Despite global efforts to combat malaria, the disease caused an estimated 247 million new cases and more than 619,000 deaths in 2021 (World Malaria Report 2022). The etiological agents of human malaria are apicomplexan parasites of the genus Plasmodium. Among the six known Plasmodium species that can infect humans, Plasmodium falciparum is the most lethal, causing the majority of annual deaths if left untreated (Cowman et al. 2012). The intraerythrocytic developmental cycle (IDC) of P. falciparum is responsible for the clinical symptoms of malaria. The IDC commences when liver-stage merozoites enter the circulatory system and invade red blood cells (RBCs). While growing inside RBCs, parasites undergo multiple developmental phases with distinct morphological characteristics (ring, trophozoite, and schizont). Maturation and schizogony leads to the formation of 16-32 daughter merozoites destined to invade new RBCs (Singh et al. 2010). A small fraction (<10%) of parasites differentiate into non-replicative sexual gametocytes, which are transmitted to the mosquito during a second blood meal to complete sexual development.

Parasite development through the asexual blood stage is facilitated by precise transcriptional regulation, where genes are only expressed when needed in a just-in-time fashion (Bozdech et al. 2003). Approximately 90% of genes across the P. falciparum genome are transcribed during the asexual blood stage in a cascade of gene expression believed to be controlled by both sequence-specific transcription factors and dynamic epigenetic changes to chromatin (Painter et al. 2011, Toenhake et al. 2018, Jeninga et al. 2019, Hollin et al. 2021). The typical gene regulatory toolbox in malaria parasites is lacking many transcriptional regulatory factors conserved in other eukaryotes (Gardner et al. 2002). The identification of Plasmodium homologues of the plant APETALA2/Ethylene Response Factor (AP2/ERF) transcription factors (TFs) provided a breakthrough to unravel key regulators of gene expression in these parasites (Balaji et al. 2005). There are 28 putative APETALA2 (ApiAP2) TFs identified in P. falciparum, each protein containing one to three AP2 DNA binding domains (Painter et al. 2011, Jeninga et al. 2019). Multiple studies in Plasmodium spp., using a variety of approaches, have characterized essential functions of ApiAP2 TFs in RBC invasion, gametocytogenesis, oocyst formation and sporozoite formation (Yuda et al. 2009, Kafsack et al. 2014, Sinha et al. 2014, Modrzynska et al. 2017, Santos et al. 2017, Zhang et al. 2018). ApiAP2 proteins in Plasmodium species display a wide array of functions during parasite development in both the vertebrate host and the mosquito vector, but surprisingly, approximately 70% of ApiAP2 proteins are expressed in the asexual blood stage of the lifecycle (Bozdech et al. 2003, Le Roch et al. 2003).

Despite increasing evidence detailing ApiAP2 protein regulatory complexes (Santos et al. 2017, Harris et al. 2019, Hillier et al. 2019, Hoeijmakers et al. 2019, Farhat et al. 2020, Josling et al. 2020, Miao et al. 2021, Antunes et al. 2023, Srivastava et al. 2023, Yuda et al. 2023), the functional properties and specific interaction partners of many ApiAP2 TFs remain to be elucidated. A quantitative mass spectrometry-based analysis of the parasite protein interaction network has revealed links between ApiAP2 TFs and many chromatin remodelers, such as an extended Egl-27 and MTA1 homology 2 (EELM2) domain-containing proteins (PF3D7_0519800 and PF3D7_1141800), histone deacetylase protein 1 (HDAC1; PF3D7_0925700), and the microrchidia family protein PfMORC (PF3D7_1468100) (Hillier et al. 2019). Genome-wide mutagenesis studies revealed that several genes within these proposed networks, including pfmorc, are essential for parasite proliferation (Bushell et al. 2017, Zhang et al. 2018). Using a targeted deletion strategy, we previously were unable to delete pfmorc, further suggesting that it is essential for parasite growth (Singh et al. 2021). Moreover, STRING network analysis has shown that the putative ApiAP2:PfMORC complex forms a network with proteins having DNA-binding or nucleosome assembly properties, suggesting that PfMORC may function as an accessory protein in epigenetic regulation (Hillier et al. 2019). Previous work identified PfMORC in a chromatin complex containing the chromatin remodeling protein PfISWI (PF3D7_0624600) located at var gene promoter regions (Bryant et al. 2020). Bryant et al. proposed that PfMORC is recruited to these regions to help repress silenced var genes on the basis of its known function as a repressor complex component in model eukaryotes. In the related apicomplexan parasite Toxoplasma gondii, TgMORC functions as a repressor of sex-associated genes by recruiting the histone deacetylase protein TgHDAC3 and forming heterogenous complexes with eleven ApiAP2 TFs (Farhat et al. 2020). To date, only two TgMORC:HDAC3 complexes have been characterized, including a TgAP2XII-2:HDAC3 complex and a heterotrimeric TgAP2XII-1:AP2XI-2:HDAC3 complex (Antunes et al. 2023, Srivastava et al. 2023).

MORC proteins canonically consist of two major conserved regions: (1) a catalytic ATPase domain at the N-terminus (contains a GHKL [Gyrase, HSP90, Histidine kinase, and MutL] domain and S5 fold domain) and (2) a C-terminal protein-protein interaction domain with one or more coiled-coils (Koch et al. 2017). The MORC family of proteins is highly conserved in all eukaryotic cells, with the exception of fungi, often with multiple paralogs per genome (Dong et al. 2018), and has been extensively investigated in model various systems in the context of epigenetic gene regulation. For example, in plants MORC family proteins function in gene repression and heterochromatin compaction (Koch et al. 2017, Zhong et al. 2023). Additionally, MORC family proteins have been shown to play diverse roles by forming protein-protein interactions with immune-responsive proteins, SWI chromatin remodeling complexes, histone deacetylases, and histone tail modifications across metazoans (Iyer et al. 2008, Kang et al. 2012, Moissiard et al. 2012, Bordiya et al. 2016, Kim et al. 2019).

While most metazoans possess five to seven MORC paralogs, apicomplexan parasites contain a single morc gene (Iyer et al. 2008), which encodes not only the canonical animal-like GHKL ATPase domain, but also three Kelch-repeats, and a CW-type zinc-finger domain not found in mammalian MORCs (Farhat et al. 2020). This unique domain architecture suggests that the Apicomplexan MORC proteins may have parasite-specific roles. To dissect the functional roles of PfMORC, we conducted a proteomic analysis with PfMORCGFP which identified several nuclear proteins, including a cluster of ApiAP2 TFs, as possible interacting partners. We also determined the genome-wide localization of PfMORC at multiple developmental stages, which revealed PfMORC recruitment predominantly to subtelomeric regions, corroborating that PfMORC may act as a repressor of clonally variant gene families. Finally, we performed transcriptomic analysis in PfMORCHA-glmS knockdown parasites at the asexual stage to investigate alterations in global gene expression. Our results indicate an overrepresentation of downregulated genes belonging to the heterochromatin-associated hypervariable gene family proteins. Overall, this study allows us to understand the plasticity in epigenetic regulation via PfMORC during asexual blood stage development.


