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Open Access

Peer-reviewed

Research Article

Nutrient stress dramatically increases malaria parasite clag2 copy number to increase host cell permeability and enable pathogen survival

  • Nicole B. Potchen ,

    Contributed equally to this work with: Nicole B. Potchen, Tatiane Macedo Silva, Inderjeet Kalia

    Roles Conceptualization, Formal analysis, Investigation, Writing – original draft, Writing – review & editing

    Current Address: Vaccine and Infectious Disease Division, Fred Hutchinson Cancer Center, Seattle, Washington, USA

    Affiliation Laboratory of Malaria and Vector Research, National Institute of Allergy and Infectious Diseases, Division of Intramural Research, National Institutes of Health, Rockville, Maryland, United States of America

    ⨯
  • Tatiane Macedo Silva ,

    Contributed equally to this work with: Nicole B. Potchen, Tatiane Macedo Silva, Inderjeet Kalia

    Roles Investigation, Writing – review & editing

    Affiliation Laboratory of Malaria and Vector Research, National Institute of Allergy and Infectious Diseases, Division of Intramural Research, National Institutes of Health, Rockville, Maryland, United States of America

    ⨯
  • Inderjeet Kalia ,

    Contributed equally to this work with: Nicole B. Potchen, Tatiane Macedo Silva, Inderjeet Kalia

    Roles Formal analysis, Investigation, Writing – review & editing

    Affiliation Laboratory of Malaria and Vector Research, National Institute of Allergy and Infectious Diseases, Division of Intramural Research, National Institutes of Health, Rockville, Maryland, United States of America

    ⨯
  • Justin B. Lack,

    Roles Formal analysis, Methodology, Writing – review & editing

    Affiliation Integrated Data Sciences Section, National Institute of Allergy and Infectious Diseases, Division of Intramural Research, National Institutes of Health, Rockville, Maryland, United States of America

    ⨯
  • Sanjay A. Desai

    Roles Conceptualization, Formal analysis, Methodology, Supervision, Writing – original draft, Writing – review & editing

    sdesai@niaid.nih.gov

    Affiliation Laboratory of Malaria and Vector Research, National Institute of Allergy and Infectious Diseases, Division of Intramural Research, National Institutes of Health, Rockville, Maryland, United States of America

    ⨯

Abstract

To grow and replicate in erythrocytes, malaria parasites must increase the host cell’s permeability to a broad range of nutrients. The plasmodial surface anion channel (PSAC) mediates this increased permeability and has been linked to CLAG3, a protein encoded by a multigene family conserved in Plasmodium spp. Surprisingly, an CLAG3 knockout parasite produced in P. falciparum exhibits incomplete reductions in PSAC activity, propagates normally in standard nutrient-rich media, but is unable to expand in modified media with more physiological levels of key nutrients. To explore these unexpected findings, we used in vitro selections on a CLAG3-null parasite and obtained a mutant capable of expansion under nutrient-limiting conditions. This growth was associated with restored solute uptake despite absence of CLAG3 protein. The mutant parasite expressed channels with characteristics of PSAC though with altered solute selectivity and lack of protease susceptibility, suggesting a modified channel and genome-level changes in the pathogen. Whole-genome sequencing revealed a dramatically increased clag2 copy number without other relevant changes. Quantitative PCR and DNA transfection confirmed increased production of the clag2 gene product. These findings implicate CLAG2 in direct formation of nutrient channels, suggest a new model that accounts for variable expansion of clag genes in Plasmodium spp., and uncover a dramatic genome plasticity available to malaria parasites.

Author summary

Malaria parasites grow within circulating red blood cells and acquire nutrients from human and animal plasma via a pore they insert in the host membrane. This pore is linked to CLAG3, a protein conserved in all examined malaria parasites. Surprisingly, deletion of CLAG3 only partially reduces formation of the nutrient pores, allowing parasites to grow normally under standard culture conditions that provide high levels of nutrients. This CLAG3-null parasite could not grow in modified media with two nutrients reduced to levels resembling those in human plasma. Here, we used prolonged culture of the CLAG3-null parasite in nutrient-limited medium to produce a mutant that can grow at near-normal rates. Despite its inability to express CLAG3, this mutant increased its nutrient uptake using pores with altered properties. Molecular studies revealed DNA-level amplification of the gene encoding CLAG2, a closely related protein from another parasite chromosome. Our findings suggest that malaria parasites can change their DNA in response to sustained changes in nutrient availability as may occur with host migration, climate change, or introduction into new host species.

Citation: Potchen NB, Silva TM, Kalia I, Lack JB, Desai SA (2025) Nutrient stress dramatically increases malaria parasite clag2 copy number to increase host cell permeability and enable pathogen survival. PLoS Pathog 21(10): e1013321. https://doi.org/10.1371/journal.ppat.1013321

Editor: Tania F. de Koning-Ward, Deakin University - Geelong Waurn Ponds Campus, AUSTRALIA

Received: June 21, 2025; Accepted: October 3, 2025; Published: October 16, 2025

This is an open access article, free of all copyright, and may be freely reproduced, distributed, transmitted, modified, built upon, or otherwise used by anyone for any lawful purpose. The work is made available under the Creative Commons CC0 public domain dedication.

Data Availability: All relevant data are within the manuscript and its Supporting Information files. The raw sequencing data generated for this study have been deposited in the NCBI Sequence Read Archive (SRA) under BioProject accession PRJNA1327946.

Funding: This work was funded by the Division of Intramural Research, NIAID/NIH. N.P. was a recipient of an Intramural NIAID Research Opportunities (INRO) Training Award. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.

Competing interests: The authors have declared that no competing interests exist.

Introduction

Malaria parasites evade immune attack by replicating within erythrocytes of their vertebrate hosts. P. falciparum, a virulent and deadly human pathogen, dramatically remodels its host erythrocyte through exported effector proteins that alter the cell’s deformability, cytoadherence and permeability [1–4]. These changes compromise immune evasion because surface display of parasite antigens and altered cellular properties can elicit host immune responses [5–7]. Epigenetic switching of multigene families encoding surface-displayed antigens, such as the PfEMP1 cytoadherence receptor or the RIFIN immunity modulator [8,9], is generally thought to be the parasite’s primary defense against immune recognition.

The clag multigene family is unique because its encoded proteins represent the only surface-displayed antigens conserved throughout the genus Plasmodium. In contrast to other surface exposed antigens, the CLAG proteins do not function in cytoadherence or immune evasion, but instead enable nutrient uptake via formation of the plasmodial surface anion channel (PSAC) [10–14]. While the two copies on chromosome 3 (clag3.1 and clag3.2) are under epigenetic control in P. falciparum [15,16], switching between these paralogs does not alter channel properties but it may finetune parasite replication in human infections [17]. Remarkably, a CLAG3 knockout line exhibits only partially compromised PSAC activity and expands normally in nutrient-rich RPMI 1640-based media, but cannot be propagated in media with more physiological levels of key nutrients [18]. The paralogs encoded by three clag genes on other chromosomes are exported into host cytosol [19], but their roles remain unclear as they have not been linked to PSAC formation [20–23]. Although not subject to mutually exclusive expression like the two clag3 paralogs, clonal variation and a blasticidin S resistant PSAC mutant have established epigenetic regulation of clag2 but not of clag8 or clag9 in P. falciparum [12,15].

We now report copy number variation (CNV) as an alternate parasite strategy for modifying host cell properties. We used in vitro nutrient restriction on CLAG3-null parasites to select a mutant with a nearly 20-fold amplification of the clag2 genomic locus [18]. The resulting increases in CLAG2 expression restored host cell permeability through formation of channels with altered properties. Our studies uncover a capacity for large-scale genome amplification in Plasmodium spp., demonstrate that CNV is a novel strategy for altering host cell properties, reveal evolutionary forces that drive clag gene expansion in Plasmodium spp., and implicate a CLAG2 contribution to nutrient uptake.

Results

Small numbers of CLAG3 knockout parasites persist and expand in nutrient-restricted media

CLAG proteins are translated in late schizont stage parasites and assemble cotranslationally with RhopH2 and RhopH3, two unrelated and conserved parasite proteins, to form the RhopH complex; this complex is targeted to rhoptry organelles in developing merozoites and transferred to the new host cell during erythrocyte invasion [19]. It is then exported into host cytosol, becomes integral at the erythrocyte membrane, and fully induces PSAC activity by the early trophozoite stage [24].

DNA transfection to study clag3 in P. falciparum is complicated by the presence of two copies, clag3.1 and clag3.2, that undergo epigenetic switching and monoallelic expression in most parasite clones [15]. KC5, a laboratory clone that carries a single hybrid clag3 gene termed clag3h [25], was recently used to produce a clag3-null parasite termed C3h-KO [18]. We examined sorbitol and isoleucine permeabilities in synchronous trophozoite-stage cells infected with C3h-KO or the KC5 parent. Both solutes are primarily acquired via PSAC in infected cells [10,26]. Molecular confirmation of these transport studies has been established by knockdown of RhopH2 and RhopH3 [24]. Isoleucine uptake is critical for parasite propagation as it is absent from human hemoglobin and cannot be acquired through hemoglobin digestion [27].

