Calcium Dependent Protein Kinases are key effectors of calcium signaling in malaria parasite. PfCDPK1 is critical for asexual development of Plasmodium falciparum, but its precise function and substrates remain largely unknown. Using a conditional knockdown strategy, we here establish that this kinase is critical for the invasion of host erythrocytes. Furthermore, using a multidisciplinary approach involving comparative phosphoproteomics we gain insights into the underlying molecular mechanisms. We identify substrates of PfCDPK1, which includes proteins of Inner Membrane Complex and glideosome-actomyosin motor assembly. Interestingly, PfCDPK1 phosphorylates PfPKA regulatory subunit (PfPKA-R) and regulates PfPKA activity in the parasite, which may be relevant for the process of invasion. This study delineates the signaling network of PfCDPK1 and sheds light on mechanisms via which it regulates invasion.
Protozoan parasite Plasmodium falciparum is a major causative agent of pernicious human malaria, which infects the mosquito and the human host. Plasmodium infects two different cell types in the human host; hepatocytes and the erythrocytes and encounters diverse host environments, which it successfully survives to propagate. The asexual development of the parasite involves invasion of host RBCs by the parasite followed by its intraerythrocytic development, multiplication and egress to invade fresh RBCs, which results in clinical manifestations and pathogenesis of disease. While it has become increasingly clear that the subtle regulation of parasite developmental processes occurs via signaling events, the underlying pathways are poorly understood at the molecular level. Calcium signaling is a central player that regulates almost all developmental stages of the parasite1, 2. The parasite entraps calcium, which it possibly acquires during invasion3, in intracellular stores and uses it judiciously during the course of its development. Phospholipase C4, as well as cADP-ribose pathways5 have been shown to exist in the parasite and are involved in host cell invasion and sexual differentiation4, 6.
The malarial parasite possesses unique sets of calcium effectors Calcium Dependent Protein Kinases (CDPKs), which are absent from the host but regulate processes in Plasmodium and related apicomplexan Toxoplasma gondii 1, 2. While the parasite seems to lack the classical Calmodulin dependent protein kinases (CamKs), CDPKs possess a Calmodulin Like Domain at their C-terminus via which calcium dependent activation of the enzyme occurs7. PbCDPK4 regulates sexual differentiation of the rodent parasite P. berghei and PfCDPK5 guides the egress of merozoites from the host erythrocyte8. CDPKs regulate important processes in T. gondii as well. For instance, TgCDPK1 is involved in microneme secretion triggered by calcium9. While PbCDPK1 is not essential for P. berghei asexual development10, independent reports have suggested that PfCDPK1 is refractory to gene disruption11, 12, indicating that it may be indispensable for asexual blood stage development of P. falciparum. Insights into the putative role of PfCDPK1 in P. falciparum have come from studies using a pharmacological inhibitor purfalcamine11, and peptide inhibitors13 which have suggested that PfCDPK1 may be involved in egress from the RBC and/or invasion. Since these inhibitors and other tools are likely to “hit” other targets, the specific function of CDPK1 in P. falciparum life cycle remains largely unknown and a genetic approach was needed to specifically determine its role in parasite biology.
We have used a conditional “knockdown” approach to dissect the role of PfCDPK1 in the process of host RBC invasion. Quantitative phosphoproteomics was employed for the identification of potential PfCDPK1 targets in the parasite to gain insights into its putative role in this process. PfCDPK1 may contribute to the process of invasion by regulating key parasite proteins, which include proteins of the inner membrane complex (IMC) and cAMP signaling module. Present studies also identify molecular interactions via which calcium and cAMP pathways may cross-talk in the parasite.
Conditional knockdown of PfCDPK1 in P. falciparum
To elucidate the function of PfCDPK1 and identify its putative substrates, we generated parasites in which PfCDPK1 expression was down regulated. Since PfCDPK1 is refractory to gene disruption11, 12, a FKBP destabilization domain (DD) strategy was used to conditionally regulate its expression in P. falciparum 14. The DD-fusion proteins are unstable in the absence of the DD ligand Shield-1 (Shld-1), which allows conditional knockdown of fused proteins. Using a single crossover strategy, PfCDPK1 was fused to the triple HA- tag followed by a DD domain at its C-terminus (Fig. 1a, Supplementary Fig. 1) to obtain PfCDPK1-3HA-DD parasites, which were cultured in the presence of Shld-1. The removal of Shld-1 resulted in ~70% reduction of PfCDPK1 expression as quantified by western blotting (Fig. 1b).
Identification of potential PfCDPK1 substrates
In order to elucidate the mechanism via which PfCDPK1 interplays with cellular processes of the parasite, it was important to globally identify proteins that undergo PfCDPK1-dependent phosphorylation in the parasite to unravel CDPK1 signaling pathways. The phosphoproteome of PfCDPK1-3HA-DD parasites was compared in the presence or absence of Shld-1. During asexual blood stage reproduction, PfCDPK1 exhibits maximum expression in late schizont stages and merozoites15. Therefore, it was pertinent to use these stages for phosphoproteomics. Shld-1 was removed at the ring stage and late schizont lysates were prepared for phosphoproteomic analysis. A mass spectrometry-based quantitative phosphoproteomic and proteomic approach involving iTRAQ labeling to measure differences in the phosphorylation state of proteins upon PfCDPK1 knockdown was employed (Fig. 1c). These studies resulted in identification of 2057 unique phosphosites from 1233 P. falciparum proteins (Fig. 1d, Supplementary Data 1). Several of these peptides exhibited differential phosphorylation upon PfCDPK1 knockdown achieved by Shld-1 removal (Fig. 1d, Supplementary Data 1).
Proteins that exhibited >0.75 fold change in phosphorylation in at least two replicates at specific residues upon PfCDPK1 ablation were considered as significant (Supplementary Data 1). This cutoff range was defined by using the PfCDPK1-dependent phosphorylation of S103 in PfGAP45 as an internal standard, as this protein was previously demonstrated to be phosphorylated by PfCDPK1 in vitro15. This glideosome-associated protein is expressed in late stage parasites and showed a ~0.75 fold reduction in phosphorylation at S103 upon PfCDPK1 knockdown, which could be detected using a S103 specific phospho-antibody (Fig. 2a, see below).