Enriched proteins represent gene regulatory and chromatin remodeling components

A previous study using Blue-Native PAGE identified a PfMORC complex in association with other ApiAP2 proteins and chromatin remodeling machinery (Hillier et al. 2019). To validate the interacting partners of PfMORC, we used a targeted immunoprecipitation approach coupled to LC‒MS/MS proteomic quantification. We used a previously generated PfMORCGFP parasite line (Singh et al. 2021) to carry out immunoprecipitation with an anti-GFP antibody at the trophozoite stage, where PfMORC is abundant (Singh et al. 2021). The P. falciparum 3D7 strain expressing wild-type pfmorc was used as a negative control. Trophozoite lysates were incubated with anti-GFP-Trap-A beads (ChromoTek, gta-20), and the immunocaptured proteins were resolved by SDS‒PAGE (Supplemental Figure 1A). We applied a label-free quantitative proteomics approach with a false discovery rate (FDR) of 1% and number of peptides ≥2 to excised gel samples to identify proteins interacting with PfMORCGFP. From three replicates, we identified 211, 617, and 656 proteins respectively (Figure 1B, Supplemental Table 1). We further identified the overlap between all three wild-type 3D7 and PfMORCGFP replicates and found a total of 132 and 142 proteins, respectively (Supplemental Figure 1C).

– Proteomic analysis of parasites expressing PfMORCGFP reveals PfMORC association with nuclear proteins of epigenetic regulation.

(A) Venn diagram depicting protein enrichment from three biological replicates using PfMORC as bait from 32 hpi (±4 h) trophozoite stage PfMORCGFP parasite lysate with anti-GFP-Trap-A beads. (B) Venn diagram was created for CoIPed protein in PfMORCGFP with selected proteins from recently published work by Hillier et al, Bryant et al. and Subudhi et al. Intersecting proteins showing the majority of proteins are AP2 and chromatin remodellers. (C) Protein-protein interaction network of enriched proteins co-IPed with anti-GFP and detected by mass spectrometry was generated with known PfMORC interactome from published work. The String database and Cytoscape were used to create an interactive protein-protein interaction network.

To analyze the relative ratio of proteins between wild-type 3D7 and PfMORCGFP groups, we used the mean normalized MS/MS count to calculate a fold change and selected differentially abundant proteins above a 1.5x cutoff filter. This resulted in 143 significantly enriched proteins (Supplemental Table 2). From these candidate PfMORC-interacting proteins, the top enriched protein (20.8-fold enrichment) was PfEELM2 (PF3D7_0519800). PfEELM2 was previously predicted as a PfMORC interactor (Hillier et al. 2019) and identified in a quantitative histone peptide pulldown to be consistently recruited to H2B.Z_K13/14/18a (Hoeijmakers et al. 2019). Furthermore, we also detected numerous ApiAP2 transcription factors [PfAP2-G5, PfAP2-O5, PfAP2-I, PF3D7_1107800, PF3D7_0613800, PF3D7_0420300 and PF3D7_1239200] (Table 1), similar to results reported both by Hillier et al. and with Toxoplasma TgMORC complex (Farhat et al. 2020, Antunes et al. 2023, Srivastava et al. 2023).PfAP2-G5 (PF3D7_1139300) and PfAP2-O5 (PF3D7_1449500) were enriched 20.5- and 14.99-fold, respectively, suggesting that these factors are likely major components in-complex with PfMORC. To corroborate our results, we compared our PfMORCGFP coIPed proteins to a recently published protein‒protein network (Hillier et al. 2019, Bryant et al. 2020, Subudhi et al. 2023) and found many of the same ApiAP2 and EELM2 proteins across both datasets (Figure 1B). Collectively, our results demonstrate a direct association of PfMORC with various chromatin-associated factors, including many ApiAP2 proteins.

– Potential PfMORC interacting proteins enriched in CoIP eluates and identified in LC‒ MS/MS from three independent experiments and fold change ≥ 1.5x GFP/3D7.

We also identified proteins implicated in DNA replication and repair, including the ATP-dependent RNA helicase DBP5 (PF3D7_1459000) and the DNA helicase 60 DH60 (PF3D7_1227100) associated with PfMORC. PfDH60 exhibits DNA and RNA unwinding activities, and its high expression in the trophozoites suggest a role in DNA replication (Pradhan et al. 2005). We also identified two putative chromatin-associated proteins, chromodomain-helicase-DNA-binding protein 1 CHD1 (PF3D7_1023900) and the SNF2 chromatin-remodeling ATPase ISWI (PF3D7_0624600), which are associated with chromosome structure maintenance, DNA replication, DNA repair, and transcription regulation. PfISWI was previously reported to be associated with PfMORC in the context of transcriptional activation of var genes during ring stage development (Bryant et al. 2020). Gene Ontology (GO) analysis was performed to identify enriched biological processes, cellular components, and molecular functions using a p-value cut-off of 0.05. We found significant enrichment of DNA-binding transcription factor activity and mRNA binding, transcription and regulation of transcription activity (Supplemental Figure 1D, Supplemental Table 3). Overall, we again find that PfMORC forms a link between ApiAP2 TFs and chromatin remodelers (Figure 1C).

PfMORC localizes to multigene families in subtelomeric regions

To determine the genome-wide occupancy of the PfMORC chromatin-associated remodeling complex, we used chromatin immunoprecipitation followed by high-throughput sequencing (ChIP-seq). Using purified, crosslinked nuclear extracts, we immunoprecipitated PfMORC from a 3xHA-tagged PfMORCHA-glmS parasite line (Singh et al. 2021) for ChIP-seq at the trophozoite stage (30hpi) and the schizont stage (40hpi) in biological duplicates. These timepoints represent the stages at which PfMORC is most highly expressed (Singh et al. 2021). An independent ChIP-seq experiment in biological duplicate using anti-GFP and a PfMORCGFP parasite line (Singh et al. 2021) at the schizont stage was used to confirm our findings, demonstrating that the protein tags do not affect PfMORC immunoprecipitation or genome-wide localization (Supplemental Figure 2A,B). As an additional control, we correlated one no-epitope, negative control sample using the same anti-HA antibody on unmodified parasite lines for immunoprecipitation (Supplemental Figure 2A,B; (Bonnell et al. 2023)), which resulted in an expected low correlation to the tagged samples. The biological ChIP-seq replicates showed high fold enrichment (Log2[IP/Input]) (Supplemental Figure 2C) and were highly correlated within each timepoint (Supplemental Figure 2D-F).