Both solutes exhibited slower osmotic lysis kinetics in C3h-KO (Fig 1A), indicating reduced uptake. Because osmotic lysis kinetics correlate with whole-cell currents in patch-clamp [28,29], these measurements quantitatively estimate permeability reduction (Fig 1B). Sorbitol permeability was reduced by 48 ± 2%; isoleucine exhibited a greater reduction at 68 ± 2% (P < 10-4, Student’s t test, n = 7–21 trials for each solute and parasite). It is not clear why these permeabilities are differentially affected by the loss of CLAG3, but studies implicating distinct routes through PSAC for these solutes may provide a structural basis [30].

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Fig 1. Compromised growth of a CLAG3 knockout in nutrient-limited medium with rare persister parasites.

A) Osmotic lysis kinetics in indicated solutes for C3h-KO and the KC5 wild-type parent (red and black traces, respectively). B) Mean ± S.E.M. permeabilities, calculated as 1/lysis halftime from osmotic lysis kinetic experiments. Black and red bars represent KC5 and C3h-KO. C) Parasitemia (% infected cells), estimated from daily microscopic examination of Giemsa-stained thin smears, for KC5 and C3h-KO (black and red symbols). Propagation in standard RPMI-based medium and in PGIM are shown as circles and triangles, respectively. While the knockout expands normally in RPMI-based medium, its cultures fail to expand in PGIM. Symbols, mean ± S.E.M. parasitemias from 3-4 independent trials each. D) Microscopic image of Giemsa-stained infected cell with two trophozoite-stage C3h-KO parasites observed during cultivation in PGIM. Occasional ring- and schizont-stage parasites were also observed. E) Osmotic lysis kinetics in sorbitol with 0, 2, 4, 6, 8, 10 nM ISG-21 (left to right traces, respectively). Note slowed kinetics due to reduced sorbitol uptake by ISG-21 block. Right panel, mean ± S.E.M. lysis halftimes (t0.5) vs. ISG-21 concentration from sorbitol uptake experiments as in left panel, calculated from up to 6 independent trials at each concentration. Horizontal red line represents the mean inhibitor-free sorbitol t0.5 for C3h-KO from Fig 1B. F) Lysis kinetics in isoleucine with 0, 10, 20, 30, 40, 50 nM ISG-21 (left to right traces). Higher concentrations of this and other inhibitors are required to block isoleucine transport through PSAC [30]. Right panel, mean ± S.E.M. lysis halftimes (t0.5) vs. ISG-21 concentration from isoleucine uptake experiments (n up to 3 each). Red line, mean inhibitor-free isoleucine t0.5 for C3h-KO from Fig 1B. G) Propagation of parasites in PGIM with indicated nanomolar concentrations of ISG-21. Black symbols represent mean ± S.E.M. parasitemias for wild-type; red line reflects C3h-KO growth, reproduced from panel C for comparison (n = 3-4 trials each).

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We next examined the effect of reduced host cell permeability on in vitro parasite propagation and found that C3h-KO cultures expanded at rates comparable to KC5 in standard RPMI 1640-based medium (red vs black circles, Fig 1C), a general-purpose formulation with supraphysiological levels of most nutrients. Cultivation in a more physiological medium designed to evaluate PSAC inhibitors under conditions that simulate human plasma (PGIM, PSAC growth inhibition medium) [16], however, revealed a dramatic difference as KC5 cultures continued to expand while the C3h-KO parasitemia failed to increase over 8 days (Fig 1C). KC5 expansion was slower in PGIM than in the standard RPMI 1640-based medium (black triangles vs. black circles, Fig 1C), as has been reported previously for other wild-type parasite lines [16]. This reduced propagation in PGIM presumably reflects growth limitation due to nutrient restriction. Because growth rates in PGIM are comparable to those in human serum without addition of commercial media [16], PGIM may predict in vivo parasite nutrient access and replication more faithfully than RPMI 1640. Thus, stalled growth of the C3h-KO line in PGIM suggests that CLAG3 is essential for parasite expansion in human infections.

Interestingly, microscopic examination revealed occasional apparently healthy C3h-KO infected cells despite PGIM cultivation for more than 10 days (Fig 1D). To examine viability, we cultured C3h-KO in PGIM for various durations and quantified recovery from nutrient restriction upon return to the standard RPMI-based medium (S1A Fig). Each culture quickly resumed normal expansion; increasing the duration of PGIM exposure to 8 days did not increase the lag time (S1B Fig), indicating that a stable fraction of C3h-KO parasites remains viable in PGIM over this duration. One possibility is that compromised nutrient acquisition, imposed here through the combination of reduced host cell permeability and limited nutrient levels in the external medium, triggers a dormant parasite state [31,32].

Growth compromised to a greater extent than expected from permeability reduction

The marked reduction in growth using PGIM is surprising given the incomplete reduction in solute permeabilities in the C3h-KO line. To explore this finding quantitatively, we measured expansion of wild-type parasite cultures in the presence of ISG-21, a potent and specific PSAC inhibitor also known as MBX-2366 [33]. We quantified dose-dependent ISG-21 inhibition for both sorbitol and isoleucine uptake (Fig 1E and 1F). We then estimated the ISG-21 concentration required to reduce each solute’s permeability in wild-type KC5 parasites to levels matching those in C3h-KO without inhibitor addition (right panels, Fig 1E and 1F). The dose-response profiles for sorbitol and isoleucine as well as the ISG-21 concentrations required to yield osmotic lysis halftimes matching values for C3h-KO without inhibitor addition, 1.2 and 3 nM respectively, differed modestly, possibly reflecting these solutes’ distinct transport mechanisms through PSAC [30,34].

We then cultured the KC5 parental line with and without ISG-21 and compared expansion to that of C3h-KO cultivated without inhibitor. Remarkably, although 10 nM ISG-21 reduces permeability to a much greater extent than clag3 knockout, growth of KC5 in PGIM despite addition of this inhibitor is comparatively well-preserved (Fig 1G), indicating that reduced permeability of these solutes does not adequately account for C3h-KO’s failure to expand in PGIM. These findings are consistent with parasite growth as a complex process dependent on PSAC for uptake of many nutrients from an incompletely defined medium and intracellular utilization; there may also be contributions from channel-mediated efflux of soluble metabolic waste products, some of which remain unknown.

In vitro selection with PGIM restores host cell permeability via altered channels

As rare parasites were observed in nutrient-restricted cultures (Fig 1D), we used in vitro selection of C3h-KO to identify mutants capable of expansion in PGIM. A gradually increasing parasitemia suggested selection of replicating parasites (Fig 2A). After ~ 2 months, expansion yielded the KO-PGIM parasite pool suitable for molecular and biochemical studies. Cross-contamination with wild-type lines was excluded by PCR, which revealed an unchanged deletion locus in KO-PGIM and no detectable wild-type band (Fig 2B, p1-p2 amplicons); PCR from the unmodified downstream sequence also did not reveal changes that might have resulted from indels or other recombination events (p3-p4 and p3-p5). DNA sequencing of the clag3 promoter and deletion locus excluded mutations that could confer growth advantage to KO-PGIM and further excluded cross-contamination with wild-type parasites.

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Fig 2. Growth in PGIM after in vitro selection is linked to altered channel properties.

A) Timeline of parasitemia increase in a C3h-KO culture continuously maintained in PGIM. After 2 months, the resulting KO-PGIM reached levels suitable for secondary studies. B) Ethidium-stained gel showing PCR amplicons from indicated parasite lines and primers. Ribbon schematic above the gel shows the CRISPR/Cas9 transfection strategy used to produce C3h-KO; a 359 bp smaller amplicon from primers p1 and p2 is predicted for C3h-KO and its derivatives because transfection deletes part of the clag3 exon 1 and replaces it with three stop codons; amplicons distal to the disrupted size are unchanged. Primer sequences are provided in S1 Table. C-D) Osmotic lysis kinetics in sorbitol and isoleucine for the wild-type KC5 parent, the C3h-KO knockout, and KO-PGIM (black, red, and cyan traces in this and subsequent figures, respectively). Notice restored lysis kinetics for KO-PGIM. Bar graphs, mean ± S.E.M. sorbitol permeabilities of indicated lines. For sorbitol, KO-PGIM measurements are separated into trials between 68-120 days after initiation of in vitro PGIM selection and those after 200 days of selection; isoleucine trials for KO-PGIM performed between 211-330 days of selection. n ≥ 4 trials for each condition. E) Lysis kinetics in sorbitol for matched cultures of KO-PGIM maintained in PGIM (cyan trace) or returned to nutrient-rich RPMI 1640 medium for 204 days (KO-rev, dark red trace). F) Mean ± S.E.M. permeabilities of indicated solutes for KO-PGIM and KO-rev (cyan and dark red bars); n = 3-12 trials each. G) Mean ± S.E.M. propagation of KC5, KO-PGIM and KO-rev in the nutrient-limited PGIM (black, cyan, and dark red symbols, respectively); n = 2-4 trials each. H) Osmotic lysis kinetics in sorbitol for indicated parasites with and without pronase E treatment (green trace in each panel). Note that channels on C3h-KO and KO-PGIM are pronase E-resistant. I) Mean ± S.E.M. permeabilities after pronase E treatment, normalized to 1.0 for matched untreated controls.