Since PfCDPK1 is a kinase, the proteins that exhibited significant reduced phosphorylation upon its depletion were of specific interest. In all, 79 sites from 64 proteins exhibited significant decrease in phosphorylation in at least two replicates (Fig. 1d, Supplementary Data 2). Motif analysis of hypophosphorylated peptides showed overrepresentation of certain conserved amino acid sequences spanning the altered phosphorylation sites. Interestingly, most represented motifs comprised of basic amino acids with a preference for an R (or K) preceding the target S/T (Fig. 1f, Supplementary Data 2). These data agree well with previously identified preferred motifs for CDPK phosphorylation16. In addition, motifs in which target S/T were followed by acidic D/E residues were also found to be modulated (Fig. 1f, Supplementary Data 2).
Gene Ontology (GO) analysis suggested that a number of differentially phosphorylated proteins may be involved in invasion and/or motility (Fig. 1e, Supplementary Data 2). Several ribosomal proteins, proteins involved in RNA metabolism and processing, were also part of this group, but they are unlikely to be a direct PfCDPK1 targets. Surprisingly, the low molecular weight rhoptry complex containing RAMA and RAP1 also appeared to be modulated by PfCDPK1.
The regulatory subunit of cAMP dependent Protein Kinase (PfPKA-R) exhibited a change in its phosphorylation status at S149, which was just above the indicated threshold in phosphoproteomic analysis (Fig. 1d, Supplementary Data 1). Importantly, this phosphorylation site was part of a motif closely related to PfCDPK1 target motifs mentioned above. Since PfPKA-R is a key signaling molecule of the cAMP pathway, which our preliminary studies had implicated in PfCDPK1 function, it was also validated and pursued for further studies (described below).
Interestingly, a large number of putative target proteins were predicted or known to be associated with the IMC and the parasite pellicle (Fig. 1e, Supplementary Fig. 2, Supplementary Data 2), a membranous structure that underlies the plasma membrane. Given the membrane localization of PfCDPK1, which is facilitated by its N-terminus lipid modification and its previously reported interaction with IMC proteins in the membrane17, 18, these findings corroborated well and raised the possibility of these targets in close proximity of PfCDPK1.
We predicted the likelihood of protein–protein interactions (PPI) among the differentially phosphorylated proteins identified in our study from STRING database (Fig. 1g, Supplementary Data 3), which is a resource of PPI that have emerged either from direct experiments reported in the literature and predicted on the basis of co-expression and gene arrangement in the genome19. STRING has been used successfully to predict PPI in Plasmodium 20. STRING analysis demonstrated a confident clustering PPI among the candidate proteins, which supports the results obtained by comparative phosphoproteomic analysis (Fig. 1g). Importantly, PfCDPK1 was predicted to be involved intimately with several of its targets identified by phosphoproteomics such as GAP45 and IMC1g that were validated during the course of these studies.
PfCDPK1 is involved in the phosphorylation of IMC proteins
Several IMC proteins, which are part of the actomyosin motor like GAP45 and Myosin A, or other IMC proteins such as IMC1c (ALV5), IMC1g (ALV4) associated with the IMC protein meshwork exhibited reduced phosphorylation upon PfCDPK1 knockdown (Fig. 1d). Previous studies have indicated that PfCDPK1 co-localizes with the Myosin Tail Interacting Protein, as well as Merozoite Surface Protein 1 (MSP1) in both schizonts and free merozoites17 suggesting that it is in close proximity to the IMC and plasma membrane. As mentioned above, PfGAP45-which was previously demonstrated to be an in vitro substrate of PfCDPK115, 21-exhibited differential phosphorylation at S89 and S103 (Fig. 1d, Supplementary Data 2). Using an antibody which recognizes S103 phosphorylated PfGAP4515, we were able to demonstrate that PfGAP45 phosphorylation at this site is indeed reduced upon PfCDPK1 knockdown (Fig. 2a) and supported the phosphoproteomics data (Fig. 1d). In addition, two other IMC proteins PfIMC1g (PF3D7_1003600) (Fig. 2b) and PfIMC1c (PF3D7_0525800) were differentially phosphorylated (Fig. 1d). PfCDPK1 phosphorylated IMC1g in vitro (Fig. 2c). Importantly, metabolic labeling revealed that PfCDPK1 depletion resulted in reduced phosphorylation of PfIMC1g (Fig. 2d). These data strongly suggested that PfCDPK1 is a major kinase that phosphorylates IMC1g in the parasite. Moreover, PfCDPK1 exhibited localization in close proximity with IMC1g (Fig. 2e) in the parasite, which was reflected by overlapping fluorescence in IFA. In addition, the fact that IMC1g immunoprecipitated with PfCDPK1 suggested its interaction with the kinase in the parasite (Fig. 2f).
Regulation of PfPKA by PfCDPK1
Recently published reports have hinted at a cross talk between cAMP and calcium signaling during invasion22. However, the underlying molecular mechanisms are poorly understood. cAMP mediates signaling via cAMP dependent protein kinase (PKA) in most organisms including the malaria parasite23. Therefore, we investigated the possibility of PfPKA regulation by PfCDPK1. To this end, PfPKA-C was immunoprecipitated and its activity was assayed upon PfCDPK1 knockdown. Interestingly, a significant decrease in its activity upon PfCDPK1 knockdown suggested that PfCDPK1 regulates PfPKA-C in the parasite (Fig. 3a).
As mentioned above, analyses of phosphoproteomic data revealed that the phosphorylation of PfPKA-R was down regulated at S149 upon PfCDPK1 knockdown in one of the replicates (Supplementary Data 1, Fig. 3b). It was worth noting that S149 belongs to K/RRxSxS motif (Fig. 3d), which is very closely related to one of the major PfCDPK1 target motifs indicated above (Fig. 1f) that were enriched among significantly altered phosphopeptides. In order to confirm if PfPKA-R is a substrate of PfCDPK1, in vitro kinase assays were performed using recombinant PfPKA-R. Indeed, PfCDPK1 phosphorylated PfPKA-R in vitro (Fig. 3c, Supplementary Fig. 3b). In addition to S149, in vitro phosphorylation of other sites of PfPKA-R was detected by LC–MS/MS studies (Fig. 3c, Supplementary Fig. 3a).
To confirm that PfPKA-R phosphorylation is compromised upon PfCDPK1 depletion, metabolic labeling of parasite proteins with 32P-labelled orthophosphate was followed by PfPKA-R-IP. These experiments revealed reduction in phosphate incorporation in PfPKA-R upon PfCDPK1 ablation, which indicated that PfCDPK1 is involved in PfPKA-R phosphorylation (Fig. 3e). An antibody against the S149-phosphorylated form of PfPKA-R, which mainly recognizes the S149 phosphorylated form of PfPKA-R was custom generated (Supplementary Fig. 3c). Using this antibody, a decrease in its phosphorylation at S149 was observed upon PfCDPK1 depletion (Fig. 3f). IFAs were performed to check if PfPKA-R and PfCDPK1 co-localized in late schizont parasites. PfCDPK1 exhibited co-localization with PfPKA-R (Supplementary Fig. 4c). In addition, co-immunoprecipitation of PfPKA-R with PfCDPK1 indicated their association in the parasite (Fig. 3h). PfPKA-R-PfCDPK1 interaction was also observed in parasites that overexpress PfPKA-R (Supplementary Fig. 4b).