We identified PfMORC localized to subtelomeric regions on all chromosomes across the P. falciparum genome with additional occupancy at internal heterochromatic islands (Figure 2A,B). Within the subtelomeric regions, PfMORC was bound upstream and within the gene bodies of many hypervariable multigene families (Figure 2C), including the var genes (Supplemental Figure 3), rif genes (Supplemental Figure 4), and stevor genes (Supplemental Figure 5). Predicted binding sites (across both biological replicates) between the 30hpi and 40hpi timepoints showed a high degree of overlap, suggesting that PfMORC binds many of the same regions throughout the later stages of asexual development when PfMORC is highly expressed (Figure 2D). The proportion of PfMORC-bound regions was similar across the 5′ upstream region of genes and the gene bodies throughout the genome, including subtelomeric regions (Figure 2E). As opposed to the binding of other proteins at the subtelomeric regions of P. falciparum, such as the heterochromatin protein 1 (PfHP1), PfMORC occupancy is not widespread (Flueck et al. 2010). Instead, PfMORC forms sharp peaks within and adjacent to HP1-bound regions (Figure 2F), suggesting a unique role for PfMORC in heterochromatin condensation, boundary demarcation, and gene repression.

Genome-wide occupancy of PfMORC reveals localization to hypervariable surface antigen genes at 30 h and 40 h.

(A) Coverage tracks of PfMORC across all 14 P. falciparum chromosomes. Plotted values are fold enrichment (Log2[IP/Input]) of a representative replicate at 30 h. (B) Zoom-in of the last 100kb region of chromosome two from Panel A. Gene annotations represented in blue bars (P. falciparum 3D7 strain, version 3, release 57; (C) Mean fold enrichment of PfMORC occupancy across all var genes (top left), all rif genes (top right), and all stevor genes (bottom right), excluding pseudogenes. Graphical representation of exons to scale for each gene family annotated below enrichment plot in grey (e1=exon one; e2=exon two). (D) Quantitative Venn diagram comparing the number of MACS2 called peaks across each timepoint (light pink for 30 h; dark pink for 40 h). (E) Pie charts showing the type of genomic locations PfMORC peaks overlap at both 30 h and 40 h. Pink slices are 5’ regions upstream of the ATG start site of genes, blue slices are coding sequences/gene bodies of genes, and green slices are 3’ regions downstream of the stop codon of genes. (F) Zoom-in of the first 100kb region (left) and the last 100kb region (right) of chromosome two. Plotted are the ChIP-seq fold enrichment of PfMORC (top track; pink) and heterochromatin protein 1 (HP1; middle track; orange) with gene annotations (bottom track; blue bars; P. falciparum 3D7 strain, version 3, release 57;

We further defined PfMORC putative gene targets as genes displaying peaks within 2-kb upstream of the ATG start codon or within gene bodies. For those peaks between gene targets in a head-to-head orientation, the closest gene was chosen. This resulted in 149 putative gene targets at 30hpi and 102 gene targets at 40hpi. A close examination of the 84 overlapping genes shows that many are var, rRNA, and exported proteins (Supplemental Table 4), with GO terms related to cell adhesion, host‒pathogen interactions, and antigenic variation (Supplemental Table 5). The 65 uniquely bound genes at the 30hpi timepoint showed an enrichment of highly expressed tRNA genes, rRNAs, and conserved unknown genes, while those 18 unique to the 40hpi timepoint included a variety of late-stage expressed genes. Transcript abundance (Chappell et al. 2020) of the predicted PfMORC gene targets at both the 30hpi and 40hpi timepoints form two major clusters: cluster one being genes expressed at the late ring/early trophozoite stage (10-24hpi) and cluster two at the late schizont stage (40-48hpi) (Supplemental Figure 6). This two-cluster gene target pattern of expression mirrors the biphasic pattern of expression by PfMORC, suggesting that PfMORC could have distinct functions, forming complexes with different sets of transcriptional regulators, at various times during asexual proliferation. As determined in other eukaryotic organisms, MORC family proteins do not generally bind DNA in a sequence-specific manner; it is, therefore likely that PfMORC is recruited to these genome-wide regions by sequence-specific transcription factors, such as the ApiAP2 proteins identified in our proteomics results.

Binding sites of PfMORC overlap with ApiAP2 proteins and epigenetic marks

PfMORC has previously been found to interact with several ApiAP2 proteins (Hillier et al. 2019, Bryant et al. 2020, Singh et al. 2021), as does the Toxoplasma orthologue (Farhat et al. 2020, Antunes et al. 2023, Srivastava et al. 2023). We identified the overlap between genome-wide PfMORC binding and putatively interacting ApiAP2 proteins using available ChIP-seq datasets. In addition to our protein-protein interaction results (Table 1), previous studies have also suggested that PfMORC interacts with a broad array of ApiAP2 TFs, such as PfAP2-G5, PfAP2-O5, PfAP2-I, PF3D7_1107800, PF3D7_0613800, PF3D7_0420300, and PF3D7_1239200 (Hillier et al. 2019, Bryant et al. 2020, Subudhi et al. 2023). Therefore, we compared binding sites between interacting ApiAP2s and PfMORC using available ChIP-seq data on PfAP2-G5, PfAP2-O5, PfAP2-I, PF3D7_1107800, PF3D7_0613800, PF3D7_1239200 (Josling et al. 2020, Shang et al. 2021, Shang et al. 2022). Interestingly, there is a degree of overlap between the binding sites of all six ApiAP2 TFs and PfMORC, suggesting that PfMORC and these ApiAP2 TFs may cooperate in the regulation of gene expression at these loci (Figure 3A-B; Supplemental Figure 7). However, the available data cannot differentiate whether all of these factors are in one complex together, multiple smaller heterologous complexes, or are components of separate complexes in individual cells. DNA motif enrichment analysis (Bailey 2021) identified several unique and significant DNA motifs at both the 30hpi and 40hpi timepoints, which suggests that more than one sequence-specific transcription factor may be responsible for recruiting PfMORC to specific genomic regions (Supplemental Figure 8). The common motifs identified across replicates and timepoints are RGTGCAW or TGCACACA, which are similar to the in vitro and/or in vivo DNA-binding motif of PfAP2-I (RGTGCAW) or PF3D7_0420300 (TGCACACA), suggesting that these ApiAP2 factors may play major roles in PfMORC recruitment (Supplemental Figure 8).

(A) Mean fold enrichment (Log2[IP/Input]) of PfMORC, six associated factors (AP2-G5, AP2-O5, AP2-I, PF3D7_1107800, PF3D7_0613800, and PF3D7_1239200), HP1, and a negative no-epitope control across PfMORC binding sites at the 30 h timepoint. (B) Mean fold enrichment (Log2[IP/Input]) of PfMORC, six associated factors (AP2-G5, AP2-O5, AP2-I, PF3D7_1107800, PF3D7_0613800, and PF3D7_1239200), HP1, and a negative no-epitope control across PfMORC binding sites at the 40 h timepoint. (C) Mean fold enrichment (Log2[IP/Input]) and heatmap of two H3K36me2 epigenetic mark timepoints across PfMORC binding sites at 30 h. (D) Mean fold enrichment (Log2[IP/Input]) and heatmap of two H3K36me2 epigenetic mark timepoints across PfMORC binding sites at 40 h.

