Research Articles:

Microbial Cell, Vol. 3, No. 5, pp. 215 - 223; doi: 10.15698/mic2016.05.500

Optogenetic monitoring identifies phosphatidylthreonine-regulated calcium homeostasis in Toxoplasma gondii

Arunakar Kuchipudi1, Ruben D. Arroyo-Olarte1, Friederike Hoffmann1, Volker Brinkmann2, Nishith

Gupta1, 2

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    1 Humboldt University, Berlin, Germany.

    2 Max-Planck Institute for Infection Biology, Berlin, Germany.

Keywords: Toxoplasma gondii, phosphatidylthreonine, optogenetics, gene-encoded calcium indicator, lytic cycle, intracellular parasite, calcium homeostasis.


CaM – calmodulin,

CpEGFP - circularly-permuted enhanced green fluorescent protein,

EGFP - enhanced green fluorescent protein,

FUDR - 5-fluorodeoxyuridine,

GECI - gene-encoded calcium indicator,

HFF - human foreskin fibroblasts,

IP3 - inositol tri-phosphate,

MOI - multiplicity of infection,

PBS – phosphate buffered saline,

PLC - phospholipase C,

PtdThr – phosphatidylthreonine,

PTS - phosphatidylthreonine synthase,

UPRT – uracil phosphoribosyltransferase.
Received originally: 22/12/2015 Received in revised form: 22/03/2016
Accepted: 06/04/2016 Published: 02/05/2016

Nishith Gupta, PhD, Department of Molecular Parasitology, Humboldt University, Philippstrasse 13, House 14, Berlin, Germany; Telephone: +49-30-20936404; Fax: +49-30-20936051

Conflict of interest statement: The authors declare that there are no conflicts of interest pertaining to this work.
Please cite this article as: Arunakar Kuchipudi, Ruben Dario Arroyo-Olarte, Friederike Hoffmann, Volker Brinkmann, Nishith Gupta (2016). Optogenetic monitoring identifies phosphatidylthreonine-regulated calcium homeostasis in Toxoplasma gondii. Microbial Cell 3(5): 215-223.


Toxoplasma gondii is an obligate intracellular parasite, which inflicts acute as well as chronic infections in a wide range of warm-blooded vertebrates. Our recent work has demonstrated the natural occurrence and autonomous synthesis of an exclusive lipid phosphatidylthreonine in T. gondii. Targeted gene disruption of phosphatidylthreonine synthase impairs the parasite virulence due to unforeseen attenuation of the consecutive events of motility, egress and invasion. However, the underlying basis of such an intriguing phenotype in the parasite mutant remains unknown. Using an optogenetic sensor (gene-encoded calcium indicator, GCaMP6s), we show that loss of phosphatidylthreonine depletes calcium stores in intracellular tachyzoites, which leads to dysregulation of calcium release into the cytosol during the egress phase of the mutant. Consistently, the parasite motility and egress phenotypes in the mutant can be entirely restored by ionophore-induced mobilization of calcium. Collectively, our results suggest a novel regulatory function of phosphatidylthreonine in calcium signaling of a prevalent parasitic protist. Moreover, our application of an optogenetic sensor to monitor subcellular calcium in a model intracellular pathogen exemplifies its wider utility to other entwined systems.


Toxoplasma gondii is considered as one of the most successful parasites on Earth, infecting humans as well as a wide range of animals [1]. The parasite causes debilitating opportunistic infections in individuals with inadequate and compromised immunity, such as neonates, HIV-AIDS and organ transplantation patients. Acute disease is due to asexual reproduction of the fast-dividing tachyzoite stage of T. gondii, which undergoes recurring lytic cycles in the target host cells. The lytic cycle of tachyzoites comprises the sequential events of invasion, replication and egress [1]. Our recent work has identified an atypical phospholipid in tachyzoites designated as phosphatidylthreonine (PtdThr) that is crucial for an efficient lytic cycle and virulence [2]. PtdThr is produced by a novel enzyme PtdThr synthase (PTS) located in the endoplasmic reticulum (ER) of the parasite. Surprisingly, the loss of PtdThr in a mutant of lipid synthesis (Δtgpts strain) does not affect membrane biogenesis and intracellular replication but compromises the gliding motility, which in turn blights the downstream events of parasite egress and invasion.