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Remarkably, sorbitol permeability was significantly increased in the selected parasite when compared to C3h-KO (Fig 2C, P < 0.0001, n = 4 trials), reaching levels modestly greater than those of the KC5 wild-type parent (P = 0.07 for comparison to KC5). To explore ongoing changes that may confer additional survival advantages, we continued KO-PGIM propagation in PGIM for over 1 year; transport measurements revealed modest additional increases in sorbitol permeability (Fig 2C, bar graph; 8 trials after 200 days of cultivation in PGIM), suggesting a plateau in uptake kinetics. Isoleucine permeability also increased over this period but was not fully restored to wild-type levels (Fig 2D, P = 0.006 when compared to KC5, n = 8–10 trials each). The correlation between restored growth in nutrient-limited PGIM and increased solute permeabilities suggests that parasite replication depends on sufficient PSAC-mediated uptake of essential solutes under physiological nutrient levels.

To explore whether the increased permeability is reversible and sustained by nutrient restriction, we next returned KO-PGIM to nutrient-rich RPMI 1640-based media to generate a parasite pool we termed KO-rev. Transport studies after continuous cultivation in nutrient-rich standard medium for up to 228 days revealed modest, statistically insignificant decreases in sorbitol and isoleucine permeabilities (Fig 2E and 2F; P ≥ 0.19 for comparisons to KO-PGIM maintained in PGIM). This finding suggests stable increases in permeability not dependent on continued nutrient restriction.

To further evaluate the selected mutant’s stability, we examined parasite expansion rates and found that KO-rev retained its ability to expand in PGIM despite growth in nutrient-rich RPMI 1640-based media for up to 165 days (Fig 2G). Both KO-PGIM and KO-rev could be propagated in PGIM, albeit at rates below that of the wild-type KC5 parent.

Interestingly, our analysis revealed changes in relative solute permeabilities for the selected KO-PGIM mutant that could not be explained by simple upregulation of transport. While cells infected with KC5 parasites have a 2-fold greater permeability to isoleucine than to sorbitol (black bars in Fig 2C and 2D; P < 0.0001), KO-PGIM parasites produce channels with negligible differences between these solutes’ permeabilities (cyan bars in Fig 2F, P = 0.21). This altered preference reflects changes in the channel’s solute selectivity and indicates that the increased permeabilities in KO-PGIM do not result from an increased number of unmodified channels; channels with altered properties are instead required.

We explored channel properties further using protease susceptibility studies as protease treatment of intact infected cells is known to compromise PSAC activity [10,35]. Although proteases cleave many host and parasite proteins on infected cells, genetic mapping and molecular studies have established that CLAG3 cleavage within an exposed variant loop accounts for the transport’s protease susceptibility [36]. Here, we used pronase E, a mixture of nonspecific proteases active against nearly all exposed sites, and found reduced uptake by wild-type cells (Fig 2H, KC5) [36]. In contrast, channels associated with C3h-KO were insensitive to pronase E. Although sorbitol permeability is restored to wild-type levels, the channels on cells infected with KO-PGIM were also unaffected by this treatment (Fig 2H and 2I; P < 0.0001, one-way ANOVA with post-hoc Tukey’s multiple comparisons test; n = 3–8 trials each parasite). Solute uptake into cells infected with C3h-KO and KO-PGIM is resistant to pronase E, further implicating channels with altered properties.

We then used whole-cell patch-clamp to examine channel-mediated Cl- flux in these clonal lines [28]. While uninfected human erythrocytes have substantial exchange-restricted Cl- flux through the Cl-/HC03 exchanger [37], they mediate negligible conductive Cl- flux and have small whole-cell currents at all membrane potentials (Vm) [38]. Induction of PSAC activity on the infected cells permits net Cl- flux and relatively large currents in whole-cell patch-clamp, which measures net ion flow only at the plasma membrane of a single infected cells (Fig 3A, schematic). These currents have been confidently linked to PSAC through electrophysiological studies of conditional knockdown of either RhopH2 or RhopH3, where net Cl- transport is abolished [24].

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Fig 3. Whole-cell patch-clamp reveals altered solute selectivities.

A) Whole-cell patch-clamp recordings on cells infected with indicated parasites. In each group of traces, current responses to 50 ms pulse application of membrane potentials (Vm) between -100 and +100 mV in 10 mV increments are superimposed; Vm held at 0 mV between pulses. Red dashes, zero current level. Notice the larger negative currents at -100 mV (bottom trace in each group) than positive currents at +100 mV (top trace in each group), indicating preserved voltage-dependent gating in each clone’s channels. Schematic at top left, whole-cell configuration on an infected erythrocyte. Scale bar at bottom right, 2 nA (vertical)/ 20 ms (horizontal). B) Mean ± S.E.M. whole-cell chord conductances (γ) determined from currents at applied Vm between -100 to 0 mV (n = 3-15 cells for each line). C) Mean ± S.E.M. currents (I) at each applied Vm for KC5, C3h-KO, and KO-PGIM (black, red, and cyan symbols, respectively), normalized to -100 at Vm = -100 mV. PSAC voltage-dependence, apparent as steeper slopes of these profiles at negative Vm, does not differ significantly between these clones. D) Voltage-dependent inactivation in response to 1 s pulses to Vm = -100 mV for indicated lines. Scale bar, 2 nA/400 ms.

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In our studies, KC5 exhibited larger currents at negative membrane potentials (Vm) than at positive values (Fig 3A), consistent with PSAC’s voltage-dependent gating. Remarkably, although organic solute permeabilities are reduced in C3h-KO, we found that Cl- conductance was not significantly decreased (Fig 3A and 3B; P = 0.99 for post-hoc Tukey’s multiple comparison test; n = 3–15 cells each). Also surprisingly, KO-PGIM produced even larger whole-cell currents (P < 0.0001). The channel’s voltage dependence was not affected by either clag3 knockout or by subsequent PGIM selection (Fig 3C); a modestly greater inward rectification for Ch3-KO and KO-PGIM, apparent in the I-Vm plot as smaller normalized currents at Vm of +100 mV, was not significant (P = 0.05, one-way ANOVA). Voltage-dependent inactivation, a property previously linked to a cleavable cytoplasmic domain on PSAC [39], was also preserved in these lines (Fig 3D). Cell-to-cell variation in inactivation kinetics and magnitude, which appear to reflect variable liberation of cytoplasmic channel components during whole-cell patch-clamp [39], prevented comparison of inactivation time courses. Thus, CLAG3 knockout and in vitro PGIM selections produce complex and unexpected changes in channel properties.

A markedly increased copy number for the clag2 paralog

To examine possible molecular mechanisms for adaptation to nutrient restriction and the observed transport changes, we performed whole-genome long-read sequencing of the KC5 parent, the C3h-KO transfectant, and the KO-PGIM mutant. After quality filtering and alignment to the reference sequence, average read lengths ranged between 10,900 and 11,800 base pairs with median coverages of 128-fold to 160-fold. These long-read lengths revealed a marked increase in clag2 copy number resulting from multiple duplications of a 6.8 kbp region that included the entire ORF and flanking untranslated sequences (Fig 4A and S2 Table).

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Fig 4. Dramatic clag2 amplification in KO-PGIM.

A) Integrative Genomics Viewer image of the locus containing clag2 (PF3D7_0220800), showing sequencing coverage and alignment (cvrg and align) for KC5, C3h-KO, and KO-PGIM. Coverage is scaled to show the markedly increased coverage of a 6.8 kb region including clag2 in KO-PGIM, suggesting multiple duplication events. Positions matching the reference genome sequence are gray and mismatches are colored depending upon the mutant allele. The amplified region begins 753 bp upstream of the clag2 transcription start site and ends 15 bp before the mRNA terminus; its chromosomal positions are listed in S2 Table. B) Schematic shows inverted PCR strategy to identify tandem duplication events. Ethidium-stained gel showing that the wild-type KC5 does not produce an amplicon, but that C3h-KO produces a single band and PGIM-selected lines produce multiple bands, implicating duplication in C3h-KO and many copies in KO-PGIM and KO-rev. C) Mean ± S.E.M. DNA copy numbers of indicated genes in KC5, C3h-KO, KO-PGIM and KO-rev (left to right bars in each group), estimated by qPCR.

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An additional 910 bp deletion in PF3D7_1418600, one member of the multigene 5S rRNA family, was detected in KO-PGIM relative to KC5 and C3h-KO. We also compared genomic sequences to detect mutations relative to the reference and sought differences between the parental and derivative strains. Only two were found in KO-PGIM relative to KC5 and C3h-KO (blue rows, S3 Table). The PF3D7_1418600 deletion and these mutations—a 5’UTR indel in Pf3D7_0608700 and a nonsynonymous mutation in Pf3D7_0821400 encoding a small uncharacterized protein with predicted nuclear localization—were deemed unlikely to contribute to the selected mutant phenotype and were not pursued further.

PCR using a reverse primer at the start of the clag2 gene and a forward primer at the gene’s 3’ end excluded detectable tandem duplication in KC5, but revealed a low-level amplification in the C3h-KO line (Fig 4B). This amplification, not reported in previous studies of the C3h-KO knockout [18], may reflect a compensatory change required for growth of successfully transfected cells carrying the engineered CLAG3 knockout. PCR revealed a more dramatic clag2 amplification in KO-PGIM, with several bands and more intense amplicons that parallel the multiple duplication events suggested by whole-genome sequencing. Real-time quantitative PCR (qPCR) was then used to estimate clag2 copy numbers at 2, 18, and 8 in C3h-KO, KO-PGIM, and KO-rev, respectively (Fig 4C; P < 10-4, n = 4 independent trials).