In addition to overlapping occupancy with ApiAP2 TFs, we found that PfMORC co-localizes with the depletion of H3K36me2 (Figure 3C, D), which is demarcated by the SET2 methyltransferase (Jiang et al. 2013), both at 30hpi and 40hpi. No other significant co-localization was found between PfMORC and other epigenetic marks (H2A.Z, H3K9ac, H3K4me3, H3K27ac, H3K18ac, H3K9me3, H3K36me2/3, H4K20me3, and H3K4me1) (Supplemental Figure 9). Therefore, it is likely that PfMORC co-localizes with other, as of yet uncharacterized, epigenetic marks. In summary, PfMORC was found to be recruited to 5’-untranslated regions (UTRs), gene body regions, and subtelomeric regions of repressed, multigene families, and overlaps with other known ApiAP2 binding sites and DNA motifs.

Depletion of PfMORC results in upregulation of late-stage genes associated with invasion

PfMORC association with chromatin remodelers has been shown (Bryant et al. 2020), but how PfMORC regulates gene expression in the asexual stage has not been evaluated. In T. gondii, the TgMORC:TgApiAP2 complex acts as a transcriptional repressor of sexual commitment (Farhat et al. 2020, Antunes et al. 2023, Srivastava et al. 2023). This study found that PfMORC co-immunoprecipitates with several chromatin remodeling proteins and many ApiAP2 transcription factors. Furthermore, our ChIP-seq data revealed that PfMORC is located at subtelomeric regions of the genome. Based on this evidence, we hypothesized that PfMORC may regulate transcriptional changes during blood stage development of the parasite. To knock down the expression of PfMORC (PfMORC-KD), sorbitol-synchronized MORCHA-glmS parasites (22-24hpi) were subjected to 2.5 mM glucosamine (GlcN) treatment for little over 48 hours when they reached the trophozoite stage (32hpi ± 3hpi), at which point parasites were harvested for RNA isolation for transcriptomic analysis. In parallel, another flask with PfMORCHA-glmS parasites was set up without GlcN and used as control for RNA-seq comparison. We previously demonstrated that treatment with 2.5 mM GlcN results in a 50% knockdown of PfMORC protein but does not cause any growth delay, however using >2.5 mM GlcN caused a measurable slow growth and reduced parasitemia (Singh et al. 2021). Three biological replicates with and without GlcN were collected for knockdown transcriptomics to ensure reproducibility.

For each PfMORC RNA-seq sample, gene counts were ued to identify the differentially expressed genes (DEGs). Significant threshold parameters were assigned to a p value <0.05, yielding a total of 2558 DEGs (Supplemental Table 6). Applying a log2-fold change cut-off from >1 to <-1 and filtering out pseudogenes reduced this number to 163 DEGs. Among these, 60 genes display more abundant transcripts, whereas 103 genes were reduced relative to control parasites grown without GlcN (Figure 4A). Pathway and functional enrichment analysis yielded several genes from apical organelles. GO analysis enriched with molecular function (p-adj = 0.0006) which has gene clusters involved in the movement into the host environment and entry into the host, and molecular function of protein binding (p-adj = 0.009) (Figure 4B, Supplemental Table 7). More specifically, upregulated genes implicated in the invasion of merozoites were found to be expressed prematurely; these include several rhoptry-associated genes, notably PfRON2 (PF3D7_1452000) and PfRON3 (PF3D7_1252100). Both PfRON2 and PfRON3 are part of a micronemal complex at the erythrocyte membrane where PfRON2 anchors PfAMA1 to facilitate merozoite invasion (Srinivasan et al. 2013). In addition, PfSUB3 (PF3D7_0507200), PfSERA5 (PF3D7_0207600) and PfDPAP3 (PF3D7_0404700), all of which are critical for schizont rupture (Yeoh et al. 2007, Arastu-Kapur et al. 2008), were among the upregulated DEGs (Figure 4C). In general, we found that depletion of PfMORC leads to upregulation of invasion-related genes, which suggests that PfMORC has an additional function in the regulation of genes specifically associated with red blood cell invasion.

– Transcriptome analysis of PfMORC knockdown revealed differential gene expression.

(A) Volcano plot showing the differential gene expression in PfMORC-KD compared to the PfMORC-WT phenotype. Tightly synchronized parasites were treated with 2.5 mM GlcN to obtain the PfMORC knockdown phenotype and another without GlcN treatment. Total RNA was collected from three biological replicates, and RNA-seq was performed. Significant threshold parameters for DEGs were assigned to a p value < 0.05. (B) Up and downregulated DEGs were further functionally categorized using KEGG database. (C) The violin plot of log2FoldChange of genes belonging to the multigene family is constructed from PfMORC-KD vs PfMORC-WT shows DEGs of multigene family proteins upon PfMORC knockdown. (D) The bar plot shows upregulated DEGs of apical organelle origin in PfMORC-KD parasites that are involved in host cell invasion. (E) Venn diagram showing the comparison between genes obtained from ChIP-seq data and DEGs obtained from RNA-seq data. Both 30hpi and 40 hpi time points were taken for comparison and showed high overlap with each other but there was no overlap with RNA-seq data.

PfMORC-depleted parasites downregulate hypervariable gene families

Among the genes with reduced mRNA abundance, DEGs linked to cytoadherence, antigenic variation and interaction with host (Figure 4B and D) where over-represented in the GO analysis. Many of the genes enriched in the downregulated group belong to the clonally variant var multigene family that represents 60 members encoding the P. falciparum erythrocyte membrane proteins (PfEMP1), which upon switching expression, aid in pathogenesis and immune evasion (Guizetti and Scherf 2013). Furthermore, a cluster of genes encoding putative exported proteins were also enriched including members of the exported protein family (EPFs), Plasmodium exported protein (hyp), and Plasmodium exported protein (PHISTa/b). Other significantly overrepresented downregulated genes belonged to serine/threonine protein kinases, the FIKK family (Ward et al. 2004) and Maurer’s clefts two transmembrane proteins (Pfmc-2TM) (Figure 4 D). Notably, expressed proteins are conserved across the Plasmodium family and remain confined to the hypervariable subtelomeric region of P. falciparum chromosomes (Sargeant et al. 2006).

Comparison of ChIP-seq gene targets and DEGs by RNA-seq

To identify whether genes found to be dysregulated after PfMORC knockdown are associated with the genome-wide occupancy of PfMORC, we correlated the gene targets identified by ChIP-seq with the DEGs determined by RNA-seq. We identified a total of 135 gene targets from the 30hpi ChIP-seq timepoint, 72 gene targets from the 40hpi ChIP-seq timepoint, and 163 DEGs by RNA-seq. The low correlation between the ChIP-seq gene targets and the RNA-seq DEGs suggest that PfMORC genome-wide occupancy is more likely involved in chromatin structure, rather than specific regulation of gene targets (Figure 4E). Likely, PfMORC localizes to these sites to aid in chromatin condensation, as shown in other eukaryotic systems (Zhang et al. 2019, Zhong et al. 2023).