The induction of gliding motility in T. gondii tachyzoites requires a calcium-mediated signaling cascade leading to activation of calcium-dependent kinases and exocytosis of micronemes once the proliferation phase is completed [3][4][5][6][7][8]. The level of calcium in the cytosol is elevated prior to initiation of the parasite egress from dilapidated host cells [9][10]. Given the phenotype of the Δtgpts strain, we postulated a role of PtdThr in governing subcellular calcium homeostasis during the lytic cycle of T. gondii. Calcium-regulated processes in T. gondii occur in an entwined system, comprising the parasite and host cell. While the use of calcium-sensitive fluorophores has proven extremely valuable to examine calcium homeostasis in extracellular stage of apicomplexan parasites [11], similar studies during intracellular development are rather limited [12][13]. Specific real-time monitoring of subcellular calcium has become more feasible using optogenetic sensors, which have aided detection of calcium in specific cell types, populations or even organelles [14][15][16]. A rich repertoire of gene-encoded calcium indicators (GECI) have been engineered by fusing different types of calcium-binding and regulatory domains with fluorescent proteins to meet the desired specificity, sensitivity, signal-to-noise ratio and temporal scale [14][15][16]. For instance, GCaMP6 family proteins consist of a myosin light chain kinase domain (M13) conjugated to a circularly permuted enhanced GFP (CpEGFP) and calmodulin (CaM) [14]. A rise in calcium induces conformational change in the CaM domain, which in turn activates the M13 kinase domain to block a hole in the CpEGFP barrel exposing the otherwise quenched chromophore [17]. This work deployed a member of GCaMP6 family, GCaMP6s, to discern the functional importance of PtdThr by examining the calcium dynamics in intracellular tachyzoites.


GCaMP6s localizes in the parasite cytosol.

To determine the calcium oscillation in intracellular tachyzoites, we deployed a gene-encoded calcium indicator GCaMP6s, which was originally designed to image the neuronal activity [14]. We generated the parental and PTS-knockout strains stably expressing the GCaMP6s fusion protein, which consists of a M13 kinase peptide, a CpEGFP barrel and a calcium-sensitive calmodulin (Fig. 1A). Transgenic parasites were subjected to immunofluorescence assays to examine the subcellular location and relative expression of GCaMP6s in the two strains (Fig. 1A). GCaMP6s signal was confined within the parasite periphery, as shown by co-staining of EGFP domain with the TgGap45 protein located in the inner membrane complex [18]. Co-localization of the EGFP domain with a cytosolic marker TgHsp90 [19] revealed an apparently uniform distribution of GCaMP6s in the parasite cytosol. Immunoblot analysis demonstrated the expression of a protein band with an apparent molecular weight of about 55 kDa (Fig. 1B), which confirmed the physical integrity of GCaMP6s fusion protein in both strains. Taken together, these data provided the initial basis to monitor cytosolic calcium in tachyzoites.

Figure 1 PtdThr-regulated calcium homeostasis in Toxoplasma gondii

FIGURE 1: GCaMP6s is expressed in the cytosol of intracellular tachyzoites. (A) Images illustrating co-staining of EGFP (GCaMP6s) with the markers for cytosol (TgHsp90) or inner membrane complex (TgGap45). Stable transgenic parasites of the parental (RHΔku80-hxgprt-) and PTS mutant (Δtgpts) strains, expressing GCaMP6s under the control of the TgGRA1 promoter, were generated by negative selection with FUDR (targeting the UPRT locus). Intracellular tachyzoites (MOI, 1; 24 h infection) were imaged following the immunofluorescence assay using the indicated antibodies. No cross-fluorescence (bleeding effect) was observed across the two color channels. (B) A representative immunoblot confirming the expression of intact M13-CpEGFP-CaM fusion protein (a.k.a. GCaMP6s or GECI) in the parental and PTS knockout strains. TgHsp90 was used as the loading control.

