranged from 5.1 to 8.5-fold on day 5 and 16.6 to 25.15-fold on day 10 after cultivation (Fig. 1a). The viability of the immune cells was more than 90% over the cultivation period (Fig. 1b).
Populations of leukocytes in the HSC cultures were characterized by flow cytometry on day 10 post in vitro cultivation. Several types of immune cell (Fig. 1c) were observed, CD3+ T lymphocytes (20.96% ±1.33), B lymphocytes (7.47% ±0.80), monocytes (10.64% ±0.72), dendritic cells (5.28% ±0.72), natural killer cells (1.88% ±0.31), natural killer T cells (6.18% ±1.17) and granulocytes (25.65% ±1.94) (examined by Giemsa staining). The rest were CD34+ HSC (21.94% ±2.57) remaining in the culture. Taken together (Fig. 1d), mononuclear cells (52.4% ±2.26) were the majority of immune cells in this HSC culture giving twofold higher numbers than that of the polymorphonuclear cells (25.6% ±1.94).
Alterations of lymphocyte population by an in vitro exposure to malaria parasites
An inhibitory effect of Plasmodium to the newly produced T lymphocytes was observed in the in vitro culture system (Fig. 2). Both intact PfIEs and PfIEs lysates significantly reduced (P ≤ 0.001) CD4+ T lymphocytes by 0.35 ± 0.12 and 0.45 ± 0.11-fold, respectively (Fig. 2a). Only intact PfIEs could deplete half of CD8+ T lymphocytes (P ≤ 0.05) (Fig. 2B). Neither antigen from P. vivax showed any significant effect on either CD4+ or CD8+ T lymphocytes compared to their corresponding uninfected erythrocytes control (UIEs). The mitogenic effect of PHA was also observed, showing a 1.4 ± 0.18-fold increases of CD4+ T lymphocytes, whereas CD8+ T lymphocytes were not affected in the HSC culture (Fig. 2b).
The influence of Plasmodium to the transitional stages of T lymphocytes (CD3+4−8− cells and CD3+4+8+ cells) was monitored in this HSCs culture system. Double positive T lymphocytes (CD3+4+8+ cells) increased 2.5 ± 0.79-fold in the presence of PfIEs lysates (Fig. 2c) whereas double negative T lymphocytes (CD3+4−8− cells) were elevated 1.6 ± 0.13-fold when exposed to PvIEs lysates compared to UIEs (Fig. 2D) (scatter plots and absolute number of T lymphocyte, can be viewed in Additional files 2 and 3).
Plasmodium falciparum induced expression of CD95 on the surface membrane of T lymphocytes
Depletion of T lymphocytes by the malaria parasite was associated with apoptosis through the CD95 pathway. Abundant CD8 T lymphocytes expressing CD95 on their surface were found on day 2 after being exposed to both intact PfIEs (3.69 ± 0.21-fold) and PfIEs lysates (2.15 ± 0.16-fold). CD4 T lymphocytes expressing CD95 were increased slightly in co-cultivation with intact PfIEs (1.52 ± 0.21-fold) compared to all other antigens in this study (Additional file 3). Plasmodium vivax did not significantly induce the expression of CD95 on T lymphocytes compared to UIEs (Fig. 3) (scatter plots can be viewed in Additional file 4).
The diverse effects of Plasmodium falciparum and Plasmodium vivax on antigen presenting cells
The effects of malaria parasites on monocytes and dendritic cells were assessed (Fig. 4). PfIEs lysates significantly (P ≤ 0.05) increased the number of HSC-derived monocytes by 2.14 ± 0.78-fold when compared to UIEs lysates. Intact PfIEs did not affect the monocyte population but reduced by more than half HSC-derived dendritic cells (0.45 ± 0.09) compared to the intact UIEs (P ≤0.05). Neither intact IEs nor the IEs lysates of P. vivax showed any effect on monocytes or dendritic cells (scatter plots, can be viewed in Additional file 5).
Malaria parasites altered the expression of human leucocyte antigen (HLA)-DR on the surface of monocytes and dendritic cells
To observe any modulation of antigen presenting cells by the malaria parasites, the level of HLA-DR expression by monocytes and dendritic cells was measured. Flow cytometric analysis showed that intact PfIEs increased HLA-DR expression by twofold as shown by increased mean fluorescence intensity (MFI) on the surface of monocytes (CD14+ cells). In contrast, intact PvIEs compared with intact UIEs did not show any difference on the overall level of HLA-DR as indicated by the MFI values (12.6 and 14.8, respectively); nonetheless the patterns of HLA-DR expression on CD14+ cells under the influence of P. vivax antigens were noticeably different compared to that of CD40+ cells (Fig. 5). The IEs lysates from both P. falciparum (MFI = 38.2) and P. vivax (MFI = 32.1) parasites also showed twofold higher HLA-DR expression than that of UIEs lysates (MFI = 16.2).