Periodic gene expression during the asexual blood stage directly corresponds to the timing in which gene products are needed (Bozdech et al. 2003) and shows oscillation patterns associated with circadian rhythms (Smith et al. 2020, Subudhi et al. 2020). Transcription factors are critical regulators of this dynamic pattern in concert with epigenetic regulators and genome-wide changes to chromatin structure (Painter et al. 2011, Toenhake et al. 2018, Jeninga et al. 2019, Hollin et al. 2021). The ApiAP2 family members undergo unique binding preferences in the genome (Campbell et al. 2010), display stage-specific expression (Painter et al. 2011), and have been identified to regulate virtually all stages of development across multiple Plasmodium species (Jeninga et al. 2019). To date, ApiAP2 proteins have been reported in the transcriptional silencing of clonally variant genes, regulation of invasion genes, and sexual commitment by interaction with other epigenetic factors, such as heterochromatin protein 1 [PfHP1 (Flueck et al. 2010, Brancucci et al. 2014, Fraschka et al. 2018)], bromodomain protein 1 [PfBDP1 (Santos et al. 2017, Josling et al. 2020, Quinn et al. 2022)], or general control non-depressible 5 [PfGCN5 (Miao et al. 2021)]. Despite the known DNA-binding sites of many ApiAP2 proteins (Flueck et al. 2010, Santos et al. 2017, Sierra-Miranda et al. 2017, Josling et al. 2020, Carrington et al. 2021, Shang et al. 2021, Singh et al. 2021, Russell et al. 2022, Shang et al. 2022, Bonnell et al. 2023), limited information is available for other accessory proteins. Recently, TgMORC was identified in a complex with HDAC1, AP2XII-2, and AP2XII-1:AP2XI-2 in T. gondii and orchestrates epigenetic rewiring of sexual gene transcription (Farhat et al. 2020, Antunes et al. 2023, Srivastava et al. 2023). In P. falciparum, PfMORC has been copurified with several ApiAP2 proteins, as shown by different independent studies (Hillier et al. 2019, Bryant et al. 2020, Singh et al. 2021).

In this study, we used an integrated multi-omics approach to explore the function of PfMORC during asexual blood stage development. We identified a number of nuclear proteins that interact with PfMORC using immunoaffinity-based purification. More specifically, PfMORC was associated with PfAP2-G5, which is essential for gametocytogenesis (Shang et al. 2021), PfAP2-I, which is required for the expression of many invasion-related genes (Santos et al. 2017), and with other ApiAP2 TFs of unknown function during the asexual blood stage of development (PfAP2-O5, PF3D7_1107800, PF3D7_0613800, PF3D7_0420300, and PF3D7_1239200). The identification of PfISW1 and PfCHD1 in association with PfMORC strengthens the link between PfMORC and a role in chromatin remodeling. This finding suggests that PfMORC may participate in regulating chromatin structure, gene expression during the IDC, and in the specific regulation of var genes, which are critical to antigenic variation in P. falciparum. We note that some nuclear proteins were not identified in this study despite their expected interaction with PfMORC as shown in other studies (Hillier et al. 2019, Bryant et al. 2020, Singh et al. 2021, Subudhi et al. 2023). This may be due to limitations in the experimental conditions and low abundance of the proteins. Despite this, the identification of these nuclear proteins in complex with PfMORC provides insights into potential interactions and regulatory mechanisms involved in molecular mechanisms underlying gene regulation and chromatin remodeling in P. falciparum, which may have implications for developing new strategies to combat malaria.

In other eukaryotic organisms, MORC family proteins are known to function in gene repression and chromatin compaction at heterochromatic regions (Koch et al. 2017). Therefore, to determine if PfMORC localizes to heterochromatic regions across the P. falciparum genome, we performed ChIP-seq assays with MORCHA-glmS parasites during peak PfMORC expression (trophozoite and schizont stages). In general, PfMORC occupied regions 5’–upstream of the ATG start site or bound within coding region, irrespective of the parasite stage. Most importantly, PfMORC peaks were reproducibly detected in subtelomeric regions containing hypervariable multigene families, including the var genes, thereby confirming the findings that PfMORC localized to var gene promoters as reported using dCas9 (Bryant et al. 2020). The specific binding pattern of PfMORC near or within PfHP1-bound regions suggests two critical functions: heterochromatin condensation and gene repression. It is possible that PfMORC changes the nucleosome landscape by either direct association or by binding to different chromatin remodelers. Recent work in Arabidopsis has further confirmed the importance of AtMORC paralogs in gene regulation by chromatin compaction (Zhong et al. 2023), which resembles the function of PfMORC in P. falciparum. Interestingly, in T. gondii, the major function of TgMORC was in the repression of sex-determination genes (Farhat et al. 2020), suggesting MORC family proteins have the capacity to perform diverse functions across eukaryotic organisms.

Based on our immunoprecipitation results, we compared PfMORC occupancy with available ChIP-seq data for the interacting ApiAP2 proteins. Interestingly, our analysis revealed a significant overlap between the binding sites of all ChIP-ed ApiAP2 proteins with PfMORC, suggesting a cooperative role in gene regulation. We also identified enriched motifs similar to those bound by our ApiAP2 proteins of interest, further suggesting the functional cooperation between PfMORC and ApiAP2 proteins. Of note, only one of the seven ApiAP2 of interest in our study has not been ChIP-ed to date (PF3D7_0420300) (Shang et al. 2022). However, we found an enrichment of the DNA motif (TGCACACA) at PfMORC-bound sites. This motif is bound in vitro by PF3D7_0420300 (Bonnell et al. 2023) suggesting that this ApiAP2 protein may localize to these regions. Overall, since these seven ApiAP2 proteins are expressed at distinct time points during the P. falciparum cycle (Bozdech et al. 2003) and regulate different sets of genes (Santos et al. 2017, Josling et al. 2020, Shang et al. 2021, Shang et al. 2022, Subudhi et al. 2023), we believe this indicates a broad function of PfMORC at different stages. In addition, a recent study reported that AtMORC-mediated regulation of transcription may be due to both direct chromatin interactions or indirect association via sequence-specific transcription factors (Zhong et al. 2023), suggesting a complex landscape of chromatin remodeling by MORC family proteins. We also interrogated the co-localization of PfMORC and numerous epigenetic profiles (H2A.Z, H3K9ac, H3K4me3, H3K27ac, H3K18ac, H3K9me3, H3K36me2/3, H4K20me3, and H3K4me1), with a specific focus on H3K36me2, since it has been shown to act as a global repressive mark in P. falciparum (Karmodiya et al. 2015) and other organisms (Strahl et al. 2002, Wagner and Carpenter 2012). Interestingly, we did not find a strong co-localization with any of these epigenetic marks, suggesting a unique role of the epigenetic landscape on PfMORC global occupancy. Therefore, the functional association between PfMORC and a specific, unknown epigenetic mark remains to be determined.

