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A forward genetic screen identifies erythrocyte CD55 as essential for Plasmodium falciparum invasion

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Science  08 May 2015:
Vol. 348, Issue 6235, pp. 711-714
DOI: 10.1126/science.aaa3526

A way to dissect malaria's secrets

Malaria has exerted a strong selective force on the human genome. However, efforts to identify host susceptibility factors have been hindered by the absence of a nucleus in red blood cells. Egan et al. developed an approach involving blood stem cells to discover host factors critical for Plasmodium falciparum infection of red blood cells. The authors identified an essential host receptor for parasite invasion that could provide a target for malaria therapeutics.

Science, this issue p. 711

Abstract

Efforts to identify host determinants for malaria have been hindered by the absence of a nucleus in erythrocytes, which precludes genetic manipulation in the cell in which the parasite replicates. We used cultured red blood cells derived from hematopoietic stem cells to carry out a forward genetic screen for Plasmodium falciparum host determinants. We found that CD55 is an essential host factor for P. falciparum invasion. CD55-null erythrocytes were refractory to invasion by all isolates of P. falciparum because parasites failed to attach properly to the erythrocyte surface. Thus, CD55 is an attractive target for the development of malaria therapeutics. Hematopoietic stem cell–based forward genetic screens may be valuable for the identification of additional host determinants of malaria pathogenesis.

Severe malaria is caused by Plasmodium falciparum and is one of the leading causes of mortality among children globally (1). During infection, parasites invade and replicate within human erythrocytes (2). Host erythrocyte polymorphisms that confer resistance to severe malaria have been identified with epidemiologic approaches (3, 4). Genome-wide association studies have searched for host determinants of malaria, but functional validation in the erythrocyte remains challenging owing to the absence of a nucleus (57). Recent advances in the ex vivo production of erythrocytes now enable generation of genetically altered cells that support P. falciparum infection (811). Here, we used ex vivo–cultured red blood cells (cRBCs) in a forward genetic screen in order to identify host determinants of malaria infection.

The human erythrocyte is a terminally differentiated minimal cell that lacks organelles and a nucleus and has a small proteome (12). To identify erythrocyte proteins that influence P. falciparum infection, we designed a screening strategy involving RNA interference (RNAi)–based knockdown of gene expression in hematopoietic progenitor cells, induction of ex vivo erythropoiesis, and last, infection of terminally differentiated erythroblasts with P. falciparum. Because gene knockdowns that affect erythroid development could have potent yet nonspecific effects on parasites in this approach, we first screened the erythrocyte proteome so as to identify genes that influence terminal differentiation of erythrocytes (Fig. 1A, fig. S1A, and data set S1). CD34+ hematopoietic stem cells (HSCs) were transduced with our pooled erythrocyte proteome short hairpin RNA (shRNA) library and induced to proliferate and differentiate to the orthochromatic erythroblast stage (when parasite infection can occur) (13). After 19 days, we quantified each shRNA in the surviving orthochromatic erythroblasts relative to the original library, with the prediction that shRNAs underrepresented in the differentiated erythroblasts would target genes important for erythropoiesis.

Fig. 1 Pooled shRNA screen for genes that regulate terminal erythroid differentiation.

(A) Schematic of pooled shRNA screen. CD34+ HSCs were induced toward erythroid development, transduced with shRNA library on Day 6, and selected with puromycin. On day 19, shRNA proviruses in orthochromatic erythroblasts were quantified by means of Illumina (San Diego, CA) sequencing. (B) Change in relative abundance of 5530 shRNAs in erythrocyte proteome library after 19 days of differentiation. (C) RNAi gene enrichment ranking (RIGER) analysis of 116 candidate genes based on magnitude of erythropoiesis phenotype. NES, normalized enrichment score. (D) Predicted localization of library components, with percent of genes that influence erythropoiesis in red.