S149, which is the target site of PfCDPK1 in the parasite, resides in the Inhibitory Segment (IS) of PfPKA-R (Fig. 3d). While cAMP binding to PKA-R is essential for dissociation of the R and the C subunits, subsequent phosphorylation of the IS contributes to this process and catalytic activation of the C subunit in the case of mammalian PKA24. The IS sequence is reasonably well conserved in mammalian and Plasmodium PKA-R and S149 aligns with corresponding site in PKA-R from other species23 (Fig. 3d). The impact of PfCDPK1 knockdown on PfPKA-R/PfPKA-C interaction was analyzed by performing co-immunoprecipitation experiments. PfPKA-R was pulled down with PKA-C in the presence of Shld-1 (Fig. 3g). Upon Shld-1 removal, there was a significant increase (Fig. 3g) in binding of these proteins, which suggested that PfCDPK1 may prevent interaction between the R and the C subunits of PfPKA. PfCDPK1 is activated by calcium, which induces conformational change that facilitates this process7. Co-IP experiments revealed that chelating intracellular calcium by BAPTA-AM resulted in a loss of PfPKA-R-PfCDPK1 interaction (Fig. 3h) suggesting that calcium-induced effects on PfCDPK1 are required for its binding to PfPKA-R. In contrast, BAPTA-AM treatment resulted in an increase in PfPKA R and C subunits (Fig. 3i) and a corresponding decrease in PfPKA activity (Supplementary Fig. 4a). Collectively, these data indicated that PfCDPK1 interacts and phosphorylates PfPKA-R in a calcium dependent manner, which may contribute to dissociation of PfPKA R and C subunits and promote the activation of PfPKA-C.
A negative feedback loop between PfCDPK1 and PfPKA
In independent preliminary studies that were directed at understanding the effect of cAMP on calcium signaling, we noted that modulation of cAMP levels impacted PfCDPK1 activity. Strikingly, phosphodiesterase inhibitor IBMX, which sustains cAMP levels in the parasite22 and addition of 8Br-cAMP to parasites caused a significant decrease in PfCDPK1 activity (Fig. 4a). These data indicated that cAMP signaling may negatively regulate PfCDPK1 activity. The next logical step was to investigate the involvement of PfPKA in this process. We used parasites that overexpressed PfPKA-R as GFP fusion protein under AMA-1 promoter, which ensured its expression in schizont and segmenter stages. The overexpression of PfPKA-R sequesters PfPKA-C, which results in suppression of its activity and increasing cellular cAMP by addition of 8Br-cAMP to parasites resulted in elevation of the activity (Fig. 4b, red bars). In contrast, PfCDPK1 activity was significantly reduced (Fig. 4b, blue bars). A reverse experiment was also performed in which parasites were treated with a PKA inhibitor peptide PKI, which directly inhibits PfPKA-C25, 26. This inhibitor caused a significant increase in PfCDPK1 activity (Fig. 4c). Collectively, these data suggested that PfPKA-C may negatively regulate PfCDPK1 in the parasite.
Next, the direct effect of PfPKA-C on PfCDPK1 activity was assessed by performing in vitro kinase assays using recombinant PfCDPK1. Since recombinant PfPKA-C is catalytically inactive, a parasite line that over expresses PfPKA-C fused to 3xHA tag was used to immunoprecipitate PfPKA-C-HA and IP was used as a source of active PfPKA27. PfPKA-C-IP was incubated with PfCDPK1 in the absence or presence of unlabelled ATP, which was added to facilitate possible phosphorylation of PfCDPK1 by PfPKA-C. Subsequently, PfCDPK1 was separated from PfPKA-C-HA-IP. The activity of PfPKA-phosphorylated PfCDPK1 (+ATP, Fig. 4d, lane 2), or the unphosphorylated (-ATP, Fig. 4d, lane 3) was compared by performing assays using 32P-labelled ATP and MBP, which was used as a phosphoacceptor substrate for PfCDPK1. A significant decrease in PfCDPK1 activity was detected when PfPKA-C-HA-IP was added along with cold ATP (Fig. 4d, lane 2) in comparison to the reaction in which cold ATP was excluded from the first step of the assay (Fig. 4d, lane 3). In addition, a control IP of an unrelated protein failed to alter PfCDPK1 activity (lane 1). These results indicated that PfPKA-C may inhibit PfCDPK1 activity. The observed negative feedback loop may be mechanism via which PfPKA may down regulate or shut down PfCDPK1 in the parasite.
PfCDPK1 may regulate RBC invasion by the parasite
PfCDPK1 seems to regulate a variety of parasite proteins, which possibly explains its importance for blood stage development11, 12. Efforts were made to understand the process it may regulate during blood stage development. To this end, the effect of PfCDPK1 knockdown on parasite growth was assessed by culturing parasites in the absence of Shld-1. A decrease in parasitemia was observed after each cycle, which was even more accentuated after the second cycle (~2 fold, Fig. 5a). Since decrease in parasitemia was observed mainly after each cycle and because PfCDPK1 is expressed mainly in schizonts15, a defect in egress or invasion was suspected. Next, we tested if the knockdown of PfCDPK1 had an impact on the invasion of host RBCs. To achieve this, Shld-1 was removed from ring stage parasites and schizonts were used for the invasion assays. Schizonts ruptured normally in the absence or presence of Shld-1 and were rarely observed after ~6 h of incubation with fresh erythrocytes suggesting that PfCDPK1 knockdown did not cause an apparent defect on egress. However, a significant decrease in the invasion, which was indicated by reduction in freshly formed rings, was observed in the case of Shld-1 deprived parasites (Fig. 5b). The invasion of RBCs by merozoites is a multi-step process initiated by the attachment to the RBC28. We tested if PfCDPK1 may regulate invasion by regulating the process of attachment. For this purpose, cytochalasin D (Cyt D) an inhibitor of actin polymerization, which allows attachment but prevents RBC entry29, 30 was used. Cyt D treated parasites from Shld-1+/− cultures were allowed to rupture and release merozoites that attached to erythrocytes. A significant decrease in parasites attached to erythrocytes was observed when PfCDPK1 was depleted (Fig. 5c) implicating PfCDPK1 in the host RBC attachment.