Previous to this work, there was no direct evidence correlating PfMORC-mediated transcriptional changes during the IDC of P. falciparum. Therefore, we investigated the differentially expressed genes (DEGs) in PfMORC knockdown parasites and found two distinct subsets of genes that were enriched. The upregulated DEGs were enriched with genes related to invasion, with downregulated DEGs belonging to hypervariable genes associated with parasite virulence. Upregulation of invasion genes after depletion of PfMORC, along with the putative interaction we identified with PfAP2-I, is particularly interesting as it provides further understanding of the essential red blood cell invasion step of parasite development. Overall, our data with PfMORC-KD revealed a change in the expression of both antigenically variable and invasion-related genes. Expression of clonally variant genes occurs in a different but tightly regulated manner in IDC (Scherf et al. 1998, Scherf et al. 2008), which may be regulated by PfMORC occupancy. Data regarding changes in var genes expression are difficult to interpret, as the KD experiments were performed on a parasite that had not be recently recloned and may therefore express various var genes; single-cell experiments would be needed to clarify the effect of PfMORC KD on var gene regulation.

The Garcia group showed previously that parasites in which PfMORC is knocked-down display reduced sensitivity to melatonin (Singh et al. 2021). This prompted us to investigate if overall gene expression in PfMORC KD parasites is affected by melatonin treatment. We detected only very slight changes (Supplemental Figure 10A-D), suggesting that melatonin does not exert its effect on gene expression through PfMORC, or at least that the latter protein plays a minor role in the process.

This study shows that PfMORC interacts with different ApiAP2 TFs, as demonstrated in previous studies (Hillier et al. 2019, Bryant et al. 2020, Singh et al. 2021, Subudhi et al. 2023). Furthermore, we found that PfMORC is localized at sub-telomeric regions and contains significant overlap with the binding sites of several ApiAP2 transcription factors. Our results support a role for PfMORC in the regulation of hypervariable genes that are essential for Plasmodium virulence and rhoptry genes critical to red blood cell invasion. Collectively, our data identify an important role for PfMORC in chromatin organization, as well as in the epigenetic regulation of gene expression through regulatory complexes with an array of transcription factors, making it an attractive drug target.

Materials and Methods

Plasmodium falciparum culture

The P. falciparum strains were cultured at 37°C in RPMI 1640 medium supplemented with 0.5% Albumax II (Gibco) (Trager and Jensen 1976). Parasites were grown under a 5% CO2, 5% O2, and 90% N2 atmosphere. Cultures were synchronized with 5% sorbitol (Lambros and Vanderberg 1979).

Coimmunoprecipitation and mass spectrometry

Infected erythrocytes at the trophozoite stage were collected from culture and washed twice in 1x phosphate-buffered saline (PBS). The culture pellet was suspended in PBS containing 0.05% (w/v) saponin to lyse the erythrocyte membrane and centrifuged at 8,000 × g for 10 min. The supernatant was discarded, and the parasite pellet was washed 3 times in cold PBS. Samples were lysed in modified RIPA buffer (50 mM Tris, pH 7.5, 150 mM NaCl, 0.5% sodium deoxycholate, 1% Nonidet P-40, 10 µg/ml aprotinin, 10 µg/ml leupeptin, 10 µg/ml, 1 mM phenylmethylsulfonyl fluoride, benzamidine) for 30 min on ice. The lysate was precleared with 50 µl of protein A/G-Agarose beads at 4 °C for 1 h and clarified by centrifugation at 10,000 × g for 10 min. The precleared lysate was incubated with an anti-GFP-Trap-A beads (ChromoTek, gta-20) antibody overnight. The magnetic beads were then pelleted using a magnet (Invitrogen), and the beads were washed extensively. To elute the immunoprecipitated proteins, the magnetic beads were resuspended in 2X SDS loading buffer and resolved by SDS‒PAGE. Following SDS‒PAGE, the whole gel band for each sample was excised and further analysed by mass spectrometry. We used a service provider (CEFAP core-facility de Espectometria de Massa) to analyse GFP-coimmunoprecipitated proteins.

In-gel digestion and peptide desalting

Protein bands from polyacrylamide gel were cut into pieces (approximately 1 mm3), transferred to a clean 1.5 ml low binding tube and washed with washing solution (40% acetonitrile, 50 mM ammonium bicarbonate) until the bands were completely distained and dehydrated with ACN 100% for 5 min followed by vacuum centrifugation. Proteins were then reduced with 10 mM dithiothreitol (DTT) in 50 mM ammonium bicarbonate and incubated for 45 minutes at 56 °C. Protein alkylation was performed with 55 mM iodoacetamide (IAA) in 50 mM ammonium bicarbonate and incubated for 30 minutes at room temperature. Proteins were digested into peptides by trypsin overnight reaction at 37 °C. The trypsin reaction was stopped with 10% TFA (1% TFA final concentration). The supernatant was collected into a new tube. Extraction buffer (40% ACN/0.1% TFA) was added to the gel pieces and incubated for 15 minutes on a thermomixer at room temperature. The supernatant was transferred to the same microtube. The peptide extraction was performed twice and then dried in a vacuum centrifuge. Peptides were resuspended in 0.1% TFA for desalting.

Nano LC‒MS/MS analysis

The LC‒MS/MS system employed was an Easy-nano LC 1200 system (Thermo Fisher Scientific Corp) coupled to an Orbitrap Fusion Lumos mass spectrometer equipped with a nanospray source (Thermo Fisher Scientific Corp). Samples were loaded onto a trapping column (Acclaim PepMap 0.075 mm, 2 cm, C18, 3 μm, 100 A; Thermo Fisher Scientific Corp.) in line with a nano-LC column (Acclaim PepMap RSLC 0.050 mm, 15 cm, C18, 2 μm, 100 A; Thermo Fisher Scientific Corp.). The gradient was 5-28% solvent B (A 0.1% FA; B 90% ACN, 0.1% FA) for 25 minutes, 28-40% B for 3 minutes, 40-95% B for 2 minutes and 95% B for 12 minutes at 300 nL/min. Orbitrap Fusion Lumos mass spectrometer operated in positive mode. The full MS scan had an automatic gain control (AGC) of 5 x 105 ions and a maximum filling time of 50 ms. Each MS scan was acquired at 120K full width half maximum (FWHM) high resolution in the Orbitrap with a mass range of m/z 400-1600 Da. High-resolution dissociation (HCD) with a normalized collision energy set at 30 was used for fragmentation. The resulting MS/MS fragment ions were detected in the Orbitrap mass analyser at a resolution of 30,000. An AGC of 5 x 104 ions and a maximum injection time of 54 ms were used. All raw data were accessed in Xcalibur software (Thermo Scientific).