The erythropoiesis screen yielded sufficient cells for full coverage of the library (>1500 cells per shRNA) (fig. S1B) (14), and deep sequencing of shRNA proviruses isolated from the terminally differentiated erythroid cells revealed a normal distribution (fig. S1C). Of shRNAs, 4.4% were depleted more than 50% in day-19 cRBCs relative to the original library pool, whereas 2% were enriched (Fig. 1B), indicating that these shRNAs can influence erythropoiesis. We ranked genes according to the depletion or enrichment of multiple shRNAs (15) and identified 116 candidates that grouped into categories relevant to terminal erythroid differentiation, including heme metabolism, protein turnover, and apoptosis (Fig. 1C, figs. S1D and S2, and data sets S2 and S3). We validated four top hits (fig. S3 and data set S4). This functional analysis of erythropoiesis provides a framework with which to study host determinants of malaria infection.

To identify factors that influence host susceptibility to P. falciparum infection, we chose to focus on a small subset of the erythrocyte proteome: 42 genes encoding human blood groups. All known P. falciparum receptors fall within this group, and the shRNAs targeting these genes did not appear to affect erythroid development (Fig. 1D). Also, focusing on a small gene set increased the sensitivity to a level required for the inherently complex parasite screen (16).

We transduced hematopoietic progenitor cells (HPCs) with a pooled lentivirus shRNA library targeting the blood group genes (Fig. 2A). At the late orthochromatic erythroblast stage, we infected the knockdown cells with a green fluorescent protein (GFP)–expressing line of P. falciparum strain 3D7. We isolated the parasitized cells and quantified the relative abundance of each shRNA in the population by means of deep sequencing (fig. S4). In parallel, we quantified the abundance of each shRNA in a control population of knockdown cRBCs not exposed to parasites. Hairpins underrepresented in infected cells compared with control cells were considered hits because they may target host genes required for efficient parasite infection.

Fig. 2 Pooled shRNA screen to identify host determinants of P. falciparum infection.

(A) Schematic of blood group shRNA screen. HPCs were transduced with pooled lentivirus library expressing 308 shRNAs targeting 42 blood group genes. Knockdown cRBCs infected with P. falciparum were sorted, and shRNAs were quantified by means of deep sequencing. (B) RIGER analysis ranking results for three independent experiments. Genes were ranked according to NES scores (green heat map). Arrows indicate top hits; asterisks indicate additional candidates.

We ranked candidates from three replicates (Fig. 2B and data set S5) (15). Among the highly ranked genes were basigin (BSG) and CR1, both of which have described roles in P. falciparum invasion (1719). The top-ranked candidate was CD55, also known as decay-accelerating factor (DAF), which carries the Cromer blood group antigens. CD55 is a glycosylphosphatidylinositol-linked complement-regulatory protein that protects cells from lysis by complement (20). On epithelial cells, CD55 is a receptor for bacterial and viral pathogens (2123). Another hit, CD44, defines the Indian blood group and facilitates keratinocyte invasion by group A Streptococcus (24, 25).

For validation, we expressed individual shRNAs targeting CD44 and CD55 in HPCs so as to generate mature red blood cells deficient in CD44 or CD55 (Fig. 3A). Morphological development of the knockdown cells was indistinguishable from control cRBCs (Fig. 3B), as were levels of Band 3, CD49d, and CD71 (fig. S5) (26). To determine whether the amount of CD44 or CD55 on red blood cells influences P. falciparum infection, we assessed parasite invasion into the knockdown cRBCs compared with control cRBCs. We observed ~30% reduction in parasitemia in cells deficient for either CD44 or CD55 relative to control cRBCs (Fig. 3C). The same trend was observed by using alternative shRNAs for CD44 and CD55, suggesting that the results were not because of off-target effects of the shRNAs (fig. S6). Levels of known P. falciparum receptors were unchanged in CD44- and CD55-deficient cRBCs, which suggests that the observed effects on invasion were directly attributable to CD44 and CD55 (fig. S7).