CLAG2 upregulation accounts for altered channels and growth phenotype

Because clag genes are known to undergo complex epigenetic regulation and silencing, we next used real-time quantitative reverse transcriptase PCR (RT-qPCR) to explore whether genome-level clag2 amplification alters transcription of clag paralogs, rhoph2 and rhoph3. Consistent with the marked copy number increases observed in Fig 4, RT-qPCR using synchronized, trophozoite-infected parasites identified a marked upregulation of clag2 transcription in both KO-PGIM and KO-rev (Fig 5A; P = 2 x 10-4, one-way ANOVA; n = 3–4 trials each parasite). Significant changes in transcript abundance were not detected for other clag paralogs, rhoph2, or rhoph3; clag3 transcripts remained at or below detection thresholds (Figs 5A and S2). Paralleling an apparent copy number reduction upon return to RPMI 1640-based media (Fig 4C), clag2 expression decreased upon extended propagation in nutrient-rich media (Fig 5A, dark red bars for KO-rev; P = 0.002 in post-hoc multiple comparison test). Although evolving gene copy number, possible promoter and ORF mutations, and cell-level epigenetic marks complicate attempts to correlate copy number and transcript abundance, comparisons of our qPCR and RT-qPCR results (Figs 4C and 5A, respectively) suggest that increased clag2 transcription results primarily from genome-level amplification without controlling effects of epigenetic marks.

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Fig 5. Increased clag2 transcription and translation.

A) Mean ± S.E.M. expression of indicated clag and rhoph genes in KC5, C3h-KO, KO-PGIM, and KO-rev parasites (black, red, cyan, and dark red bars in each group, respectively; n = 3-4 independent RNA harvests each), normalized to 1.0 for matched measurements using the KC5 wild-type parent. The msp2 control is included as an unrelated gene with similar stage-specific expression; similar msp2 transcript levels establish matched harvest of cell cycle stages. B) CRISPR/Cas9 transfection strategy for C-terminal addition of a NanoLuc reporter tag on CLAG2. Indicated primers were used for PCR integration checks (S3A Fig and S1 Table). C) Nano-Glo blot showing the tagged CLAG2 protein in indicated lines. Loading control, anti-aldolase immunoblot at bottom. Notice the increased intensities in C3h-KOC2NLuc and KO-PGIMC2NLuc. Right panel, mean ± S.E.M. CLAG2 band densities, normalized to the loading control and presented in arbitrary units (AU) for each parasite. n = 3 independent harvests and blots. D) Osmotic lysis kinetics for KO-PGIMC2NLuc in sorbitol. The lysis halftime t1/2, 5.6 min, is comparable to untransfected KO-PGIM, suggesting that NanoLuc tagging does not alter channel activity. Representative of 2 independent trials.

https://doi.org/10.1371/journal.ppat.1013321.g005

To examine the effects of increased clag2 transcription, we used CRISPR transfection of KC5, C3h-KO and KO-PGIM to introduce a C-terminal NanoLuc tag on CLAG2 (Fig 5B). Integration PCRs using the resulting limiting dilution clones—KC5C2NLuc, C3h-KOC2NLuc and KO-PGIMC2NLuc—confirmed faithful addition of the tag and replacement of all clag2 genomic copies in each line, without residual wild-type copies of the gene (S3A Fig). Indirect immunofluorescence microscopy revealed that the modified protein was transferred to new erythrocytes after invasion and exported to the host cell cytoplasm with RhopH3 (S3B Fig), as previously reported for each CLAG paralog [19,20].

We then estimated CLAG2 abundance on nitrocellulose blots with the Nano-Glo blotting system, which can quantify NanoLuc expression [40]. ImageJ quantification with loading control normalization revealed marked increases in the tagged protein with KO-PGIMC2NLuc having greater increases than C3h-KOC2NLuc (Fig 5C right panel; P = 0.01, n = 3 independent trials each). This C-terminal tag did not compromise the increased solute uptake of the KO-PGIM mutant (Fig 5D). Although the transfection strategy included a glmS element in the 3’ UTR of clag2, our attempts to examine conditional knockdown using this riboswitch were unsuccessful, possibly due the presence of multiple gene copies with separate promoters and glucosamine-associated toxicity on parasite cultures. Cas9-mediated cleavage during transfection, possible changes in channel-mediated nutrient uptake due to CLAG2 tagging, and variable genome remodeling in transfection subclones all may alter clag2 copy number.

We also found that the increased CLAG2 abundance in the untransfected KO-PGIM could be detected in conventional immunoblots due to cross-reactivity with the anti-CLAG3 antibody (S4A Fig), consistent with significant sequence homology over the epitope used for production of this antibody (S4B Fig). We excluded low-level contamination with parasites carrying the wild-type clag3 locus (Fig 2B); ectopic recombination to transfer the distal clag3 sequence that encodes the antibody epitope to another clag paralog [10], as established for other gene families in P. falciparum [41], was also excluded with PCR experiments (S4C and S4D Fig).

Discussion

Epigenetic switching of variant surface antigens is considered P. falciparum’s primary method of responding to changes in the host environment [42,43]. Switching and expression of single PfEMP1 paralogs, as encoded by members of the var gene family, allows infected cells to escape newly-mounted immune responses [44]. PfEMP1 isoforms bind to distinct endothelial receptors [45], so switching also bestows infected cell tropism for different host tissues and organs. This is particularly advantageous in pregnancy where placental sequestration leads to marked parasite expansion [46]. Epigenetic control of RIFINs, encoded by the rif gene family, is not under the same tight regulation as var gene transcription [47], but upregulation of specific rif genes facilitates evasion through LILRB1 or LAIR1 receptor binding to suppress host immune responses [9]. Frequent recombination between member genes for these variant antigens (50–60 var genes and 150–200 rif genes in P. falciparum clones) also generates distinct paralogs with new properties [48]. Despite the remarkable plasticity of these genes and their transcription profiles, studies have not revealed drastic changes in copy number for these and other variant surface antigens in Plasmodium spp.

We now report copy number variation (CNV) as a distinct parasite mechanism for responding to changes in host plasma. Although CNV generally cannot match the speed and reversibility characteristic of epigenetic regulation, it can provide adaptive advantage under sustained selective pressure. In our study, nutrient restriction appears to have promoted repeated duplication events including the full-length clag2 gene and essential flanking sequences. The gene’s subtelomeric location may have facilitated amplification as such sites are hotspots for chromosome reshuffling [49,50]. Copy number changes can arise in clinical P. falciparum isolates [51], but have been largely limited to intracellular parasite proteins with minimally variant sequences. PfMDR1, a transporter on the parasite’s digestive vacuole, exhibits CNV to acquire resistance to mefloquine, quinine and halofantrine [52,53]; resistant clinical isolates have at most 2–4 copies of the pfmdr1 gene, but they revert to a single copy upon drug removal to reduce the associated fitness cost [54]. GTP cyclohydrolase underwent a similar duplication in some clinical isolates to confer sulfadoxine resistance [55]. Genome-level amplifications are generally considered deleterious, especially when open reading frames are involved [56]. Thus, clag2 amplification to 18 copies in KO-PGIM represents an unprecedented increase. It appears to have been necessary to restore uptake of isoleucine, an essential amino acid, establishing that nutrient restriction provided the selective pressure to drive amplification. KO-rev, as obtained after return of the mutant to nutrient-rich medium, exhibits a lesser copy number increase, consistent with a balance between the benefit of restored nutrient uptake and the fitness cost from high-level amplification.

There are many potential explanations for why an 18-fold increase in clag2 copy number was required for KO-PGIM expansion in PGIM. These include lower transcription and translation rates for clag2 than clag3 (S2 Fig), differing affinities of CLAG paralogs for interaction and transport in the RhopH complex, differing efficiencies of channel subunit delivery and insertion at the host membrane (a highly regulated process for other ion channels [57]), variable subunit stoichiometries in functional channels, and differences in relative permeabilities of key nutrients in the channels formed by combinations of expressed paralogs. These possibilities may be explored when the PSAC structure is solved.

As with mutations and indels, CNV appears to rise regularly in parasite populations only to disappear quickly in the absence of associated survival advantage. CLAG3 knockout to produce C3h-KO provided adequate survival advantage to yield a detectable subpopulation with 2 or more copies of clag2 despite cultivation in nutrient-rich RPMI 1640-based medium (Fig 4B); greater selective pressure upon transfer to PGIM presumably enabled growth of individual parasites carrying larger scale clag2 amplifications. Thus, our findings help establish the pathogen’s remarkable capacity for CNV under appropriate and sustained selective pressure.