Expression of GCaMP6s is not detrimental to the parasite growth and replication.

Next, we determined the impact of GCaMP6s expression on the parasite growth by plaque assays, which signify consecutive lytic cycle of tachyzoites in host cells (Fig. 2A). As reported previously [2], the Δtgpts mutant displayed a considerably reduced plaque numbers and area compared to the parental strain (Fig. 2B). More importantly, expression of GECI did not exert an apparent negative impact on the growth of either of the GCaMP6s-transgenic strains when compared to their corresponding reference (non-GECI) strains. To reinforce these data, we measured intracellular replication of the indicated strains by scoring the number of tachyzoites per vacuole throughout the lytic cycle. The replication rates of respective GCaMP6s-transgenic strains were comparable during the entire proliferation phase (Fig. 2C). Collectively, these results excluded a detrimental effect of GECI for tachyzoite growth and enabled the study of calcium dynamics during the intracellular development of the two strains.

Figure 2 PtdThr-regulated calcium homeostasis in Toxoplasma gondii

FIGURE 2: In vitro growth and replication rates of GCaMP6s-expressing parasite strains are comparable to the respective parental strains. (A) Image illustrating the lytic cycle of tachyzoites leading to plaque formation in host-cell monolayers. (B) Growth fitness of the specified strains, as measured by plaque assays. In total, 100-200 plaques of each strain were evaluated for their sizes and numbers using ImageJ suite. (C) Replication rates of the GCaMP6s-expressing strains. Intracellular tachyzoites proliferating in their vacuoles were immunostained with αTgGap45 antibody at the indicated time points. The average number of tachyzoites/vacuole was used to calculate parasite doublings (Example: 1 doubling = 2 parasites/vacuole, and 5 doublings = 32 parasites/vacuole). Graphs depict the mean ± SEM from 3 assays (student’s t-test, *p<0.05, ***p<0.001).

GCaMP6s fluorescence is increased during parasite egress.

Having established the relative expression and growth parameters of the GCaMP6s-transgenic strains, we next examined the functionality of GCaMP6s in tachyzoites. As illustrated in Fig. 3A, tachyzoites egressing at the end of lytic cycle exhibit induced cytosolic calcium levels, which exert conformational changes in EGFP, leading to increased fluorescence. To examine the modulation of GCaMP6s activity during natural egress, we monitored EGFP signal in tachyzoites nearing the end of lytic cycle. Certainly, as anticipated, parasites exiting from dilapidated human host cells displayed an intense EGFP signal, whereas fluorescence in the immature vacuoles was notably lower (Fig. 3B). We endorsed these results by time-lapse microscopy of the parasite vacuoles exposed to an ionophore A23187 (Fig. 3C), which is known to induce calcium influx and consequently the premature egress of intracellular tachyzoites [3][20][21][22]. As expected, tachyzoites within vacuoles displayed basal level of fluorescence prior to ionophore treatment (0 min). EGFP signal increased rapidly within a minute of drug exposure and saturated gradually over a period of 10 min. Together with aforesaid assays, these data firmly established the utility of GECI to measure and compare the cytosolic calcium levels in intracellular parasites of the parental and mutant strains. The method also offered other desired benefits, including spatiotemporal detection, high signal/noise ratio, genetic inheritability to the progeny and uniformity of calcium-dependent GCaMP6s signal across the parasite population in parasitized cultures.