In dendritic cells, the intact PfIEs (MFI = 12.8) reduced HLA-DR expression by half while intact PvIEs (MFI = 24.4) did not reduce in comparison with intact UIEs (MFI = 22.4). However, PfIEs lysates (MFI = 46.2) and PvIEs lysates (MFI = 30.3) increased the levels of HLA-DR by twofold and 1.5-fold, respectively, on these cells compared to that of UIEs lysates (Fig. 5).
Plasmodium falciparum sustained existence of CD34+ HSCs in the culture
The effect of malaria parasites on the development of HSCs is not well understood. Results obtained from the in vitro model presented in this study showed that intact PfIEs significantly increased the CD34+ HSCs remaining in the culture, resulting in a 1.5 ± 0.24-fold higher abundance of these cells when compared to the control (Fig. 6). All other antigens tested did not alter the number of CD34+ HSCs in the cultures (scatter plots, can be viewed in Additional file 6).
The development of an in vitro model for HSC-derived MNCs with minimal cytokine supplementation (SCF, IL-3, transferrins and human insulin)  generating naïve mononuclear cells is crucial to the study of the response of newly produced immune cells to any agent. Such a system eliminates problems frequently encountered when using PBMCs from donors with various immunological profiles. In the HSC-derived MNC culture, phenotypic markers of mature leukocyte populations were variously expressed on consecutive days as reported previously . On day 10 of cultivation, the expression of all mature leukocytes markers was observed with sufficient cell numbers to perform the experiment. The high percentage of monocytes and dendritic cells obtained under these culture conditions was an additional factor favouring the use of HSC-derived MNCs to study the responses of naïve immune cells to an infection. The activation of newly produced T lymphocytes by malaria antigens was verified by showing up-regulation of an activation marker, CD25 (IL2 receptor) (more view in Additional file 7). This study shows an alternative model to follow the responses of naïve lymphocytes to P. falciparum and P. vivax malaria.
Immunity to malaria relies on T lymphocytes as the agents for combating malaria parasites in both the pre-erythrocytic and erythrocytic stages [9–11]. However, understanding the mechanism or function of these cells is not yet complete. In the study presented here, P. falciparum depleted T lymphocytes in accordance with previous studies [12, 13], although some previous studies have also shown lymphopaenia in P. vivax patients . Different mechanisms for the suppression of T lymphocytes by malaria parasites have been proposed, and two possible hypotheses could explain lymphopaenia during acute malaria infection. Firstly the distribution of activated T lymphocyte to other organs such as spleen has been reported in mice  although this phenomenon could not be observed in this in vitro system. Secondly, the depletion of T lymphocyte observed in this experiment could occur as a result of the induction of T lymphocyte apoptosis upon malaria parasite infection.
Apoptosis is suggested to be associated with lymphopaenia through various mechanisms during acute infection [16, 17]. The data showed that P. falciparum but not P. vivax caused the loss of CD4 and CD8 positive T cells and these were associated with the CD95 (Fas)-ligand binding pathway. Our unpublished data indicated that CD95 appeared on lymphocytes after the cells were exposed to P. falciparum antigens from day 2 onward and these cells were undetectable on day 4. Therefore CD95 was determined on day 2 whereas other population markers were done on day 4. Plasmodium falciparum affected the expression of CD95 of the CD8+ subpopulation more than that of CD4+ lymphocytes. However, a study in murine malaria showed that depletion of parasite-specific T cells was not via the Fas pathway . Therefore, the present findings confirmed previous report on the difference in immune modulatory roles between human and murine malaria.