When compared to other multigene copies, clag genes exhibit an unparalleled range of species-specific family sizes in Plasmodium spp. with some species such as P. berghei having only two copies and others exhibiting marked expansion, with the gorilla parasite P. blacklocki having over 35 copies [58,59]. Even within a single species, P. falciparum isolates are also known to have clag copy numbers that range between 3 and 7 even without engineered clag3 knockout [60]. The reasons for this variable expansion are unclear, but our findings suggest nutrient restriction in specific hosts may be a key driving force. Copy number increases appear to be followed by ongoing evolution of members through mutations [60]. Interestingly, despite variable expansion, each examined Plasmodium species has a single clag closely related to the P. falciparum clag9 gene while all other members group with P. falciparum clag3. While a distinct role for clag9 has been proposed and debated [21,23], the encoded CLAG9 protein shares key phenotypes with the CLAG3 group: translation in schizonts, trafficking as a ternary complex with RhopH2 and RhopH3 via merozoite rhoptries into new erythrocytes upon invasion, and similar membrane topologies at the host cell surface [59].

In combination with copy number, epigenetic regulation of clag member genes serves to regulate total production of CLAG protein but the reasons for this complex regulation are unknown [61]. One possibility, switching between members to allow fine-tuning of nutrient uptake in response to changing host nutritional status [17], is appealing and consistent with some of our findings, but is unfortunately not associated with differences in nutrient permeability, as might be predicted [16]. Another possibility, switching between clag3 genes and potential up- and down-regulation of other paralogs to permit immune evasion, is also unsatisfying, given that other multigene families require a larger number of paralogs to achieve satisfactory escape from mounted immune responses [62]. In addition to changes in PSAC-associated subunits, nutrient stress may also produce adaptive changes in the intracellular pathogen including altered expression of sugar and amino acid transporters; one example is PfAAT1, an amino acid transporter and drug susceptibility modulator localized at the parasite digestive vacuole [63].

We propose that this complex multi-layered regulation may be driven by a need to achieve adequate nutrient uptake while maintaining a sufficiently low Na+ permeability to avoid premature osmotic lysis of infected cells. While PSAC has an unparalleled ability to exclude this cation [64], there is a nonzero Na+ leak through the channel [65]. Upregulated nutrient permeability, as required when the host may be malnourished, must be achieved without increasing Na+ uptake to levels that would lead to infected cell lysis before lifecycle completion. Fine-tuning of each paralog’s expression may enable balanced permeabilities for multiple solutes in response to host nutritional status [15,20]. Consistent with this model, in vitro selections of mutant channel phenotypes, in the present study and in production of a mutant with reduced blasticidin S uptake [11,12,66], invariably leads to reversion to wild-type phenotypes when selection is removed.

Methods

Parasite culture and in vitro selection

Asexual P. falciparum parasites including KC5 and its derivative C3h-KO, KO-PGIM, and KO-rev lines were cultivated at 5% hematocrit in O+ human erythrocytes (Interstate Blood Bank, Inc.). All cultures were maintained with regular media changes under 5% O2, 5% CO2, 90% N2 at 37 °C. Standard, nutrient-rich propagation used RPMI 1640 medium supplemented with 25 mM HEPES, 31 mM NaHCO3, 0.37 mM hypoxanthine, 10 µg/mL gentamicin, and 0.5% w/v NZ Microbio BSA (MP Biomedicals).

In vitro selection for C3h-KO parasites capable of expansion in physiological, nutrient-restricted medium was performed using PGIM medium with modifications [16]. PGIM was prepared using glutamine and isoleucine deficient RPMI 1640 (US Biological) supplemented with 25 mM HEPES, 31 mM NaHCO3, 3.01 µM hypoxanthine, 11.4 µM L-isoleucine, 10 µg/mL gentamicin, and 0.5% w/v NZ Microbio BSA. Erythrocytes were washed in PGIM before addition to cultures to minimize carryover of supraphysiological nutrient levels. Propagation was evaluated with microscopic examination of Giemsa-stained smears. Expansion rate analysis used sorbitol-synchronized cultures seeded at 0.5% initial ring-stage parasitemias. Some comparisons of parasite growth rates used blinded examination of smears to exclude observer bias. Two independent trials of in vitro PGIM selection produced similar results.

DNA sequencing and PCR were performed with selected lines to exclude contamination by other parasite strains and to evaluate possible genomic recombination. DNA was isolated from parasite cultures using Quick-DNA Miniprep kit (Zymo Research) according to the manufacturer’s protocol. Primers used are listed in S1 Table.

Solute uptake measurements

PSAC-mediated uptake of solutes was measured using transmittance-based tracking of infected cell osmotic lysis. Synchronous cultures containing trophozoite- and schizont-stage infected cells were harvested and enriched to > 95% parasitemia using percoll-sorbitol density gradient separation. Prior studies have found that trophozoite- and schizont-infected cells have maximally induced PSAC activity on their host cells. Enriched cells were washed in saline (150 mM NaCl, 20 mM HEPES, pH 7.4) before resuspension at 0.125% hematocrit in lysis solution (280 mM sorbitol or 280 mM isoleucine with 20 mM HEPES, 0.1 mg/mL BSA, pH 7.4) at 37 °C. Solute uptake and the resulting osmotic lysis were tracked at 15–20 s intervals by recording transmittance of 700 nm light through the cell suspension (DU800 spectrophotometer with Peltier temperature control, Beckman Coulter). Where used, ISG-21, a potent PSAC inhibitor [16], was freshly prepared in lysis solution before each experiment. Solute permeabilities and inhibitor efficacies were determined using locally developed code (SigmaPlot, Systat), based on a two-compartment model of infected cell osmotic lysis [29].

Protein blots

CLAG protein expression was evaluated with immunoblotting of cell membranes. Sorbitol-synchronized cultures were evaluated for maturity by examination of serial Giemsa-stained smears and harvested at matched levels of trophozoite- and schizont-infected cells. Infected cells were enriched by percoll-sorbitol separation and lysed in hypotonic buffer (7.5 mM Na2HPO4, 1 mM EDTA, 1 mM PMSF at pH 7.5) at 4 °C. Membrane-associated proteins were enriched by centrifugation (14,000 x g, 30 min at 4 °C) and solubilized in modified Laemmli buffer with a final 6% SDS concentration. Proteins were separated by electrophoresis in 4–15% Mini-PROTEAN TGX gels (Bio-RAD) and transferred to nitrocellulose membrane. This membrane was blocked for 1 h in 3% milk solution in TBST (150 mM NaCl, 20 mM TrisHCl, pH 7.4 with 0.1% Tween20) at room temperature. Primary anti-CLAG3 and secondary HRP-conjugated anti-mouse antibodies were applied in blocking buffer as described previously [24]. Bound antibodies were visualized on Hyblot X-ray film after addition of Clarity Western ECL chemiluminescent substrate (Bio-Rad).

Nano-Glo blots (HiBiT blotting system, Promega) were used to quantify CLAG2 abundance in engineered lines expressing NanoLuc-tagged protein using antibody-free blotting to measure luminescence on membranes [40]. After SDS-PAGE and transfer to nitrocellulose membranes, blots were washed in 150 mM NaCl, 20 mM Tris-HCl (pH 7.4) with 0.1% Tween 20. Furimazine was then added in blotting buffer at a 1:500 dilution before imaging and band intensity quantification using ImageJ software (NIH) and normalization with an aldolase loading control (HRP anti-Plasmodium aldolase antibody, Abcam).

Protease susceptibility

Enriched late-stage infected cells were washed and resuspended in PBS-2 (140 mM NaCl, 2.7 mM KCl, 9.6 mM Na2HPO4, 1.5 mM KH2PO4, 0.6 mM CaCl2, 1 mM MgCl2, pH 7.4) with 0.5 mg/mL pronase E (Sigma Aldrich) at 2.5% hematocrit. Cells were incubated with protease for 1 h at 37 °C. The cells were then washed with ice-cold PBS-2 supplemented with 1 mM phenylmethylsulfonyl fluoride (PMSF) and 1 mM EDTA before resuspension in saline for solute uptake measurements or hypotonic buffer for harvest of membranes and immunoblotting as described above.

Whole-genome sequencing and analysis

The parental KC5, C3h-KO transfectant, and the selected KO-PGIM P. falciparum clones were sequenced using the PacBio SMRT Sequel II Cell with standard PacBio protocol. The samples yielded 259,683–390,238 ccs reads each, with mean read lengths of 10.9-11.8 kb and mean read qualities of QV29.7 to QV30.3. CCS reads were mapped to the PF3D7 reference genome (GCA_000002765) using pbmm2 v1.16.0 (https://github.com/PacificBiosciences/pbmm2), and resulting BAM files underwent INDEL realignment using GATK v3.8-1 [67]. Variant calling was then performed using the HaplotypeCaller from GATK v4.1.9.0 followed by joint genotyping. Resulting raw variants were then filtered with SNPs and INDELs less than 2 base pairs in length filtered at QD < 2.0 and INDELs ≥ 2 base pairs filtered at QD < 5.0, as described [68]. Variants with < 0.75 frequency in each sample were removed to minimize mapping artifacts and exclude low-quality regions or variant positions with high clonal diversity. Highly clustered variants that presumably represent mismapped, problematic regions were visually confirmed as artifacts before exclusion from downstream analysis. Structural variant calling was performed using pbsv v2.9.0 (https://github.com/PacificBiosciences/pbsv); structural variants were annotated using the PF3D7 annotation (GCA_000002765) and VEP release 111 [69]. The raw sequencing data generated for this study have been deposited in the NCBI Sequence Read Archive (SRA) under BioProject accession PRJNA1327946.