Invasion of host RBCs by Plasmodium is regulated by adhesins secreted by the parasite’s apical organelles called rhoptries and micronemes, which serve as ligands for receptors on host RBC surface2, 31. Therefore, the effect of PfCDPK1 knockdown on the secretion of major invasion ligands was tested. Western blotting of the culture supernatant containing secreted proteins revealed that the release of DBL domain protein EBA-175, which is a key invasion molecule32, was significantly reduced upon PfCDPK1 knockdown (Fig. 5d). However, another microneme protein AMA-1, which is involved in tight junction formation33, 34 did not exhibit a significant change. In addition, the exocytosis of rhoptry neck protein RH535, which is involved in sialic acid-independent invasion, also remained largely unchanged in comparison to EBA-175 (Supplementary Fig. 5).
For the invasion of host erythrocytes, P. falciparum interacts with the sialic acid present on glycophorin A at the host surface via the EBL family of invasion ligands like EBA-175, which are released from the micronemes. In addition, it utilizes sialic acid independent pathways, which typically involve RH family members31. We probed if PfCDPK1 regulates both sialic acid-dependent and -independent pathways for invasion. The fact that PfCDPK1-3HA-DD parasites were generated in the D10 strain background allowed us to address this issue, as these parasites exhibit sensitivity towards neuraminidase36. When RBCs were treated with neuraminidase, it resulted in a significant decrease in invasion of control (Shld-1+) parasites (Fig. 5e, 1st bar vs. 3rd bar). While Shld-1 removal ablated invasion of untreated RBCs (1st bar vs. 2nd bar, Shld-1), the effect was less significant in the case of RBCs treated with Nm (3rd vs. 4th bar). These data suggested that PfCDPK1 may regulate invasion via a sialic acid-dependent receptor. While glycophorin A is resistant to chymotrypsin, there are several receptors for other parasite adhesins that are sensitive to chymotrypsin31. There was almost no difference in invasion efficiency of PfCDPK1-3HA-DD (Fig. 5f, 1st bar vs. 3rd bar) upon chymotrypsin treatment, which is consistent with parental D10 line being refractory to chymotrypsin treatment36, 37. PfCDPK1 depletion caused a similar defect in invasion of chymotrypsin-treated RBCs, as was the case with untreated RBCs (Fig. 5f, 1st bar vs. 2nd bar and 3rd bar vs. 4th bar). These data suggested that the observed invasion defects might be mainly due to the inability of the parasites to use the EBA-175/glycophorin A pathway.
Regulation of invasion by PfCDPK1 and PfPKA
Previously, cAMP and PfPKA were implicated in microneme secretion22. Our studies suggested that PfPKA activity is regulated by PfCDPK1 (Fig. 3), therefore, attempts were made to see if this cross-talk may contribute to invasion. First, PfPKA-R-GFP parasites were used to confirm the role of PfPKA in invasion22, 27. An increase in the formation of rings was observed upon an increase in cAMP levels and schizont rupture remained almost unaltered (Fig. 6a), which was indicative of enhanced invasion and was consistent with a previous report22. The PKA-inhibitor PKI was also used to inhibit PfPKA in PfCDPK1-3HA-DD parasite-infected red blood cells. A marked reduction in invasion by PKI was observed (Fig. 6b, 1st bar vs. 3rd bar) in control Shld-1 treated parasites with normal PfCDPK1 expression implicating PfPKA in this process. While PfCDPK1 depletion (Shld-1) reduced invasion (Fig. 6b, 1st bar vs. 2nd bar), PKI was unable to cause an additional defect (4th bar vs. 2nd and 3rd bar). The significantly decreased sensitivity to invasion by the PKA-inhibitor when PfCDPK1 was depleted suggested that PfCDPK1-mediated regulation of PfPKA may contribute to the invasion process.
In summary, the present studies suggest PfCDPK1 may regulate invasion via phosphorylation and interaction with key proteins involved in IMC and glideosome function. Since PfCDPK1 and PfPKA regulate RBC invasion and PfCDPK1 is an upstream activator of PfPKA, it is reasonable to propose that their cross talk may contribute to the process of invasion (Fig. 6c).
While PbCDPK1 was considered to be non-essential for the growth of P. berghei 10, conditional knockdown of PbCDPK1 resulted in severe defects in ookinete differentiation and mosquito transmission38. Previous studies suggested that PfCDPK1 may be a critical enzyme, as its gene-disruption was not possible in P. falciparum 11, 12. Despite these studies, the function of PfCDPK1 in blood stage development of the human parasite had remained elusive. The present studies indicate that PfCDPK1 may regulate the invasion of host RBCs by P. falciparum, which corroborated well with its ability to regulate EBA-175 secretion. Interestingly, PfCDPK1 can complement TgCDPK3, which is its closest Toxoplasma homologue, and salvages the egress phenotype in T. gondii 39. The sialic acid -dependent invasion pathway, which involves interaction between DBL domain containing proteins like EBA-175 and the sialic acid moiety of glycophorins, was impaired upon PfCDPK1 depletion. However, invasion via chymotrypsin-resistant receptors like basigin35, 40 was not affected significantly. It will be surprising if PfCDPK1 specifically inhibits the sialic acid-dependent invasion events as it seems to target substrates, which may ubiquitously regulate the invasion process. It is possible that residual 30–40% expression of PfCDPK1 after Shld-1 removal may be sufficient for other pathways to operate. A recent study reported that knockdown of PfCDPK1 using the DD-FKBP domain did not alter parasite growth13. However, the knockdown obtained in these studies was nominal. GFP along with the DD domain was fused to PfCDPK1 instead of a HA-tag in these studies, which may have a bearing on the extent of PfCDPK1 degradation. In addition, the background parasites used were 3D7 in this case, which are largely insensitive to neuraminidase treatment and predominantly use the sialic acid-independent pathway31. The J-domain of PfCDPK1, which is inhibitory for kinase activity, caused parasite arrest in early schizogony and egress from parasites. It was rightly concluded from these studies that the J-Domain may also target proteins other than PfCDPK113.