Database searches and bioinformatics analyses

Raw files were imported into MaxQuant version for protein identification and quantification. For protein identification in MaxQuant, the database search engine Andromeda was used against the UniProt P. falciparum 3D7 strain (March 2021, 5388 entries release). The following parameters were used: carbamidomethylation of cysteine (57.021464 Da) as a fixed modification, oxidation of methionine (15.994915 Da) and N-terminal acetylation protein (42.010565 Da) were selected as variable modifications. Enzyme specificity was set to full trypsin with a maximum of two missed cleavages. The minimum peptide length was set to 7 amino acids. For label-free quantification, the “match between runs” feature in MaxQuant was used, which is able to identify the transfer between samples based on the retention time and accurate mass, with a 0.7-minute match time window and 20-minute alignment time window. Label-free quantification was performed using MaxQuant software with the “match between run” and iBAQ features activated. Protein LFQ and iBAQ ratios were calculated for the two conditions, and the protein IDs were divided accordingly. The mass spectrometry proteomics data have been deposited to the ProteomeXchange Consortium via the PRIDE (Perez-Riverol et al. 2022) partner repository with the dataset identifier PXD036092. PlasmoDB database was used to perform GO analysis.

Total RNA extraction and RNAseq

Infected RBCs containing tightly synchronized trophozoite stage parasites (32 hpi ± 3 h) were harvested and resuspended in TRIzol (Thermo Fisher Scientific). Total RNA was extracted following the manufacturer’s protocol, and an RNA cleanup kit (Qiagen) was used to achieve high-purity RNA. The isolated RNA was quantified using a NanoDrop ND-1000 UV/Vis spectrophotometer, and RNA quality was determined using an RNA ScreenTape System (Agilent 2200 TapeStation). Total RNA (10000 ng) from each sample was stabilized in RNAStable (Biomatrica) and sent to the Micromon Genomics facility at Monash University for next-generation sequencing.

RNA samples were prepared using the MGITech RNA Directional Library Prep Kit V2 (Item No. 1000006385), as per the manufacturer’s instructions, with the following parameters: input RNA: 50 ng, fragmentation: target of 200 bp-400 bp, 87 °C for 6 mins, adapter clean-up: 200 bp-400 bp and library amplification cycles: 16. Libraries were assessed for quantity using the Invitrogen Qubit and dsDNA HS chemistry (Item No. Q33230) and quality/quality using the Agilent Fragment Analyser 5200 with the HS NGS Fragment Kit (Item No. DNF-473-0500). The libraries were pooled in equimolar concentrations and sequenced using an MGITech DNBSEQ-G400RS sequencing instrument with High-Throughput Sequencing Set (FCL PE100, Item No. 1000016950) chemistry.

The quality of the RNA-seq libraries was evaluated using the FastQC tool. Next, we used Salmon (V1.9.0) (Patro et al. 2017) quant with default arguments to quantify the expression of all transcripts in the PlasmoDB release-58 Pfalciparum3D7 genome. The transcript expression was summarized to gene-level expression with tximport 1.22.0 (Soneson et al. 2015). Finally, the gene counts were used to detect differentially expressed genes (DEGs) with DESeq2 (1.34.0) (Love et al. 2014). Furthermore, only genes with an >1 log2 fold change and adjusted p value <0.1 were considered significant for further analysis.

Chromatin immunoprecipitation followed by high-throughput sequencing (ChIP-seq)

PfMORC ChIP-seq was performed similarly to previously published ChIP-seq experiments in Plasmodium falciparum (Josling et al. 2020, Singh et al. 2021, Russell et al. 2022). Five samples in total were collected: biological duplicates using the PfMORCHA-glmS parasite line at the trophozoite stage [30 hpi], biological duplicates using the PfMORCHA parasite line at the schizont stage [40 hpi], and a single replicate using the PfMORCGFP parasite line at the schizont stage [40 hpi]. In brief, the protocol includes five steps: (1) Treated with 1% formaldehyde to crosslink the suspended PfMORCHA-glmS (or PfMORCGFP) parasite cultures (at least 108 trophozoite- or schizont-stage parasites synchronized with 10% sorbitol more than one cycle prior) at 37°C for 10 minutes; (2) Collected parasite nuclei using prechilled glass dounce homogenizer for 100 strokes per 109 trophozoites/schizonts; (3) Lysed parasite nuclei and mechanically sheared chromatin until sufficiently sheared using Covaris Focus-Ultrasonicator M220 (5% duty cycle, 75 W peak incident power, 200 cycles per burst, 7°C, for 5 minutes). (4) We collected 10% of each sample for the nonimmunoprecipitated “input” control and then immunoprecipitated the remaining 90% of each sample. The remaining 90% of each sample was immunoprecipitated with 1:1000 anti-HA antibody (0.5 mg/mL Roche Rat Anti-HA High Affinity [11867423001]) or 1:1000 anti-GFP antibody (0.1 mg/mL Abcam Rabbit Anti-GFP [Ab290]) overnight at 4°C with rotation. (5) DNA was purified after reverse crosslinking using a MinElute column (Qiagen) as directed and quantified by a Qubit fluorometer (Invitrogen).

ChIP-seq library prep for Illumina sequencing

The PfMORC ChIP-seq libraries were performed similarly to previously published ChIP-seq experiments in Plasmodium falciparum (Josling et al. 2020, Singh et al. 2021, Russell et al. 2022). DNA sequencing libraries were prepared for high-throughput Illumina sequencing on the NextSeq 2000 with the 150 x 150 single-end mode. The library prep underwent 12 rounds of amplification using KAPA HiFi polymerase. Completed libraries were quantified using the Qubit fluorometer (Invitrogen) for high-sensitivity DNA and library sequence length by the Agilent TapeStation 4150.

ChIP-seq data analysis and peak calling

The MORC ChIP-seq datasets were analysed similar to previously published ChIP-seq experiments in Plasmodium falciparum (Josling et al. 2020, Singh et al. 2021, Russell et al. 2022). Raw sequencing reads were trimmed (Trimmomatic v0.32.3) to remove Illumina adaptor sequences and low-quality reads below 30 Phred (SLIDINGWINDOW: 4:30). FastQC (v0.11.9) was used to check the quality after trimming. Processed reads were then mapped to the P. falciparum genome (release 57) using BWA-MEM (v0.7.17.2) simple Illumina mode with multiple mapped reads filtered out (MAPQ=1). Once the sequences were mapped, MACS2 (v2.2.7.1) was used to call peaks with each biological replicate and its paired input sample using a standard significance cut-off (q-value=0.01). Using BedTools Multiple Intersect (v2.29.2), the narrow peak output file for each replicate was overlapped to identify the significant peaks in the overlap between both ChIP-seq biological replicates. The overlapping regions were then used to identify an enriched DNA motif (STREME Meme Suite: (Bailey 2021), and putative gene targets of PfMORC were defined as genes with peaks within 2 kb upstream of the gene target ATG start codon or peaks within gene bodies. In a situation with any peaks between gene targets in a head-to-head orientation, the closest gene was chosen.