Figure 3 PtdThr-regulated calcium homeostasis in Toxoplasma gondii

FIGURE 3: GCaMP6s activity in intracellular parasites is induced by natural egress and ionophore. (A) Schematics depicting a rise in cytosolic calcium prior to and/or during egress phase, and detection of calcium by GCaMP6s expressed in the parasite cytosol. The effect of external calcium sources is not illustrated here. (B) GCaMP6s fluorescence in response to the natural egress. Parasitized cells infected with GECI-transgenic parental strain (MOI, 3; 44 h infection) was subjected to EGFP imaging. Image shows intensified EGFP fluorescence during egress (arrow) and background signal in the intact/immature vacuoles (arrowheads). (C) Monitoring of GCaMP6s signal in the parasite cultures treated with ionophore (5 µM A23187). Host cells infected with the parental strain were imaged for 10 min using time-lapse microscopy. Ionophore was added after 1 min of imaging. Still images (snapshots), each with about 2 min intervals, are shown.

The Δtgpts mutant shows a compromised calcium flux during the parasite egress.

To investigate calcium homeostasis in the PTS mutant, we employed an automated microplate-based monitoring of EGFP fluorescence. The assay was set up to quantify the realtime levels of cytosolic signal in intracellular tachyzoites of the parental and Δtgpts strains expressing GCaMP6s (Fig. 4A). We observed a comparable level of cytosolic fluorescence during the entire replication phase of the parental and mutant strains, which confirmed a very similar functional activity of GCaMP6s in both strains. The calcium-dependent EGFP fluorescence was progressively elevated as they approached the end of their lytic cycles (42-50 h infection, Fig. 4A). Quite noticeably, the Δtgpts mutant showed a significantly diminished EGFP signal compared to the parental strain during the egress period, indicating a defective release of calcium into the parasite cytosol. To strengthen our results, we numerated intracellular parasites in the two strains at three relevant time points corresponding to replication, early and late egress phases (Fig. 4B). The numbers of intracellular parasites in both GCaMP6s strains were nearly identical at all three time points. Consistently, equivalent intensity of EGFP fluorescence during replication phase reflected a similar number of vacuoles in both strains. Last but not least, immunoblots indicated a comparable expression of GCaMP6s in both strains at specified time points (Fig. 4C). In conclusion, these data suggest a defective mobilization of calcium into the cytosol of the PTS mutant.

Figure 4 PtdThr-regulated calcium homeostasis in Toxoplasma gondii

FIGURE 4: The PTS-knockout mutant exhibits a dysregulation of cytosolic calcium during its natural egression but not during the proliferation phase. (A) Quantitation of EGFP-derived fluorescence during replication and egress phases of GECI strains. Human fibroblast cultures were infected with GCaMP6s-transgenic parental or Δtgpts strains. Calcium-induced EGFP intensity was measured in living cultures using a microplate reader. Graphs show the mean ± SEM of 9 assays, each in tripli-cates (student’s t-test, **p< 0.01, ***p<0.001). (B) Replication rates of the parental and mutant strains expressing GECI. Intracellular parasites replicating in their vacuoles were quantified at specified time points (representing replication, early and late egress) after immunostaining with anti-TgGap45 antibody (mean ± SEM, n=3 assays). Consistent with parasite counts, EGFP signal during the replication phase was indistinguishable in the two GCaMP6s-transgenic strains. (C) A representative western blot depicting the expression of M13-CpEGFP-CaM in the two parasite strains. TgHsp90 was used for normalizing the expression of GCaMP6s in each lane.

The Δtgpts mutant exhibits a poor storage of calcium in the parasite.