PfCDPK1 seems to regulate several proteins of the actomyosin motor and glideosome assembly, which connects the motor to the IMC. One of the features of network analysis was the connectivity exhibited by PfCDPK1 to proteins belonging to these complexes. Out of these, only PfGAP4515, 18 was previously implicated in PfCDPK1 signaling. Since almost all previous studies have been based on in vitro phosphorylation experiments, their association with and regulation by PfCDPK1 in the parasite remained to be established, which was possible by using PfCDPK1-3HA-DD parasites. PfGAP45 is phosphorylated at several sites other than S89 and S103. While mutation of some of these sites to A/D residues and overexpression of mutants did not alter glideosome function15, 21 it is likely that the cumulative effect of phosphorylation of these and other sites by kinases like PfPKG41 may regulate its function in Plasmodium. Other IMC proteins such as IMC1g/PfALV4 (PF3D7_0525800) and IMC1c/PfALV5 (PF3D7_10003600), which are alveolins42, were differentially phosphorylated upon PfCDPK1 knockdown. Both proteins are known to be heavily phosphorylated41, 43 and it will be interesting to dissect the role of their phosphorylation on IMC assembly and function. Interestingly, low molecular weight complex proteins RAMA-RAP1 were differentially phosphorylated upon PfCDPK1 depletion. Since PfCDPK1 does not seem to reside in rhoptries, it is possible that it may interact with these proteins in lipid rafts during trafficking, which was supported by a previous proteomics study that indicated44 the presence of these proteins in lipid rafts.
While a cross-talk between cAMP and calcium pathways has been reported in Plasmodium 22, 25, molecular interactions that guide it have largely remained unclear. We identified PfPKA-R as a substrate for PfCDPK1. The major phosphorylation site-S149, which is phosphorylated by PfCDPK1, resides in the inhibitory sequence, which lies upstream of the nucleotide binding domain (Fig. 3c). The crystal structure of the mammalian PKA complex indicates that IS docks into the active site of PKA-C rendering it to be inactive by engaging key residues24. Indeed, S149 phosphorylation of PfPKA-R was mediated by PfCDPK1 in the parasite, as suggested by use of a specific anti-pS149 antibody and co-immunoprecipitation of PfPKA-R and PfCDPK1 established their interaction in the parasite. PfCDPK1 knockdown results in enhanced interaction between R and C subunits of PfPKA-R, which corroborated well with the decrease in PfPKA-C catalytic activity. Therefore, it is reasonable to conclude that the phosphorylation and/or binding with PfCDPK1 promote the dissociation of PfPKA-R from PfPKA-C, which results in PKA-C activation. Given that K/RRxS motif that encompasses S149, may also be targeted by other kinases like AGC kinases and therefore, may be a key nodal site for cross talk of cAMP signaling with other signaling pathways as well.
A negative feedback loop via which PfCDPK1 activity can be turned off by PfPKA-C also emerged from present studies. Even though, we have not identified a PfPKA target site on PfCDPK1, it appears that PfPKA-C activity may contribute towards PfCDPK1 down regulation. A recent study suggested that PfPKG may phosphorylate PfCDPK1 at S64 and phosphorylation of this site was proposed to target PfCDPK1 to apical structures41. Our previous work demonstrated that S64 can be autophosphorylated by PfCDPK1 and mutation of this site does not cause a major change in its activity7. Therefore, the mechanism of PfCDPK1 regulation by PfPKA and PfPKG may be distinct, which will be interesting to elucidate. While this manuscript was under review, it was reported that the replacement of the gatekeeper residue in ATP-binding site attenuated PfCDPK1 activity and parasites expressing the gatekeeper mutant-PfCDPK1 were more sensitive to PfPKG inhibitor C2. Although direct demonstration was not provided, it was suggested that PfPKG or its downstream kinases might compensate for the loss of PfCDPK1 activity45, which will be an interesting proposition to test.
Previous reports have also suggested that PfPKA may regulate the secretion of microneme proteins like AMA-1 and EBA-17522, 27. We found mainly a defect in EBA-175 exocytosis and not in AMA-1, although, the possibility of residual ~30% PfCDPK1 being sufficient for AMA-1 release cannot be ruled out. Present studies highlight a novel hub involving PfCDPK1-PfPKA interaction for the cross-talk between calcium and cAMP pathways. Like PfCDPK1, PfPKA is also critical for blood stage development of P. falciparum 12. Inhibition with generic PKA inhibitors like H89 and PKI25, 26 implicated it in asexual development and invasion. Using PKI and transgenic PKA-R overexpressing parasites, we confirmed a role of PfPKA in RBC invasion. While PKI blocked invasion, its addition did not result in an additive effect upon PfCDPK1 knockdown, which hinted that PfCDPK1-mediated activation of PfPKA may be critical for invasion. While it is largely a correlation, it is indeed possible that PfCDPK1 may mediate EBA-175 secretion via PfPKA, as both these kinases regulate this process. Collectively, the present studies demonstrate the involvement of PfCDPK1 in regulating key modules like the IMC and cAMP signaling in the parasite, which might shed light on the mechanism via which it regulates host RBC invasion.
Reagents and antibodies
All the molecular biology reagents were purchased from Sigma-Aldrich. Oligonucleotides were procured form Sigma-Aldrich, restriction enzymes were obtained from New England Biolabs, USA. Commercially available antibodies were obtained from Santa Cruz Biotechnology (mouse anti- β-Actin (1:500, C4, sc-47778 HRP), rabbit anti-HA (1:500, Y-11, sc-805) and rabbit anti-GAPDH (1:500, FL 335, sc-25778)). Protein A/G plus agarose beads (sc-2003) were obtained from Santa Cruz Biotechnology. Anti-EBA-175 antibody was obtained from MR4 (1 : 1000, MRA-2). Other antibodies were kindly gifted by Dr. Chetan Chitnis, Institute Pasteur, Paris (1 : 1000, rabbit anti-AMA1), Prof. Alan Cowman, Walter & Eliza Hall Institute (1 : 2500, rabbit anti-RH5), Dr. Anthony A. Holder (1 : 2000 rabbit anti-GAP45). Shld-1 was purchased from Cheminpharma, LLC, USA. PKA Inhibitor PKI was obtained from Enzo life sciences (PKI14-22 amide, myristoylated), 8Br-cAMP, BAPTA-AM, Neuraminidase, trypsin, chymotrypsin were obtained from Sigma-Aldrich.