In this study, parasite antigens were obtained from different sources, namely P. falciparum obtained from in vitro culture and P. vivax isolated from endemically infected people with a short period of culture to reach schizont stage. The endogenous RBC membrane components should be the same, and the obvious difference is the membrane associated parasite proteins. Therefore, the difference in the source of parasites should not affect the study outcome, but the difference in species of parasites would play major role in the activation of the naïve immune cells. The results showed the response of HSCs derived T lymphocytes exposed to P. falciparum have a higher degree of immune suppression as compared to P. vivax in term of amount and polymorphism of proteins [19–21]. The antigenicity of malaria proteins depends on the nature of the proteins and the process of presentation by antigen presenting cells. In this study, particulate infected erythrocytes (intact IEs) of both parasites could alter the population of HLA−DR+ cells to a greater extent than the parasite lysates. Differential responses of T lymphocytes to different forms of antigen have been documented previously [22, 23].
Malaria infection can suppress erythropoiesis [24, 25], but little is known about the influence on immune cells in the biological niches where development and differentiation take place, i.e. the bone marrow, spleen and lymph nodes. However, a modulatory effect of malaria on the alteration of immune cell populations was demonstrated in this in vitro model. The double-positive developmental stage of T lymphocytes (CD3+CD4+CD8+) was elevated upon exposure to cell lysates of P. falciparum. This phenomenon could be associated with the severity of malaria as has been reported for several other infectious diseases, such as HIV  and Chagas disease , including autoimmune diseases  suggesting an immune suppressive role of this cell type . On the other hand, the increment of double-negative developmental stage of T lymphocytes (CD3+CD4−CD8−) when activated with cell lysates of the P. vivax malaria parasite, emphasized the difference in the response of newly produced immune cells to the two parasites. Therefore, the consequence of elevated numbers of double-positive and double-negative T lymphocytes upon exposure to proteins extracted from P. falciparum and P. vivax, respectively, observed here is interesting and deserves further investigation for their roles in immunity to malaria. This study showed for the first time that P. falciparum and P. vivax differently modulate lymphopoiesis during the immune response to malaria.
Immunity to malaria requires functional co-operation between antigen-presenting cells (macrophages and dendritic cells) and lymphocytes [30, 31], but these antigen-presenting cells can occasionally play a role in severe malaria . In this study, cell lysates from P. falciparum raised the proportion of monocytes in the HSC culture which might be associated with the immunopathology of severe malaria. Signs of defective immune priming were also seen in this study, as shown by a decrease in the population of professional antigen presenting cells, dendritic cells, after exposure to P. falciparum while the number of these antigen presenting cells was similar to control cultures after exposure to P. vivax. In addition, the opposite effects of P. falciparum and P. vivax on the expression of HLA-DR in monocytes and dendritic cells described here supports previous findings reported by others . Interestingly, the two types of antigen from P. falciparum increased expression of HLA-DR on the surface of monocytes which could be an incidence of severe outcome from immune over activation as reported in autoimmune disease patients . In contrast, antigens from P. vivax regulated the distinctive pattern of HLA-DR expression on these monocytes which could confer milder symptoms as compared to those caused by P. falciparum.
The effect of human malaria on the development of HSCs is not known and whether the prolonged CD34+ HSC propagation in vitro was due mainly to activation by P. falciparum-infected erythrocytes requires further investigation.
These finding suggest that immunosuppression by malaria infection possibly takes place at an early stage of lymphocyte maturation. In addition, the use of naïve mononuclear cells derived from HSC as an in vitro model for research in immunity can be easily implemented and would reduce the discrepancy of mononuclear cell quality between different studies.
Valdes R Jr, Jortani SA. Unexpected suppression of immunoassay results by cross-reactivity: now a demonstrated cause for concern. Clin Chem. 2002;48:405–6.
Tate J, Ward G. Interferences in immunoassay. Clin Biochem Rev. 2004;25:105–20.
Bisset LR, Lung TL, Kaelin M, Ludwig E, Dubs RW. Reference values for peripheral blood lymphocyte phenotypes applicable to the healthy adult population in Switzerland. Eur J Haematol. 2004;72:203–12.
Pierrot C, Wilson S, Lallet H, Lafitte S, Jones FM, Daher W, et al. Identification of a novel antigen of Schistosoma mansoni shared with Plasmodium falciparum and evaluation of different cross-reactive antibody subclasses induced by human schistosomiasis and malaria. Infect Immun. 2006;74:3347–54.
Waknine-Grinberg JH, Gold D, Ohayon A, Flescher E, Heyfets A, Doenhoff MJ, et al. Schistosoma mansoni infection reduces the incidence of murine cerebral malaria. Malar J. 2010;9:5.