Fig. 3 Validation of CD44 and CD55 as host factors required for P. falciparum invasion.

(A) CD44 and CD55 levels on day 19/20 cRBCs expressing CD44, CD55, or control shRNAs (EmpT). Detection was performed by means of antibody staining and flow cytometry. (B) Morphology of differentiating cRBCs depleted for CD44 and CD55, detected by means of May-Grünwald and Giemsa staining. (C) P. falciparum strain 3D7 invasion assays in control, CD44 knockdown, and CD55 knockdown cRBCs. Three independent biological replicates from two distinct bone marrow donors are shown. Mean ± SD, n = 2 or 3 assays. *P < 0.05, one-tailed t test.

Complete absence of Cromer blood group antigens is rare and has been described in nine individuals with the Inab phenotype, most of whom have stop codons in the CD55 coding sequence (20). Cells from Inab individuals have normal osmotic fragility, do not undergo hemolysis in vivo, and are not particularly susceptible to complement-mediated lysis (27, 28). We used mature erythrocytes from a Japanese patient with the Inab phenotype (termed CD55-null cells) (29) to test whether CD55 has an essential role for P. falciparum invasion. To first characterize any inherent differences between the CD55-null and wild-type (WT) control samples, we adapted plasma membrane profiling (PMP) using tandem mass tag-based mass spectrometry for use in erythrocytes (30). CD55 was absent from the Inab erythrocytes (Fig. 4A). Only two other notable differences were found between the CD55-null and WT cells: a 75% reduction in CR1, which is well within the range of natural variation (19), and a similar reduction in C4BPA, a serum protein that binds to complement regulatory proteins. Only a weak association has been observed between parasite invasion efficiency and natural variation in CR1 levels, and only when all sialylated proteins have been removed from the cell surface (18, 19).

Fig. 4 CD55 is a critical host receptor for P. falciparum.

(A) Scatter plot of plasma membrane proteins identified through PMP of CD55-null erythrocytes relative to controls from two unrelated individuals, and quantified by >2 peptides. (B) Invasion of control erythrocytes (blue) or CD55-null erythrocytes (green) by P. falciparum strain 3D7 or P. knowlesi strain YH1. Asterisk indicates below detection. (C) Invasion by laboratory-adapted P. falciparum strains. (D) Invasion by P. falciparum clinical isolates. Pound sign indicates thin smears showed 0.6 to 1% gametocytes. For (B) to (D), mean ± SD, n = 3 assays. 10,000 cells scored per well by means of flow cytometry. (E) Efficiency of P. falciparum 3D7 merozoite attachment to the surface of CD55-null (green) versus control (blue) RBCs by using cytochalasin D (Cyt D). Invasion was measured in the absence of Cyt D. T1, 30 min; T2, 60 min; and T3, 180 min after addition of schizonts (fig. S10). Attachment to controls at T1 was 3.6 to 5.3%. Mean ± SD, n = 2 biological replicates. 20,000 cells scored per well by means of flow cytometry.

To determine the contribution of CD55 to P. falciparum infection in mature erythrocytes, we used the CD55-null cells in invasion assays. The CD55-null erythrocytes were refractory to invasion by P. falciparum strain 3D7, which suggests that host CD55 is essential for parasite infection (Fig. 4B). This finding suggests that the reduced but substantial parasitemia observed in the cells in which CD55 was knocked down depended on residual CD55. The CD55-null cells were similarly nonsusceptible to invasion by additional laboratory-adapted P. falciparum strains, including the CR1-independent W2mef line (Fig. 4C). Parasite invasion was also significantly impaired in erythrocytes from a second, unrelated Inab patient with a different genetic basis for the condition (fig. S8A) (31). Proliferation of parasites was also diminished in these Inab cells (fig. S8B), which suggests that CD55 would be required to support a productive malaria infection.