Quantitative PCR for gene copy number

Genomic DNA was isolated from cultured parasites and used for clag gene copy number determination after assessing quality and concentration by NanoDrop (Thermo Fisher Scientific). Gene-specific primers (S1 Table) were used in dye-based qPCR (Luna Universal qPCR Master Mix, New England Biolabs) with amplification tracked in a real-time thermal cycler (Biorad CFX96). Ct values from three replicates were averaged and normalized to zero for alpha tubulin 1 (PF3D7_0903700). Copy number was estimated using the 2-ΔΔCT method from four independent DNA harvests.

Quantitative reverse transcriptase PCR

Gene expression was measured with real-time PCR using total RNA harvested from tightly synchronized cultures. Cultures were synchronized with two sorbitol treatments separated by 6 h. Serial smears were then used to obtain matched, schizont-stage infected cells, which were then further synchronized with percoll-sorbitol enrichment before freezing in TRIzol reagent. Total RNA was isolated using Direct-zol RNA MiniPrep kit (Zymo Research) according to the manufacturer’s protocol. Isolated total RNA (800 ng) was annealed with 250 ng random hexamer primer, heated to 65 °C for five minutes and slowly cooled. First strand cDNA was synthesized with SuperScript IV Reverse Transcriptase (ThermoFisher) according to the manufacture’s protocol. The resulting cDNA was diluted 10-fold and used for qRT-PCR (QuantiTect SYBR Green, Qiagen), as described previously [18]. Primers were designed to yield specific ~120 bp amplicons for indicated genes and are listed in S1 Table. qRT-PCR was carried out using the iCycler IQ multicolor real-time PCR system (Bio-Rad) programmed for denaturation at 95˚C for 15 min followed by 40 cycles of annealing at 52 °C and extension at 62˚C for 30 s each.

Gene expression was quantified using the 2-ΔΔCT method [70], with α-tubulin 1 (PF3D7_0903700) as a constitutively expressed loading control; msp2 was included as a stage-specific control as its transcription matches the preferential expression of clag and rhoph genes at the mature schizont stage. Normalized expression is also reported by comparison to matched trials using RNA from wild-type KC5. All reactions were performed in triplicate and are presented as the mean ± S.E.M. of results from 3-4 independent RNA harvests for each transfectant or selected mutant.

DNA transfection

CRISPR/Cas9 transfection was used to produce engineered lines that express CLAG2 with a C-terminal NanoLuc tag. A previously generated pL7 plasmid for epitope tagging CLAG2 with a high-scoring sgRNA, 5’- ACATACTAGTAATATCCAAA-3’, was modified using InFusion cloning (Clontech) to introduce a full-length NanoLuc tag after an unmodified CLAG2 protein with a two-residue linker (Bgl11 restriction site). A bsd selection marker cassette was also cloned into the plasmid and verified by sequencing. Cas9 was expressed from a separate pUF1-Cas9 plasmid. After transfection of KC5, C3h-KO, and KO-PGIM, cultures were selected with 2.5 µg/mL blasticidin S and 1.5 µM DSM-1 (5-methyl[1,2, 4]triazolo[1,5-a]pyrimidin-7-yl)naphthalen-2-ylamine). KO-PGIM was cultivated in PGIM throughout the transfection process. After parasite outgrowth and PCR confirmation of integration, limiting dilution cloning was performed for all transfectant lines without further exposure to blasticidin S. All experiments were performed with sequence-verified clones.

Indirect Immunofluorescence microscopy

Indirect immunofluorescence assays (IFA) were performed using freshly prepared thin blood smears after fixation with 1:1 acetone: methanol at -20 °C. After air drying, slides were blocked with 3% BSA in PBS for 1 h at RT and incubated with primary antibody in blocking buffer (rabbit anti-RhopH3 at 1:1000; mouse anti-NanoLuc antibody at 1:100, Promega) for 3 h at RT under a coverslip. After two washes, secondary antibodies (Alexa Fluor 488-conjugated goat anti-rabbit at 1:500, Invitrogen; Alexa Fluor 594-conjugated goat anti-mouse at 1:500, Invitrogen) with 1 μg/mL 4’,6-diamidino-2-phenylindole (DAPI; Genetex) was added in blocking buffer and incubated for 1 h at RT. After washes, slides were dried and mounted using ProLong Diamond Antifade Mountant (Molecular Probes). Images were collected on a Leica SP8 microscope using a 63x oil immersion objective. DAPI, Alexa Fluor 488, and Alexa Fluor 594 fluorescence were captured using excitation/emission wavelengths of 377/447 nm, 499/520 nm, and 590/618 nm, respectively. Images were processed using Leica LAS X and Huygens Essential software.

Statistical analysis

Numerical data are shown as mean ± S.E.M of independent trials, as reported. Statistical significance was calculated using unpaired Student’s t-test or one-way ANOVA with post-hoc testing as appropriate. Significance was accepted at P < 0.05.

Supporting information

S1 Fig. Rare C3h-KO parasites seen during PGIM cultivation resume expansion upon transfer to nutrient-rich medium.

A) C3h-KO expansion after cultivation in PGIM for 0, 2, 4, 6, or 8 days prior to return to RPMI 1640-based medium (left to right curves; symbols represent mean of 3 trials). Increasing the duration of PGIM exposure does not extend the lag before resumed growth. B) Time to 2% parasitemia after return to RPMI 1640-based medium for C3h-KO cultures seeded in PGIM for indicated number of days. Symbols represent mean ± S.E.M. estimated by linear interpolation of daily parasitemia estimates from microscopic observation; n = 3 trials each. Recovery time does not increase with extended PGIM exposure, indicating that these parasites remain viable.

https://doi.org/10.1371/journal.ppat.1013321.s001

(TIF)

S2 Fig. Transcript abundances for clag and rhoph genes.

Mean ± S.E.M. transcription of indicated clag and rhoph genes in KC5, C3h-KO, KO-PGIM, and KO-rev parasites (black, red, cyan, and dark red bars in each group, respectively), calculated as 2(-ΔCt) using ΔCt relative to the α-tubulin loading control. msp2, unrelated gene with similar stage-specific expression. Values reflect the RT-qPCR experiments shown in Fig 5A without normalization to the wild-type control.

https://doi.org/10.1371/journal.ppat.1013321.s002

(TIF)

S3 Fig. Engineered parasites carrying a NanoLuc reporter at CLAG2 C-terminus.

A) Ethidium-stained gels using indicated primers and DNA from transfectant clones and the wild-type KC5 parent. Primer pair p8-p9 is specific for the wild-type clag2 locus while other pairs yield amplicons upon integration. Loss of the p8-p9 amplicon in KC5C2NLuc, C3h-KOC2NLuc, and KO-PGIMC2NLuc indicates complete replacement of all genomic clag2 copies with the integration cassette, which adds a C-terminal NanoLuc reporter. Expected sizes (in bp): p8-p9, 605; p8-p10, 619; p8-p11, 1027; p8-p12, 1465; p8-p13, 1975 in transfectant lines and 1066 in wild-type KC5. Primer sequences are in S1 Table. B) Indirect immunofluorescence confocal microscopy images of a trophozoite-stage KO-PGIMC2NLuc parasite probed with anti-RhopH3 and anti-NanoLuc antibodies (green and red, respectively). Scale bar, 5 µm. The NanoLuc-tagged CLAG2 protein is delivered to infected cells after invasion and is exported into host cytosol [24].

https://doi.org/10.1371/journal.ppat.1013321.s003

(TIF)

S4 Fig. Increased CLAG2 production in KO-PGIM is detected by a weakly cross-reactive anti-CLAG3 antibody.

A) Anti-CLAG3 immunoblot using total membranes from indicated parasites. Samples used percoll-sorbitol enriched infected cells and were match-loaded. A low-intensity band is detected in KO-PGIM lysates but absent in the unselected C3h-KO parent. B) Sequence alignment of KC5 CLAG2 sequence with the recombinant epitope used to produce anti-CLAG3 antibody. Identical residues are highlighted in red; the ruler is numbered according to CLAG2. As the band detected in KO-PGIM reflects cross-reaction with the CLAG3 C-terminal epitope, we did not attempt to quantify band intensities. C) Ethidium-stained gels showing unaltered detection of clag genes in KO-PGIM when compared to the wild-type KC5 line. PCR of clag8 was performed in two fragments to facilitate specific detection. Ribbon schematic at top shows the sites recognized by each primer; primer sequences are in S1 Table. D) Gels showing absence of ectopic recombination between clag3 and other paralogs in either KC5 or KO-PGIM.

https://doi.org/10.1371/journal.ppat.1013321.s004

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S1 Table. Primers used in this study.

https://doi.org/10.1371/journal.ppat.1013321.s005

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S2 Table. Structural variants in KO-PGIM.

Structural variants from whole-genome sequencing filtered for variants that differ between C3h-KO and KO-PGIM. The two filtered variants are tabulated with the impacted genes, chromosomal location, structural length, mutant allele, genotypes, and flanking sequencing depth.

https://doi.org/10.1371/journal.ppat.1013321.s006

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S3 Table. Mutations and indels in C3h-KO and KO-PGIM.