Calcium in T. gondii is stored primarily in the acidocalcisomes and ER [11] and the latter organelle is a major site of PtdThr synthesis [2]. We therefore presumed a role of PtdThr in regulating the calcium stores in the parasite ER. To confirm the notion, we performed additional assays using modulators of calcium signaling. Ethanol is an agonist of PLC, which regulates the IP3-sensitive calcium stores in the mammalian cells [23] as well as in T. gondii [10][24]. We induced a maximum release of calcium to the parasite cytosol to estimate the total ion pool in the PTS mutant (Fig. 5A). Both, the parental and mutant strains expressing GECI showed equivalent fluorescence in the beginning of assays (0 min), which confirmed a comparable activity of functional GCaMP6s and vacuole numbers in both strains. We then observed a burst of EGFP signal in intracellular tachyzoites within 1 min of chemical exposure that remained constant thereafter. Even at maximal induction, fluorescence in the mutant’s cytosol was significantly less than the parental strain. Surprisingly, we also observed a much lower EGFP activity even after treatment of the Δtgpts strain with ionophore A23187 (Fig. 5B), which should have equilibrated calcium across all membranes given its high concentration in culture medium (~ 1.8 mM). There was a slow but steady increase in signal following the initial surge that was probably due to continued flow of external calcium to the parasite interior. The results indicate that lower cytosolic fluorescence in the PTS mutant is likely caused by impaired storage of calcium in the parasite.

Figure 5 PtdThr-regulated calcium homeostasis in Toxoplasma gondii

FIGURE 5: The Δtgpts strain is deficient in the storage of subcellular calcium. Calcium-induced fluorescence in the two GECI-strains following exposure to 8 % ethanol (A) or to 5 µM A23187 (B) (42 hrs post-infection). Human fibroblasts were infected with transgenic parental or Δtgpts strains. As shown in Fig. 4B, the number of intracellular tachyzoites was equivalent in the two strains. Note that EGFP fluorescence signals just prior to drug exposure (0 min) are nearly equal, indicating a comparable number of vacuoles (and thus GECI activity) in both strains. Graphs show the mean ± SEM from 6 assays (student’s t-test, ***p<0.001).

Induced flux of calcium can repair egress and motility defects in the PTS mutant.

We have previously shown that the Δtgpts mutant lacking PtdThr shows a reversible defect in egress and gliding motility [2]. To confirm whether these defects are indeed a consequence of perturbed calcium homeostasis in the mutant, we monitored the effect of ionophore on the parasite egress and motility. As shown in Fig. 6A, when intracellular Δtgpts mutant was not stimulated with the ionophore, the strain showed a reduced egress compared to the parental strain. Whereas about 20% vacuoles were naturally disrupted in the parental strain, only 8% vacuoles exhibited parasite egress in the mutant 48 hours post-infection. Both strains revealed more than 90% egress and the egress defect in the mutant was no longer evident within 3 min of ionophore stimulation. Our motility assays showed that the motile fraction and trail lengths were markedly reduced in the mutant under control condition and exposure to ionophore significantly increased both parameters to a comparable level in the two strains (Fig. 6B-C). Likewise, caffeine, a pharmacological agonist of IP3/ryanodine-sensitive Ca2+ channels in T. gondii [24][25] also repaired gliding motility of the mutant (not shown).

Figure 6 PtdThr-regulated calcium homeostasis in Toxoplasma gondii

FIGURE 6: Exposure to a calcium ionophore can reinstate the egress and motility of the PTS-knockout strain. (A) Ionophore-induced egress in the parental or Δtgpts strains. Parasitized cultures (MOI, 1; 48 h infection) were stimulated with 5 µM A23187 prior to fixation and staining. Percentage of egressed vacuoles was determined in at least 10 random fields at each time point. Note that the mutant exhibits a natural egress defect, which is amended within 2-3 min of drug exposure. (B-C) Motile fractions and trail lengths of the parasite strains treated with or without ionophore (5 µM A23187). About 500 parasites of each strain were analyzed for TgSag1 trails. Graphs in panel A-C show the mean ± SEM from 3 assays (student’s t-test, *p<0.05, **p<0.01).