Generation of transgenic parasites
For C-terminal tagging of PfCDPK1 locus with 3HA-DD, ~1.1 kb of the 3′end of the PfCDPK1 ORF (PlasmoDB ID PF3D7_0217500) without the stop codon was PCR amplified from P. falciparum genomic DNA (strain D10) with primers oJDD400 (5′-TAGGCGGCCGCTTAGTAACCGAATTTTATGAAGGTGGGG) and oJDD62 (5′- TAGCTCGAGTGAAGATTTATTATCACAAATTTTGTGCATCATG). The amplicon was ligated into 3HA-DD plasmid46 between the restriction sites NotI and XhoI, upstream and in-frame with the coding sequence of the 3HA and DD-tags8, 37. The PfCDPK1-3HA-DD plasmid, which has the human DHFR selection cassette, was prepared by using Qiagen Maxi prep kit. Approximately 100 µg plasmid DNA was transfected into D10 strain (WEHI) and selected using 5 nM WR99210 (gifted by Jacobus Pharmaceuticals). Integration of the plasmid was promoted by several cycles of drug treatment (~1 week) followed by culturing parasites without drug (~3 weeks). When parasites became resistant to WR99210 after a prolonged period off-drug, parasites were cloned by limiting dilution in a 96 well plate (nominal density, 3 parasites per 10 wells). The integration of 3HA-DD at the PfCDPK1 locus was confirmed by genotyping PCR, for which PCR primers were designed to amplify the endogenous locus, the 3′integration and the episome (see Supplementary Fig. 1). Furthermore, the 3′-integration amplicon was cloned and sequenced to confirm the integration at the desired locus.
The PfPKA-R overexpressing cell line was designed using the pARL-GFP vector47. The full length gene (PF3D7_1223100) was PCR amplified using Phusion DNA polymerase and PKA-RGFP_F and PKA-RGFP_R, KpnI/ AvrII digested and cloned into the digested pARL-GFP plasmid. The chimeric gene containing the open reading frame of PfPKA-R and GFP is driven by the late stage specific AMA1 promoter mimicking the expression profile of the endogenous PfPKA-R gene. The construct was sequenced and analyzed for accuracy.
Parasite culture and transfections
P. falciparum asexual blood stages were cultured in O+ erythrocytes according to standard procedures48. In addition, 3D7 (MR4) were transfected with 100 µg of purified plasmid DNA, as described previously49. Positive selection of transfected parasites was achieved by addition of 10 nM WR99210, an antifolate that selects for the presence of the human DHFR gene. P. falciparum lines were cultured in complete RPMI 1640 medium with 0.5% albumax and gassed with 7% CO2, 1% O2 and 88% N2 at 37 °C. Synchronization of parasites was achieved by treatment with 5% sorbitol50. P. falciparum CDPK1-3HA-DD parasites were cultured in the presence of 2.5 nM WR99210 and 0.25 μM Shld-1. PfPKA-R-GFP and PfPKA-C-HA27 overexpressing parasite cultures were supplemented with 10 nM WR99210. PfCDPK1-3HA-DD parasites were generated in D10 background by transfecting plasmids for single cross-over homologous recombination. PfPKA-R-GFP overexpressing parasites were generated by transfection of 3D7 strain.
Treatment of parasites with pharmacological reagents
Typically, schizont-infected RBCs were treated with IBMX (250 μM), BAPTA-AM (40 μM), 8Br-cAMP (100 μM), PKI (20 μM) unless indicated otherwise.
Growth rate and invasion assays
For comparison of growth rate of the PfCDPK1-3HA-DD parasites in the presence or absence of Shld-1, parasites were synchronized using 5% sorbitol. The effect of Shld-1 removal on PfCDPK1-3HA-DD parasites was studied by splitting synchronized parasite cultures into two halves at ring stage. Shld-1 was withdrawn from one half and plating was done at equal parasitemia at the schizont stage. Parasite growth was quantified for 2–3 life cycles.
The parasite invasion assays were performed, as described earlier4, 30 with minor modifications. Invasion assays were performed by using schizonts from which Shld-1 was withdrawn for one cycle, as described above. Schizonts (~38–40 h.p.i) at 0.5–1% parasitemia were incubated with fresh RBCs and formation of new rings was monitored by examining Giemsa stained smears after 3–9 h and/or by performing FACS of SYBR Green stained parasites, which were fixed 30 h post invasion. FACS assay was performed using a slightly modified previous published protocol51. Briefly, ~300 µl parasite infected RBCs were washed thrice with PBS and were fixed with 4% paraformaldehyde for 30 min. After fixation, parasites were washed twice with PBS and stained with SYBR Green (1 : 5000 in PBS) for 1 h in dark. Cells were washed with PBS twice and resuspended in 800 µl of PBS and used for FACS using BD Accuri C6 Plus machine. Data were analyzed using FloJo software after excluding the autofluorescence from unstained cells by gating. To study the effect of Neuraminidase (Nm), ring infected RBCs were treated with 66 mU ml−1 Neuraminidase and 1 mg ml−1 Trypsin to prevent reinvasion, as described previously32 for 37 °C for 1 h. To study the effect of Chymotrypsin (CT), RBCs were treated with 1 mg ml−1 CT for 1 h at 37 °C, as described previously36. For performing invasion assays with PfPKA-R-GFP parasites, parasites were treated with 100 µM 8Br-cAMP 3 h prior to performing invasion assays.
Parasite attachment assay
The attachment assays were performed as described earlier30 with slight modifications. Briefly, CDPK1-3HA-DD parasites were tightly synchronized, split into 2 × 15 ml (5% parasitemia, 5 % hematocrit) and from one half Shld-1 was withdrawn. The parasites were allowed to mature to schizonts (~ 40 h) and maintained in 50 U ml–1 of heparin for additional ~ 6 h. Subsequently, parasite-infected RBCs were plated in 6-well culture plates after washing with complete RPMI1640 along with fresh RBCs and treated with 1 μM cytochalasin D or DMSO (control). The plates were incubated in Ziploc bags, equilibrated with appropriate gas mixture and kept on a shaker at 80 rpm at 37 °C30. Thin blood smears were prepared after 8–12 h, which were used for staining parasite nuclei with DAPI. The numbers of attached parasites were counted by microscopically analyzing the DAPI stained parasites.
Protein digestion and iTRAQ labeling
The work flow followed for these studies is described in Fig. 1c. The analysis was carried out on four independent biological replicates and one of the replicate was further processed and analyzed as technical duplicates. Therefore, the phosphorylation levels of proteins upon CDPK1 knockdown was studied in five independent analyses.