Data availability

The mass spectrometry proteomics data have been deposited to the ProteomeXchange Consortium via the PRIDE partner repository with the dataset identifier PXD044256. All ChIP-seq samples were submitted to GEO, and a GEO submission ID (GSE239393) was obtained for this section. Additionally, submit all the relevant ChIP-seq files to Zenodo, since UCSC browser doesn’t easily work from Plasmodium falciparum data. All RNA-seq samples were submitted to GEO, and a GEO submission ID (GSE241313) was obtained for this section.

Author Contributions

MKS, CRSG, and ML designed the experiments. MKS, VAB, VFS and MSM performed the experiments, and data were analyzed by MKS, VAB, ITS, GP, ML and CRSG. The primary manuscript was written by MKS and VAB and proofread by CD, ML and CRSG.


This work was supported by grants from Fundação de Amparo a Pesquisa de São Paulo (FAPESP) to CRSG (2017/08684-7 and 2018/07177-7) and to MKS (2019/09490-7). CRSG is supported by “bolsa de produtividade” by CNPq. This work was supported by the National Institutes of Health grant number R01-AI125565 to M.L. and T32-GM125592 to V.A.B. We are grateful to Haemocentro Hospital do Servidor Público for providing blood and plasma. Work in CD laboratory is supported by RMIT University and by grant APP2003712 from the Australian Health and Medical Research Council (NHMRC).

Additional Information

Additional figures and tables are provided separately in Supplemental Figures and Supplemental Tables.

Competing Financial Interests

The authors declare no competing financial interests.

Supplemental Figures

Supplemental Figure 1 –

(A) Coomassie-stained 6% SDS‒PAGE gel showing the parasite lysate of wild-type 3D7 and PfMORCGFP after coimmunoprecipitation with anti-GFP magnetic beads. Both lanes were used for mass spectrometry analysis. (B) Histogram shows the total proteins identified in mass spectrometry analysis from three biological replicates in wild-type 3D7 and PfMORCGFP coimmunoprecipitated samples. (C) Venn diagram showing protein enrichment in 3D7 control samples from three biological replicates from 32 hpi (±4 h) trophozoite stage with anti-GFP-Trap-A beads which is used for normalization. (D) MS/MS normalization of identified proteins from 3D7 parasites expressing PfMORC and transgenic parasites expressing GFP (PfMORCGFP) was carried out. Gene ontology classification showing biological process, cellular component, and molecular function of PfMORCGFP/3D7 normalized proteins showing fold change ≥ 1.5.

Supplemental Figure 2 –

(A) Correlation plot (DeepTools PlotCorrelation) of the 30 h samples compared to the negative control ChIP-seq sample. (B) Correlation plot (DeepTools PlotCorrelation) of the 40 h samples compared to the negative control ChIP-seq sample. (C) Violin plot showing the ChIP-seq fold enrichment values of significantly called peaks in all 6 biological replicates. The two GFP samples were only used as additional controls for comparison purposes. (D) Venn diagram comparing the overlap of MACS2-called peaks between anti-HA biological replicates at 30 h. (E) Venn diagram comparing the overlap of MACS2-called peaks between anti-HA biological replicates at 40 h. (F) Venn diagram comparing the overlap of MACS2-called peaks between anti-GFP biological replicates at 40 h.

Supplemental Figure 3 –

(Top) Profile plot of the mean PfMORC ChIP-seq fold enrichment (Log2[IP/Input]) for all four samples across all PfEMP1 (var) gene 5’ upstream regions and gene bodies. (Bottom) Heatmap of the PfMORC ChIP-seq fold enrichment (Log2[IP/Input]) for all four samples across all PfEMP1 (var) gene 5’ upstream regions and gene bodies. (Inset to the right) Zoom in on the average enrichment of PfMORC at var genes with annotated exons.

Supplemental Figure 4 –

(Top) Profile plot of the mean PfMORC ChIP-seq fold enrichment (Log2[IP/Input]) for all four samples across all rif gene 5’ upstream regions and gene bodies. (Bottom) Heatmap of the PfMORC ChIP-seq fold enrichment (Log2[IP/Input]) for all four samples across all rif gene 5’ upstream regions and gene bodies. (Inset to the right) Zoom in on the average enrichment of PfMORC at rif genes with annotated exons.

Supplemental Figure 5 –

(Top) Profile plot of the mean PfMORC ChIP-seq fold enrichment (Log2[IP/Input]) for all four samples across all rif gene 5’ upstream regions and gene bodies. (Bottom) Heatmap of the PfMORC ChIP-seq fold enrichment (Log2[IP/Input]) for all four samples across all rif gene 5’ upstream regions and gene bodies. (Inset to the right) Zoom in on the average enrichment of PfMORC at rif genes with annotated exons.

Supplemental Figure 6 –

The heatmaps show the transcript abundance (Chappell et al. 2020) of putative PfMORC gene targets at 30 h (left) and 40 h (right). Red signifies high transcript abundance, and green signifies low transcript abundance. Both timepoints are organized into two major clusters (highlighted with the yellow bar and blue bar).

Supplemental Figure 7 –

(A) Associated with Figure 3A,B. Mean fold enrichment (Log2[IP/Input]) summary plot (top) and full heatmap (bottom) of fold enrichment of PfMORC, six associated ApiAP2 factors (AP2-G5, AP2-O5, AP2-I, PF3D7_1107800, PF3D7_0613800, and PF3D7_1239200), HP1, and a negative no-epitope control across PfMORC binding sites at the 30 h and 40 h timepoints. (B) Quantitative Venn diagrams of the binding site overlaps between PfMORC and the six associated ApiAP2 factors.

Supplemental Figure 8 –

DNA motif analyses from these different categories: (1) Unique to 30 hpi ChIP-seq Timepoint, (2) 30hpi ChIP-seq Timepoint, (3) Overlap of ChIP-seq Timepoints, (4) 40hpi ChIP-seq Timepoint, and (5) Unique to 30hpi ChIP-seq Timepoint. The values to the right of each motif contain the enrichment value, number of peaks containing that motif, and percent of the peaks the contain that motif calculated by Meme Suite.

Supplemental Figure 9 –

Mean fold enrichment (Log2[IP/Input]) summary plot (top) and full heatmap (bottom) of fold enrichment of ten selected epigenetic marks (H2A.Z, H3K9ac, H3K4me3, H3K27ac, H3K18ac, H3K9me3, H3K36me2/3, H4K20me3, and H3K4me1) across PfMORC binding sites at the 30 h and 40 h timepoints.

Supplemental Figure 10 –

Comparison of transcriptional changes with melatonin treatment. (A) Volcano plot showing the differentially expressed genes in PfMORC-KD parasites relative to PfMORC-WT after 100 nM melatonin treatment. (B) Venn diagram shows intersecting DEGs from the experiment with KD vs WT with DEGs obtained from the experiment (KD vs WT) treated with 100 nM melatonin for 5 h. Number of DEGs are shown as up (red) and downregulated (green). The intersecting region shows 282 upregulated and 340 downregulated genes. Heatmap showing significant DEGs based on p values and log2FD for upregulating (C) and downregulating (D). These genes are taken from 622 intersecting DEGs showing partial changes in expression after melatonin treatment.