Abramo C, Fontes CJ, Krettli AU. Cross-reactivity between antibodies in the sera of individuals with leishmaniasis, toxoplasmosis, and Chagas’ disease and antigens of the blood-stage forms of Plasmodium falciparum determined by indirect immunofluorescence. Am J Trop Med Hyg. 1995;53:202–5.
Payuhakrit W, Panichakul T, Charoenphon N, Chalermsaenyakorn P, Jaovisidha A, Wongborisuth C, et al. In vitro production of functional immune cells derived from human haematopoietic stem cells. EXCLI J. 2015;14:1031–9.
Duarte RF, Frank DA. SCF and G-CSF lead to the synergistic induction of proliferation and gene expression through complementary signaling pathways. Blood. 2000;96:3422–30.
Perez-Mazliah D, Langhorne J. CD4 T-cell subsets in malaria: TH1/TH2 revisited. Front Immunol. 2014;5:671.
Morrot A, Zavala F. Effector and memory CD8+ T cells as seen in immunity to malaria. Immunol Rev. 2004;201:291–303.
Cockburn IA, Amino R, Kelemen RK, Kuo SC, Tse SW, Radtke A, et al. In vivo imaging of CD8+ T cell-mediated elimination of malaria liver stages. Proc Natl Acad Sci USA. 2013;110:9090–5.
Perrin LH, Mackey LJ, Miescher PA. The hematology of malaria in man. Semin Hematol. 1982;19:70–82.
Richards MW, Behrens RH, Doherty JF. Hematologic changes in acute, imported Plasmodium falciparum malaria. Am J Trop Med Hyg. 1998;59:859.
Kassa D, Petros B, Mesele T, Hailu E, Wolday D. Characterization of peripheral blood lymphocyte subsets in patients with acute Plasmodium falciparum and P. vivax malaria infections at Wonji Sugar Estate, Ethiopia. Clin Vaccine Immunol. 2006;13:376–9.
Langhorne J, Simon-Haarhaus B. Differential T cell responses to Plasmodium chabaudi chabaudi in peripheral blood and spleens of C57BL/6 mice during infection. J Immunol. 1991;146:2771–5.
Riccio EK, Junior IN, Riccio LR, das Alecrim M, Corte-Real S, Morgado M, et al. Malaria associated apoptosis is not significantly correlated with either parasitemia or the number of previous malaria attacks. Parasitol Res. 2003;90:9–18.
Kern P, Dietrich M, Hemmer C, Wellinghausen N. Increased levels of soluble Fas ligand in serum in Plasmodium falciparum malaria. Infect Immun. 2000;68:3061–3.
Xu H, Wipasa J, Yan H, Zeng M, Makobongo MO, Finkelman FD, et al. The mechanism and significance of deletion of parasite-specific CD4+ T cells in malaria infection. J Exp Med. 2002;195:881–92.
Rayner JC, Tran TM, Corredor V, Huber CS, Barnwell JW, Galinski MR. Dramatic difference in diversity between Plasmodium falciparum and Plasmodium vivax reticulocyte binding-like genes. Am J Trop Med Hyg. 2005;72:666–74.
Neafsey DE, Galinsky K, Jiang RH, Young L, Sykes SM, Saif S, et al. The malaria parasite Plasmodium vivax exhibits greater genetic diversity than Plasmodium falciparum. Nat Genet. 2012;44:1046–50.
Jennison C, Arnott A, Tessier N, Tavul L, Koepfli C, Felger I, et al. Plasmodium vivax populations are more genetically diverse and less structured than sympatric Plasmodium falciparum populations. PLoS Negl Trop Dis. 2015;9:e0003634.
Scholzen A, Mittag D, Rogerson SJ, Cooke BM, Plebanski M. Plasmodium falciparum-mediated induction of human CD25Foxp3 CD4 T cells is independent of direct TCR stimulation and requires IL-2, IL-10 and TGFbeta. PLoS Pathog. 2009;5:e1000543.
Finney OC, Lawrence E, Gray AP, Njie M, Riley EM, Walther M. Freeze-thaw lysates of Plasmodium falciparum-infected red blood cells induce differentiation of functionally competent regulatory T cells from memory T cells. Eur J Immunol. 2012;42:1767–77.
Awandare GA, Kempaiah P, Ochiel DO, Piazza P, Keller CC, Perkins DJ. Mechanisms of erythropoiesis inhibition by malarial pigment and malaria-induced proinflammatory mediators in an in vitro model. Am J Hematol. 2011;86:155–62.