PfCDPK1-3HA-DD parasites were cultured in the presence or absence of Shld-1 and harvested at the late schizont stage, pellets were pooled and suspended in lysis buffer (8 M Urea, 1 mM Sodium fluoride, 1 mM sodium orthovanadate, 2.5 mM sodium pyrophosphate and 1 mM ß-glycerophosphate). Cells were lysed after multiple cycles of freeze thaw followed by sonication and centrifugation at 18,407 × g for 30 min. The supernatant was collected and protein was estimated using Bicinchoninic acid assay (Pierce, Waltham, MA, USA). An equal amount of protein (1.5 mg) from each case was reduced using DTT at a final concentration of 5 mM at 60 °C for 30 min and alkylated using 10 mM iodoacetamide for 10 min at room temperature kept in dark. Trypsin was added in a ratio of 1 unit of trypsin per 20 unit of sample and kept for overnight digestion at 37 °C. Buffer exchange was done using Sep-Pak C18 columns (Waters Corporation, Milford, MA, USA) and peptides were lyophilized. iTRAQ labeling of the peptides was carried out as per manufacturer’s instructions. Peptides from wild type parasites were labeled in technical replicates with 114 and 115 iTRAQ reporter ions and peptides from CDPK1 knockdown parasites were labeled with 116 and 117 reporter ions. Labeling of the peptides was checked and the four samples were pooled in equal amount and dried. One more biological replicate was processed in the same way, which was again analyzed as two technical replicates.
Basic RPLC and phosphopeptide enrichment
The lyophilized peptides were reconstituted in bRPLC solvent A (10 mM triethylammonium bicarbonate, pH 8.5) and fractionated on Xbridge C18 5 um 250 × 4.6 mm column (Waters Corporation, Milford, MA, USA) using Agilent 1100 binary pump (Agilent Technologies, Santa Clara, CA, USA). The sample was resolved through reverse-phase liquid chromatography method using a gradient of 5 to 60% solvent B (10 mM triethylammonium bicarbonate, pH 8.5 in 95% Acetonitrile) with 1 ml flow rate per minute for over 60 min. A total of 96 fractions were concatenated into 12 fractions and vacuum dried. One tenth of each fraction was taken out for total proteomic analysis and the rest was further processed for TiO2 based enrichment of phosphopeptides. Titansphere beads (GL Sciences, Japan) were mixed with peptides in 1:1 ratio and incubated on rotor for 1 h at room temperature. Peptides were then washed with 80% ACN in 3% TFA and eluted using 4% ammonia solution followed by neutralization with 3% TFA. Eluted peptides were then dried and desalted using C18 stage tips and then subjected to LC-MS/MS analysis.
Each fraction was reconstituted in 0.1% formic acid and analyzed on Orbitrap Fusion Tribrid mass spectrometer interfaced with Proxeon Easy-nLC 1000 system (Thermo Scientific, Bremen, Germany). The sample was first loaded onto a 2 cm long pre-column packed in-house with magic C18 AQ (MichromBioresources, Auburn, CA, USA). Peptides were resolved on an analytical column (75 µ × 15 cm, 3 µ particle and 100 Å pore size) using a linear gradient of 7 to 30% of solvent B (0.1% formic acid in 95% Acetonitrile) over 120 min. Both MS and MS/MS was acquired using Orbitrap mass analyzer and full scans were acquired with scan range of 350–1800 m/z and at a resolution of 120,000 at 200 m/z. The data were acquired in top speed mode with 3 s cycles, which would allow the instrument to continuously perform MS2 scans until the list of precursors diminish to zero or 3 s. Most intense precursor ions were selected and fragmented using higher-energy collisional dissociation (HCD) with 35% normalized collision energy. Fragment ions were detected in Orbitrap with mass resolution of 30,000 and AGC target value was set to 50,000 with maximum ion injection time of 200 ms. Singly charged ions were rejected and dynamic exclusion was set to 30 s. Internal calibration was carried out using lock mass option (m/z 445.1200025) from ambient air.
MS data analysis
The mass spectrometry derived data were searched using Mascot and Sequest search engines using Proteome Discoverer 1.4 (Thermo Fisher Scientific, Bremen, Germany). Phosphopeptides enriched fractions and total proteome data from each replicate were searched against a combined Human and P. falciparum NCBI RefSeq protein database (version 65) with carbamidomethylation of cysteine residues, peptide N-terminal and lysine side chain of iTRAQ as fixed modification. Oxidation of methionine and phosphorylation of serine, threonine and tyrosine was selected as dynamic modifications. Trypsin was set as the protease and maximum of one missed cleavage was allowed. Precursor mass tolerance was set to 20 ppm and fragment mass tolerance of 0.1 Da was allowed. All PSMs were identified at 1% FDR. Posterior error probability was calculated for individual PSM using percolator, providing statistical confidence for each spectral match. If a given spectrum was assigned to different peptides by Mascot and Sequest, they were discarded and not considered for further analysis. The probability of phosphorylation for each site was calculated by the phosphoRS node in Proteome Discoverer. Only the phosphopeptides with >75% site localization were considered for further analysis. Phosphorylation fold change for each peptide was normalized with the total proteome level change and a normalized phosphorylation change of >0.75 fold was considered as significantly regulated.
Gene ontology analysis
The gene ontologies for Plasmodium falciparum proteins were downloaded from PlasmoDB database52. Hypophosphorylated proteins that lacked appropriate GO annotation were assigned with relevant GO terminologies based on manual curation of the available literature. We merged our manually curated information with the available ontologies and carried out GO enrichment analysis on the list of hypophosphorylated proteins using FunRich tool53. The list of proteins identified in our analysis was selected as background and the hypophosphorylated proteins were provided as input. The fold- enrichment and P values associated with biological processes, molecular functions and cellular localizations are provided in Supplementary Data 2.
The list of hypophosphorylated sites with a width of 15 amino acids was subjected to motif analysis using motif-X tool54. A background of P. falciparum protein database was used for the analysis and occurrences threshold was set to default i.e. 20. A P value threshold of ≤ 1e-6 was used to identify enriched motifs.
Protein-protein interaction networks prediction
The list of differentially phosphorylated proteins upon CDPK1 knockdown was submitted to STRING database (version 10.0) for protein–protein interaction analysis. Interactions with high confidence and score of >0.7 were considered as significant and considered for the study.
Expression of recombinant proteins
For expression of PfPKA-C (PlasmoDB ID PF3D7_0934800), PfPKA-R (PlasmoDB ID PF3D7_1223100) and their mutants as GST fusion proteins, their ORFs were cloned in pGEX4T1 vector (GE Healthcare) using PCR primers PfPKA-R_F and PfPKA-R_R (PfPKA-R) and PfPKA-C_F and PfPKA-C_R (PfPKA-C). Primer sequences are provided in Supplementary Table 1. PfCDPK1 (PlasmoDB ID PF3D7_0217500) expression has been described previously7. For expression of PfIMC1g (PlasmoDB ID PF3D7_0525800), its ORF was cloned in pET28a (Novagen) vector using PCR primers PfIMC1g_F and PfIMC1g_R respectively. These and other 6xHis-tagged or GST-fusion recombinant proteins described in the manuscript were expressed and purified by using standard procedures using Ni-NTA or GSH-sepharose affinity matrices, respectively. Expression and purification of 6xHis-PfGAP45 has been described previously15. Protein concentration was determined by densitometry analysis of coomassie stained gels using NIH Image J software.