Variants identified from whole-genome sequencing of parental and mutant strains and mapped to the 3D7 reference strain. Following initial quality filtering outlined in the Methods, variants were filtered that did not differ between the 3 strains. The KC5, C3h-KO, and KO-PGIM genotypes are reported as 0 when identical to the reference and 1 when a mutant allele was called. The VAR column reflects the number of parasites that differed from 3D7 at the indicated position. Columns with.DP and.GT suffixes indicate read depth and the primary allele for each parasite, respectively. Blue highlighted rows indicate high-confidence mutations in KO-PGIM relative to C3h-KO; green highlights reflect those in C3h-KO relative to wild-type KC5.

https://doi.org/10.1371/journal.ppat.1013321.s007

(XLSX)

Acknowledgments

We thank BEI Resources for DSM-1 and Anna Crater for intellectual and technical input during early stages of these studies.

References

  1. 1. Cowman AF, Tonkin CJ, Tham W-H, Duraisingh MT. The Molecular Basis of Erythrocyte Invasion by Malaria Parasites. Cell Host Microbe. 2017;22(2):232–45. pmid:28799908
  2. 2. Cooke BM, Stuart J, Nash GB. The cellular and molecular rheology of malaria. Biorheology. 2014;51(2–3):99–119. pmid:24819866
  3. 3. Lee W-C, Russell B, Rénia L. Sticking for a Cause: The Falciparum Malaria Parasites Cytoadherence Paradigm. Front Immunol. 2019;10:1444. pmid:31316507
  4. 4. Desai SA. Why do malaria parasites increase host erythrocyte permeability? Trends Parasitol. 2014;30(3):151–9. pmid:24507014
  5. 5. Long CA, Zavala F. Immune Responses in Malaria. Cold Spring Harb Perspect Med. 2017;7(8):a025577. pmid:28389518
  6. 6. Arora G, Hart GT, Manzella-Lapeira J, Doritchamou JY, Narum DL, Thomas LM, et al. NK cells inhibit Plasmodium falciparum growth in red blood cells via antibody-dependent cellular cytotoxicity. Elife. 2018;7:e36806. pmid:29943728
  7. 7. Kurup SP, Butler NS, Harty JT. T cell-mediated immunity to malaria. Nat Rev Immunol. 2019;19(7):457–71. pmid:30940932
  8. 8. Deitsch KW, Dzikowski R. Variant Gene Expression and Antigenic Variation by Malaria Parasites. Annu Rev Microbiol. 2017;71:625–41. pmid:28697665
  9. 9. Saito F, Hirayasu K, Satoh T, Wang CW, Lusingu J, Arimori T, et al. Immune evasion of Plasmodium falciparum by RIFIN via inhibitory receptors. Nature. 2017;552(7683):101–5. pmid:29186116
  10. 10. Nguitragool W, Bokhari AAB, Pillai AD, Rayavara K, Sharma P, Turpin B, et al. Malaria parasite clag3 genes determine channel-mediated nutrient uptake by infected red blood cells. Cell. 2011;145(5):665–77. pmid:21620134
  11. 11. Mira-Martínez S, Rovira-Graells N, Crowley VM, Altenhofen LM, Llinás M, Cortés A. Epigenetic switches in clag3 genes mediate blasticidin S resistance in malaria parasites. Cell Microbiol. 2013;15(11):1913–23. pmid:23819786
  12. 12. Sharma P, Wollenberg K, Sellers M, Zainabadi K, Galinsky K, Moss E, et al. An epigenetic antimalarial resistance mechanism involving parasite genes linked to nutrient uptake. J Biol Chem. 2013;288(27):19429–40. pmid:23720749
  13. 13. Mira-Martínez S, Pickford AK, Rovira-Graells N, Guetens P, Tintó-Font E, Cortés A, et al. Identification of Antimalarial Compounds That Require CLAG3 for Their Uptake by Plasmodium falciparum-Infected Erythrocytes. Antimicrob Agents Chemother. 2019;63(5):e00052-19. pmid:30782998
  14. 14. Trickey ML, Chowdury M, Bramwell G, Counihan NA, de Koning-Ward TF. Utilisation of an in vivo malaria model to provide functional proof for RhopH1/CLAG essentiality and conserved orthology with P. falciparum. J Biomed Sci. 2025;32(1):13. pmid:39894870
  15. 15. Cortés A, Carret C, Kaneko O, Yim Lim BYS, Ivens A, Holder AA. Epigenetic silencing of Plasmodium falciparum genes linked to erythrocyte invasion. PLoS Pathog. 2007;3(8):e107. pmid:17676953
  16. 16. Pillai AD, Nguitragool W, Lyko B, Dolinta K, Butler MM, Nguyen ST, et al. Solute restriction reveals an essential role for clag3-associated channels in malaria parasite nutrient acquisition. Mol Pharmacol. 2012;82(6):1104–14. pmid:22949525
  17. 17. Mira-Martínez S, van Schuppen E, Amambua-Ngwa A, Bottieau E, Affara M, Van Esbroeck M, et al. Expression of the Plasmodium falciparum Clonally Variant clag3 Genes in Human Infections. J Infect Dis. 2017;215(6):938–45. pmid:28419281
  18. 18. Gupta A, Bokhari AAB, Pillai AD, Crater AK, Gezelle J, Saggu G, et al. Complex nutrient channel phenotypes despite Mendelian inheritance in a Plasmodium falciparum genetic cross. PLoS Pathog. 2020;16(2):e1008363. pmid:32069335
  19. 19. Vincensini L, Fall G, Berry L, Blisnick T, Braun Breton C. The RhopH complex is transferred to the host cell cytoplasm following red blood cell invasion by Plasmodium falciparum. Mol Biochem Parasitol. 2008;160(2):81–9. pmid:18508137
  20. 20. Gupta A, Gonzalez-Chavez Z, Desai SA. Plasmodium falciparum CLAG Paralogs All Traffic to the Host Membrane but Knockouts Have Distinct Phenotypes. Microorganisms. 2024;12(6):1172. pmid:38930554
  21. 21. Trenholme KR, Gardiner DL, Holt DC, Thomas EA, Cowman AF, Kemp DJ. clag9: A cytoadherence gene in Plasmodium falciparum essential for binding of parasitized erythrocytes to CD36. Proc Natl Acad Sci U S A. 2000;97(8):4029–33. pmid:10737759
  22. 22. Goel S, Valiyaveettil M, Achur RN, Goyal A, Mattei D, Salanti A, et al. Dual stage synthesis and crucial role of cytoadherence-linked asexual gene 9 in the surface expression of malaria parasite var proteins. Proc Natl Acad Sci U S A. 2010;107(38):16643–8. pmid:20823248
  23. 23. Nacer A, Roux E, Pomel S, Scheidig-Benatar C, Sakamoto H, Lafont F, et al. Clag9 is not essential for PfEMP1 surface expression in non-cytoadherent Plasmodium falciparum parasites with a chromosome 9 deletion. PLoS One. 2011;6(12):e29039. pmid:22205992
  24. 24. Ito D, Schureck MA, Desai SA. An essential dual-function complex mediates erythrocyte invasion and channel-mediated nutrient uptake in malaria parasites. Elife. 2017;6:e23485. pmid:28221136
  25. 25. Iriko H, Kaneko O, Otsuki H, Tsuboi T, Su X-Z, Tanabe K, et al. Diversity and evolution of the rhoph1/clag multigene family of Plasmodium falciparum. Mol Biochem Parasitol. 2008;158(1):11–21. pmid:18155305
  26. 26. Ginsburg H, Kutner S, Krugliak M, Cabantchik ZI. Characterization of permeation pathways appearing in the host membrane of Plasmodium falciparum infected red blood cells. Mol Biochem Parasitol. 1985;14(3):313–22. pmid:3887158
  27. 27. Liu J, Istvan ES, Gluzman IY, Gross J, Goldberg DE. Plasmodium falciparum ensures its amino acid supply with multiple acquisition pathways and redundant proteolytic enzyme systems. Proc Natl Acad Sci U S A. 2006;103(23):8840–5. pmid:16731623
  28. 28. Alkhalil A, Cohn JV, Wagner MA, Cabrera JS, Rajapandi T, Desai SA. Plasmodium falciparum likely encodes the principal anion channel on infected human erythrocytes. Blood. 2004;104(13):4279–86. pmid:15319279
  29. 29. Wagner MA, Andemariam B, Desai SA. A two-compartment model of osmotic lysis in Plasmodium falciparum-infected erythrocytes. Biophys J. 2003;84(1):116–23. pmid:12524269
  30. 30. Bokhari AAB, Solomon T, Desai SA. Two distinct mechanisms of transport through the plasmodial surface anion channel. J Membr Biol. 2008;226(1–3):27–34. pmid:19050955
  31. 31. Nakazawa S, Kanbara H, Aikawa M. Plasmodium falciparum: recrudescence of parasites in culture. Exp Parasitol. 1995;81(4):556–63. pmid:8542997
  32. 32. Codd A, Teuscher F, Kyle DE, Cheng Q, Gatton ML. Artemisinin-induced parasite dormancy: a plausible mechanism for treatment failure. Malar J. 2011;10:56. pmid:21385409