It is noteworthy that EGFP activity in ionophore-induced parental and mutant strains was much higher than the natural pools in the untreated samples (Fig. 4A and Fig. 5B). Just 1 min of exposure to ionophore triggered a prominent spike in fluorescence (Fig. 5B), which was greater than the apex ion level achieved in both strains under normal conditions (Fig. 4A). Such an elevated flux of calcium was indeed sufficient to restore egress and gliding motility in the mutant (Fig. 6). These results suggest a need of minimum calcium threshold for an efficient natural egress and gliding motility. Calcium signaling is also known to control exocytosis of micronemes, which actually underlies the motility and invasion [3][4][8][24][26][27]. We did not observe a secretory defect in extracellular tachyzoites of the PTS mutant (not shown), which implies a lower threshold of calcium for microneme secretion. In this context, it should also be mentioned that microplate/cuvette-based quantification of the GECI signal in the extracellular stage have been difficult, presumably due to high variations in tachyzoite preparations and influence of milieu, which prevented us from studying reproducible oscillations in calcium during the secretion and invasion events. Future studies using more sensitive and color-tuned variants of GECI may elucidate the interrelationship of calcium, microneme exocytosis, gliding motility, egress and invasion processes. Equally, organelle-specific expression of GECIs shall illuminate PtdThr-mediated regulation of distinct calcium stores and their relative impacts on calcium signaling.

One of the several known functions of PtdSer, the natural and near universal analog of PtdThr, is to regulate calcium signaling and exocytosis in mammalian cells [28][29]. In particular, PtdSer is known to facilitate the binding of membrane fusion machinery [30], alter the energy for the membrane bending [31], sense calcium to aid membrane fusion events during exocytosis [32], and regulate PLC-mediated IP3-dependent Ca2+ channels [33]. In accord, PtdSer can also inhibit the slippage of calcium to the cytosol by sarcolemmal Ca2+-ATPase, and thereby increases the ion capture in the ER [34]. Last but not least, synthetic derivatives of PtdThr containing defined acyl chains are more potent in inducing exocytosis than PtdSer species [35]. It is therefore plausible that naturally occurring PtdThr can substitute for one or more of such functions of PtdSer in T. gondii. Along the line, the most predominant species of PtdThr (20:1, 20:5) present in tachyzoites [2] may serve as a source of arachidonic acid that can affect membrane fluidity and calcium flux [36]. Although the mechanistic details remain to be examined, this work provides a stimulating premise on potential regulation of calcium homeostasis by PtdThr. Likewise, our method to quantify and compare cytosolic calcium within intracellular parasites as well as across the parasite strains should be applicable to other entwined models.


Biological reagents and resources

The RHΔku80-hxgprt– strain of T. gondii [37] was provided by Vern Carruthers (University of Michigan, USA). The Δtgpts strain was generated in our earlier work [2]. Anti-TgHsp90 [19], anti-TgGap45 [18] and anti-TgSag1 [38] antibodies were donated by Sergio Angel (IIB-INTECH, San Martin, Argentina), Dominique Soldati-Favre (University of Geneva, Switzerland) and Jean-Francois Dubremetz (University of Montpellier, France), respectively. GCaMP6s [14] was obtained from Loren Looger (Howard Hughes Medical Institute, Ashburn, USA). Anti-GFP antibody and oligonucleotides were acquired from Life Technologies (Germany).

Parasite and host cell cultures

Tachyzoites of all strains reported here were propagated in human foreskin fibroblast (HFF) cells in a humidified incubator (37°C, 5% CO2), as described previously [39]. In brief, cells were cultured in Dulbecco’s Modified Eagle Medium (DMEM) containing 10% fetal bovine serum, 2 mM glutamine, 100 µM of each MEM non-essential amino acids (glycine, alanine, asparagine, aspartic acid, glutamic acid, proline, serine), 1 mM sodium pyruvate, 100 U/ml penicillin and 100 µg/ml streptomycin. Parasites were cultured at a multiplicity of infection (MOI) of 3 every 2-3 days. HFF cells were harvested by trypsinization and grown to confluence in fresh flasks, dishes or plates as per experimental requirements.