Generation of antisera
Antisera was raised against PfPKA-C and PfPKA-R using KLH-conjugated synthetic peptides designed from their C-terminus following standard procedures in rabbits (2–3 months old, New Zealand) and mice (Balb/c, 4–6 week old) (Supplementary Fig. 6). PfPKA-C: H-(KLH) cys-VPYKPKYKNIFDSSNFE-OH; PfPKA-R: H-(KLH) cys-CDILHRNVENYKKVLNE-OH. Antisera against PfIMC1g was raised in mice using full length 6xHis PfIMC1g recombinant protein, which was expressed using standard procedures.
Antibody against PfPKA-R phosphorylated at S149 was custom generated by Antagene. Inc. (USA). For this purpose, a synthetic peptide with sequence
Cys- HFIQKKRL(p)SVSAEAYGDWNK or a control without phosphoserine was used. Cysteine at the N-terminus was added for KLH-conjugation. The phosphorylated and non-phosphorylated peptides were used to immunize rabbits over a 12-week schedule. Antisera were collected after 10 days of fourth immunization and antibody titers were determined by performing ELISA against the phosphorylated and the non-phosphorylated peptides. The antisera were enriched following a two-step phospho-peptide antibody purification method.
Protein kinase assays were performed using recombinant 6xHis-PfCDPK1 in a reaction buffer containing 50 mM Tris pH 7.4, 10 mM Magnesium Chloride, 1 mM Dithiothreitol, 100 µM CaCl2 and 100 μM γ32-P[ATP] 15μCi/reaction using recombinant substrates like PfGAP45, PfPKA-R, IMC1g. Reactions were carried out at 30 °C for 45 min and stopped by boiling them in SDS-PAGE loading buffer. The reaction mixture was electrophoresed on SDS-PAGE and phosphorylation of proteins was detected by phosphorimaging using a Fujifilm FLA-5000 scanner. For assaying activity of PfCDPK1 and PfPKA in the parasite, anti-PfCDPK1 or PfPKA-C antisera was used for immunoprecipitation and PfCDPK1-IP or PfPKA-IP was used for kinase assays as described above. For assaying PfPKA-C activity, a parasite line overexpresssing PfPKA-C-HA was used by immunoprecipitating using anti-HA antibody. The IP was subsequently used for kinase assays.
Metabolic labeling of parasites
PfCDPK1-3HA-DD parasites were synchronized twice at the ring stage. Parasites were split in two halves after washing with complete RPMI 1640 media and Shld-1 was withdrawn from one of them. ~40 h post-invasion, parasites were washed twice with phosphate deficient RPMI 1640 medium (Hyclone) supplemented with 0.5% albumax (Gibco, Life Tech). These parasites were incubated with 32P orthophosphoric acid (1–2 mCi ml–1) till segmenters were formed. Parasite lysate was prepared in complete lysis buffer described below and immunoprecipitation was done using specific antibodies. The immunoprecipitate was electrophoresed on SDS-PAGE and labeled proteins were detected by phosphorimaging using a Fujifilm FLA-5000 scanner.
Immunoblotting and immunoprecipitation
After various treatments with various pharmacological inhibitors, parasites were harvested by 0.05% saponin lysis at 4 °C for 30 min and were washed thrice with ice cold PBS and resuspended in complete lysis buffer containing 10 mM Tris pH 7.4, 100 mM sodium chloride, 5 mM ethylenediaminetetraacetic acid, 1% Triton X-100, 100 μM sodium orthovanadate, 20 μM β glycerophosphate, 1× protease inhibitor cocktail and 10% glycerol. Cell-free protein extracts were prepared from these parasites by syringe lysis and clearing by centrifugation at 15,871 × g at 4 °C for 30 min. After separation on 10% SDS-PAGE, lysate proteins were transferred to a nitrocellulose membrane. Immunoblotting was performed using specific antisera and blots were developed using SuperSignal West Pico, or Dura Chemiluminescence Substrate (Thermo Scientific) following manufacturer’s instructions.
For immunoprecipitation, 60–100 µg of lysate protein was typically used and incubated with relevant antibodies at 4 °C for 12 h followed by incubation with protein A+G plus agarose beads for 5 h. The beads were washed with cold complete lysis buffer and resuspended in 50 µl 1× kinase assay buffer for kinase assay and in 50 µl 1× SDS-PAGE loading buffer for western blotting. Immunoblots were cropped for presentation in main figures and full-sized images of some of the blots are presented in Supplementary Fig. 7.
Detection of secreted proteins
PfCDPK1-3HA-DD parasites were synchronized and Shld-1 was withdrawn at the ring stage for 1–2 cycles, as described above. Fresh media was added to schizont/segmenters, which were allowed to burst to release merozoites. Subsequently, the culture was centrifuged at 500×g for 5 min to separate the free merozoites from the infected and uninfected RBCs. The culture supernatant containing merozoites was further centrifuged at 3300×g for 5 min to separate merozoite and secreted proteins released in the supernatant.
The animal experiments, which involved antisera generation, were performed at National Institute of Immunology, New Delhi with the approval of the Institute Animal Ethics Committee (IAEC) and prescribed guidelines were followed.
Densitometry and statistical analysis
Image J (NIH) software was used to perform densitometry of western blots. The band intensity of the loading control was used for normalization. Statistical analysis was performed using Prism (Graph Pad software Inc USA). Data are represented as mean±Standard Error of Mean (s.e.m.) from three independent experiments, unless indicated otherwise and p<0.05 was taken as statistically significant.
The mass spectrometry-based proteomics data have been deposited to the ProteomeXchange Consortium (http://proteomecentral.proteomexchange.org) and can be accessed via the PRIDE partner repository with the data set identifier PXD005207.
All other relevant data are available from the authors upon request.
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We thank Divya Thomas and Gourav Dey for assistance with some of the experiments. Studies were supported by grants BT/COE/34/SP15138/2015 and BT/PR7976/BRB/10/1223/2013 from Department of Biotechnology, India and funds from NII core. S.K is a recipient of Junior Research Fellowship from the Council of Scientific and Industrial Research (CSIR), India. P.S is a J.C. Bose fellow.