Besides laboratory-adapted strains, several clinical isolates of P. falciparum from Senegalese patients were also dependent on CD55 for invasion (Fig. 4D), providing additional evidence that CD55 is likely a critical host factor for all P. falciparum strains. In contrast to P. falciparum, the zoonotic human malaria parasite P. knowlesi invaded CD55-null and WT erythrocytes with similar efficiency (Fig. 4B). Thus, CD55 on human erythrocytes may interact with a parasite ligand specific to P. falciparum that is not expressed by other malaria parasites. Deletion of known invasion ligands (EBA140, EBA175, EBA181, RH1, RH2a, or RH2b) did not enable parasite invasion in the absence of CD55 (fig. S9).

To determine whether CD55 is involved in attachment of P. falciparum to the erythrocyte or at a later stage of the invasion process, we used cytochalasin D to enable isolation of cells with parasites adhered to the outer surface (32). Initially, attachment of P. falciparum merozoites was similar for the CD55-null and WT cells, but over time, parasites selectively detached from the cells lacking CD55, mirroring the invasion defect (Fig. 4E). Thus, CD55 may not be required for the primary interaction of merozoites with the RBC surface, but instead be critical for the stage of committed, irreversible attachment seen during formation of the tight junction (33).

Our results reveal an essential role for CD55 in P. falciparum invasion of human red blood cells. Levels of CD55 vary dynamically during clinical malaria and may influence the course of infection (34). Moreover, we identified two CD55 polymorphisms significantly enriched in persons with ancestral exposure to malaria (Table 1) (35), both of which have been previously described almost exclusively in individuals of African descent (20).

Table 1 Geographic distribution of CD55* coding variants as percent of population, from the 1000 Genomes Project, phase I.

CD55 isoform ENST00000367064 (DAF-2).

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The existence of hematologically normal individuals completely lacking CD55 suggests that targeting CD55 on erythrocytes would not elicit substantial toxicity. In light of its critical role in parasite infection, CD55 could serve as an attractive target for the development of malaria therapeutics. Aside from CD55, the only other known strain-transcendent receptor for P. falciparum, basigin, binds to RH5, which is a leading malaria vaccine candidate (17, 36, 37). Our studies also establish the feasibility of forward genetic cellular screening by use of cultured erythrocytes derived from HSCs to identify critical host determinants of P. falciparum malaria biology and pathogenesis.

Supplementary Materials

www.sciencemag.org/content/348/6235/711/suppl/DC1

Materials and Methods

Supplementary Text

Figs. S1 to S10

References (3842)

Data sets S1 to S5

References and Notes

  1. Materials and methods are available as supplementary materials on Science Online.
  2. Supplementary text is provided as supplementary materials on Science Online.
  3. Acknowledgments: We thank D. Wirth, M. Ganter, A. Nicholson-Weller, M. Waldor, S. Lux, R. Husson, B. Burleigh, and members of the Duraisingh Laboratory for helpful discussions and reading of the manuscript. We thank C. Westhoff and C. Lomas-Francis of the New York Blood Center for gift of the second Inab sample. We thank U. Kanjee for technical assistance and D. Ndiaye, S. Mboup, and S. Volkman for P. falciparum clinical isolates from Senegal. This work was supported by a Gates Foundation Grand Challenges Exploration Award OPP1035276 (M.T.D.), NIH grant R01AI091787 (M.T.D.), a Pediatric Scientist Development Program Fellowship from the Eunice Kennedy Shriver National Institute of Child Health and Human Development K12-HD000850 (E.S.E), NIH grant K08 1K08AI103034-01A1 (E.S.E.), Boston Children’s Hospital Faculty Development Award (E.S.E.), NIH grant K01DK098285 (J.A.P.), and the Cambridge Biomedical Research Center, UK (M.P.W. and L.V.N.). Additional data can be found in the supplementary materials.

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