  33. 33. Butler MM, Waidyarachchi SL, Shao J, Nguyen ST, Ding X, Cardinale SC, et al. Optimized Pyridazinone Nutrient Channel Inhibitors Are Potent and Specific Antimalarial Leads. Mol Pharmacol. 2022;102(3):172–82. pmid:35798366
  34. 34. Lisk G, Scott S, Solomon T, Pillai AD, Desai SA. Solute-inhibitor interactions in the plasmodial surface anion channel reveal complexities in the transport process. Mol Pharmacol. 2007;71(5):1241–50. pmid:17287402
  35. 35. Baumeister S, Winterberg M, Duranton C, Huber SM, Lang F, Kirk K, et al. Evidence for the involvement of Plasmodium falciparum proteins in the formation of new permeability pathways in the erythrocyte membrane. Mol Microbiol. 2006;60(2):493–504. pmid:16573697
  36. 36. Nguitragool W, Rayavara K, Desai SA. Proteolysis at a specific extracellular residue implicates integral membrane CLAG3 in malaria parasite nutrient channels. PLoS One. 2014;9(4):e93759. pmid:24699906
  37. 37. Scarpa A, Cecchetto A, Azzone GF. Permeability of erythrocytes to anions and the regulation of cell volume. Nature. 1968;219(5153):529–31. pmid:5668450
  38. 38. Desai SA, Bezrukov SM, Zimmerberg J. A voltage-dependent channel involved in nutrient uptake by red blood cells infected with the malaria parasite. Nature. 2000;406(6799):1001–5. pmid:10984055
  39. 39. Alkhalil A, Hong L, Nguitragool W, Desai SA. Voltage-dependent inactivation of the plasmodial surface anion channel via a cleavable cytoplasmic component. Biochim Biophys Acta. 2012;1818(3):367–74. pmid:22115742
  40. 40. Schwinn MK, Steffen LS, Zimmerman K, Wood KV, Machleidt T. A Simple and Scalable Strategy for Analysis of Endogenous Protein Dynamics. Sci Rep. 2020;10(1):8953. pmid:32488146
  41. 41. Freitas-Junior LH, Bottius E, Pirrit LA, Deitsch KW, Scheidig C, Guinet F, et al. Frequent ectopic recombination of virulence factor genes in telomeric chromosome clusters of P. falciparum. Nature. 2000;407(6807):1018–22. pmid:11069183
  42. 42. Cortés A, Deitsch KW. Malaria Epigenetics. Cold Spring Harb Perspect Med. 2017;7(7):a025528. pmid:28320828
  43. 43. Voss TS, Bozdech Z, Bártfai R. Epigenetic memory takes center stage in the survival strategy of malaria parasites. Curr Opin Microbiol. 2014;20:88–95. pmid:24945736
  44. 44. Smith JD, Rowe JA, Higgins MK, Lavstsen T. Malaria’s deadly grip: cytoadhesion of Plasmodium falciparum-infected erythrocytes. Cell Microbiol. 2013;15(12):1976–83. pmid:23957661
  45. 45. Chamberlain SG, Iwanaga S, Higgins MK. Immune evasion runs in the family: two surface protein families of Plasmodium falciparum-infected erythrocytes. Curr Opin Microbiol. 2025;85:102598. pmid:40112571
  46. 46. Fried M, Duffy PE. Designing a VAR2CSA-based vaccine to prevent placental malaria. Vaccine. 2015;33(52):7483–8. pmid:26469717
  47. 47. Sethumadhavan DV, Tiburcio M, Kanyal A, Jabeena CA, Govindaraju G, Karmodiya K, et al. Chromodomain Protein Interacts with H3K9me3 and Controls RBC Rosette Formation by Regulating the Expression of a Subset of RIFINs in the Malaria Parasite. J Mol Biol. 2022;434(12):167601. pmid:35460670
  48. 48. Claessens A, Hamilton WL, Kekre M, Otto TD, Faizullabhoy A, Rayner JC, et al. Generation of antigenic diversity in Plasmodium falciparum by structured rearrangement of Var genes during mitosis. PLoS Genet. 2014;10(12):e1004812. pmid:25521112
  49. 49. Scherf A, Figueiredo LM, Freitas-Junior LH. Plasmodium telomeres: a pathogen’s perspective. Curr Opin Microbiol. 2001;4(4):409–14. pmid:11495803
  50. 50. Calhoun SF, Reed J, Alexander N, Mason CE, Deitsch KW, Kirkman LA. Chromosome End Repair and Genome Stability in Plasmodium falciparum. mBio. 2017;8(4):e00547-17. pmid:28790200
  51. 51. Simam J, Rono M, Ngoi J, Nyonda M, Mok S, Marsh K, et al. Gene copy number variation in natural populations of Plasmodium falciparum in Eastern Africa. BMC Genomics. 2018;19(1):372. pmid:29783949
  52. 52. Price RN, Uhlemann A-C, Brockman A, McGready R, Ashley E, Phaipun L, et al. Mefloquine resistance in Plasmodium falciparum and increased pfmdr1 gene copy number. Lancet. 2004;364(9432):438–47. pmid:15288742
  53. 53. Cowman AF, Galatis D, Thompson JK. Selection for mefloquine resistance in Plasmodium falciparum is linked to amplification of the pfmdr1 gene and cross-resistance to halofantrine and quinine. Proc Natl Acad Sci U S A. 1994;91(3):1143–7. pmid:8302844
  54. 54. Preechapornkul P, Imwong M, Chotivanich K, Pongtavornpinyo W, Dondorp AM, Day NPJ, et al. Plasmodium falciparum pfmdr1 amplification, mefloquine resistance, and parasite fitness. Antimicrob Agents Chemother. 2009;53(4):1509–15. pmid:19164150
  55. 55. Kidgell C, Volkman SK, Daily J, Borevitz JO, Plouffe D, Zhou Y, et al. A systematic map of genetic variation in Plasmodium falciparum. PLoS Pathog. 2006;2(6):e57. pmid:16789840
  56. 56. Cheeseman IH, Miller B, Tan JC, Tan A, Nair S, Nkhoma SC, et al. Population Structure Shapes Copy Number Variation in Malaria Parasites. Mol Biol Evol. 2016;33(3):603–20. pmid:26613787
  57. 57. Ross AF, Green WN, Hartman DS, Claudio T. Efficiency of acetylcholine receptor subunit assembly and its regulation by cAMP. J Cell Biol. 1991;113(3):623–36. pmid:1849906
  58. 58. Kaneko O, Yim Lim BYS, Iriko H, Ling IT, Otsuki H, Grainger M, et al. Apical expression of three RhopH1/Clag proteins as components of the Plasmodium falciparum RhopH complex. Mol Biochem Parasitol. 2005;143(1):20–8. pmid:15953647
  59. 59. Gupta A, Thiruvengadam G, Desai SA. The conserved clag multigene family of malaria parasites: essential roles in host-pathogen interaction. Drug Resist Updat. 2015;18:47–54. pmid:25467627
  60. 60. Otto TD, Böhme U, Sanders M, Reid A, Bruske EI, Duffy CW, et al. Long read assemblies of geographically dispersed Plasmodium falciparum isolates reveal highly structured subtelomeres. Wellcome Open Res. 2018;3:52. pmid:29862326
  61. 61. Desai SA. Epigenetics of malaria parasite nutrient uptake, but why? Trends Parasitol. 2022;38(8):618–28. pmid:35641406
  62. 62. Hadjimichael E, Deitsch KW. Variable surface antigen expression, virulence, and persistent infection by Plasmodium falciparum malaria parasites. Microbiol Mol Biol Rev. 2025;89(1):e0011423. pmid:39807932
  63. 63. Amambua-Ngwa A, Button-Simons KA, Li X, Kumar S, Brenneman KV, Ferrari M, et al. Chloroquine resistance evolution in Plasmodium falciparum is mediated by the putative amino acid transporter AAT1. Nat Microbiol. 2023;8(7):1213–26. pmid:37169919
  64. 64. Cohn JV, Alkhalil A, Wagner MA, Rajapandi T, Desai SA. Extracellular lysines on the plasmodial surface anion channel involved in Na+ exclusion. Mol Biochem Parasitol. 2003;132(1):27–34. pmid:14563534
  65. 65. Pillai AD, Addo R, Sharma P, Nguitragool W, Srinivasan P, Desai SA. Malaria parasites tolerate a broad range of ionic environments and do not require host cation remodelling. Mol Microbiol. 2013;88(1):20–34. pmid:23347042
  66. 66. Hill DA, Pillai AD, Nawaz F, Hayton K, Doan L, Lisk G, et al. A blasticidin S-resistant Plasmodium falciparum mutant with a defective plasmodial surface anion channel. Proc Natl Acad Sci U S A. 2007;104(3):1063–8. pmid:17213308
  67. 67. Van der Auwera GA, O’Connor BD. Genomics in the Cloud: Using Docker, GATK, and WDL in Terra. O’Reilly Media; 2020.
    • 68. Wagner J, Olson ND, Harris L, Khan Z, Farek J, Mahmoud M, et al. Benchmarking challenging small variants with linked and long reads. Cell Genom. 2022;2(5):100128. pmid:36452119
    • 69. McLaren W, Gil L, Hunt SE, Riat HS, Ritchie GRS, Thormann A, et al. The Ensembl Variant Effect Predictor. Genome Biol. 2016;17(1):122. pmid:27268795
    • 70. Livak KJ, Schmittgen TD. Analysis of relative gene expression data using real-time quantitative PCR and the 2(-Delta Delta C(T)) Method. Methods. 2001;25(4):402–8. pmid:11846609