Panichakul T, Payuhakrit W, Panburana P, Wongborisuth C, Hongeng S, Udomsangpetch R. Suppression of erythroid development in vitro by Plasmodium vivax. Malar J. 2012;11:173.
Chauhan NK, Vajpayee M, Mojumdar K, Singh R, Singh A. Study of CD4+ CD8+ double positive T-lymphocyte phenotype and function in Indian patients infected with HIV-1. J Med Virol. 2012;84:845–56.
Giraldo NA, Bolanos NI, Cuellar A, Guzman F, Uribe AM, Bedoya A, et al. Increased CD4+/CD8+ double-positive T cells in chronic Chagasic patients. PLoS Negl Trop Dis. 2011;5:e1294.
Iwatani Y, Hidaka Y, Matsuzuka F, Kuma K, Amino N. Intrathyroidal lymphocyte subsets, including unusual CD4+ CD8+ cells and CD3loTCR alpha beta lo/-CD4− CD8− cells, in autoimmune thyroid disease. Clin Exp Immunol. 1993;93:430–6.
Overgaard NH, Jung JW, Steptoe RJ, Wells JW. CD4+/CD8+ double-positive T cells: more than just a developmental stage? J Leukoc Biol. 2015;97:31–8.
Urban BC, Ing R, Stevenson MM. Early interactions between blood-stage plasmodium parasites and the immune system. Curr Top Microbiol Immunol. 2005;297:25–70.
Wykes MN, Good MF. What really happens to dendritic cells during malaria? Nat Rev Microbiol. 2008;6:864–70.
Chua CL, Brown G, Hamilton JA, Rogerson S, Boeuf P. Monocytes and macrophages in malaria: protection or pathology? Trends Parasitol. 2013;29:26–34.
Noone C, Parkinson M, Dowling DJ, Aldridge A, Kirwan P, Molloy SF, et al. Plasma cytokines, chemokines and cellular immune responses in pre-school Nigerian children infected with Plasmodium falciparum. Malar J. 2013;12:5.
Thomas R. Antigen-presenting cells in rheumatoid arthritis. Springer Semin Immunopathol. 1998;20:53–72.
SC and RU designed the study. SC performed experiment and statistical analysis, and wrote the manuscript. PP collected human cord blood from normal full-term deliveries. SC and ME isolated human CD34+ cells and cultured cells. JS provided malaria parasites. SS in vitro cultured of malaria parasite. MM and RB provided materials for malaria culture. SJ and RU contributed substantially to the design of the study and critically revised the manuscript. All authors read and approved the final manuscript.
We wish to thank staff at the Department of Obstetrics and Gynecology, Faculty of Medicine, Ramathibodi Hospital, Mahidol University for handling of cord blood samples. We sincerely thank to Prof. Dr. Kovit Pattanapanyasat, Department of Health Research and Development, Faculty of Medicine Siriraj Hospital and Dr. Pornthip Chaichompoo for flow cytometry analysis. We appreciate the useful discussions of Dr. Markus Winterberg and Dr. Warunee Hanpithakpong, The Wellcome-Mahidol-Oxford Research Unit, Faculty of Tropical Medicine, Mahidol University, and the valuable comments of Dr. Arther E. Brown. We thank Prof. Duncan R. Smith for English language proofing and editing.
The authors declare that they have no competing interests.
This project is supported by The Office of the Higher Education Commission, National Research Universities Initiative, Mahidol University; Institutional Research Grant from the Thailand Research Fund (IRG5780011) and Graduate Student Scholarship to Mr. Setthakit Chitsanoor from National Research Council of Thailand (Fiscal year 2557).
Fluorescent dye-conjugated monoclonal antibodies used for characterizing of cell phenotypes.
Responses of naïve T lymphocytes to malaria parasites.
Responses of naïve T lymphocytes to malaria parasites (absolute number).
Malaria parasites induced the expression of CD95 on T lymphocytes.
Effects of malaria parasites on the antigen presenting cells.
Effects of malaria on the remaining of CD34+ cells.
Activation of naïve T lymphocytes by the lysate of P. falciparum infected erythrocytes.
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Chitsanoor, S., Somsri, S., Panburana, P. et al. A novel in vitro model reveals distinctive modulatory roles of Plasmodium falciparum and Plasmodium vivax on naïve cell-mediated immunity. Malar J 16, 131 (2017). https://doi.org/10.1186/s12936-017-1781-4
- Hematopoietic stem cells
- Cell mediated immunity