Molecular cloning and genetic manipulation of T. gondii

GCaMP6s was cloned into pTgGRA1-UPKO plasmid at NsiI/PacI sites for expression under the control of the TgGRA1 promoter and 3’UTR. GECI expression cassette was flanked by 5’ and 3’UTR of the TgUPRT gene, which enabled targeted insertion at the UPRT locus. The complete sequence of GCaMP6s protein was amplified using CTCATCATGCATTCTCATCATCATCATCA TCATGG as the forward primer (NsiI site) and CTCATCTTAATTAATTACTTCGCTGTCATCATTTGTACA as the reverse primer (PacI site). Extracellular tachyzoites of the parental (RHΔku80-hxgprt-) and mutant (Δtgpts) strains (~ 107) were suspended in Cytomix (120 mM KCl, 0.15 mM CaCl2, 10 mM K2HPO4/KH2PO4, 25 mM HEPES, 2 mM EGTA, 5 mM MgCl2, pH 7.6), and then transfected using a BTX electroporation instrument (50 µg DNA, 2 kV, 50Ω, 25 µF, 250 µs). Parasites with a disrupted UPRT locus were selected by adding 5 µM of 5-fluorodeoxyuridine (FUDR) [40] and cloned by limiting dilution. It was not feasible to make an equivalent GCaMP6s-expressing PTS-complemented strain, which was also created by FUDR selection [2]. Furthermore, the complemented strain exhibited unwarranted growth defect due to overexpression of PTS (not observed in the Δtgpts mutant), which excluded its use for the assays reported in this work.

Parasite phenotyping

All experiments were executed using fresh syringe-released extracellular tachyzoites. For plaque assays, 100-200 parasites of each strain were used to infect confluent HFF monolayers cultured in 6-well plates. Parasitized cells were incubated for 7 days without perturbation and then fixed with cold methanol followed by staining of plaques with crystal violet dye. Plaques were imaged and scored for their sizes and numbers using the ImageJ program (NIH, USA). For egress assays, HFF monolayers cultured on glass coverslips were infected with tachyzoites (MOI, 1; 40-72 h), as described elsewhere [41]. Samples were subsequently fixed with 4% paraformaldehyde and 0.05% glutaraldehyde solution in PBS (2 min), neutralized by 0.1 M glycine/PBS (5 min) and blocked in 3% BSA/PBS (30 min). Egressed parasites were stained with anti-TgSag1 antibody (1:1500, 1 h). Cells were washed 3x with PBS, permeabilized with 0.2% Triton X-100/PBS (20 min), and stained with anti-TgGap45 antibody (1:3000, 1 h) to visualize parasites residing in the intact vacuoles. Samples were washed and stained with Alexa488/Alexa594-conjugated secondary antibodies (1:3000, 1 h). The fraction of egressed vacuoles was scored from the number of vacuoles with TgSag1-positive parasites. To examine the gliding motility, parasites were incubated on BSA (0.01%)-coated coverslips in Hank’s Balanced Salt Solution (15 min, 37°C). Samples were fixed with 4% paraformaldehyde and 0.05% glutaraldehyde for 10 min and stained with anti-TgSag1 and Alexa488 antibodies. The motile fractions and trail lengths were quantified using the ImageJ software.

Immunofluorescence and immunoblot assays

GCaMP6s was localized either by EGFP imaging or by immunofluorescence assays. The method was essentially similar to egress assays except for that samples were permeabilized prior to incubation with antibodies. Anti-TgHsp90 (1:1000, rabbit) or anti-TgGap45 (1:6000, rabbit) antibodies were used together with anti-GFP antibody (1:5000, mouse) to examine the subcellular localization of GCaMP6s. Images were acquired using ApoTome microscope (Zeiss, Germany). To do immunoblot analysis, proteins were resolved by sodium dodecyl sulfate polyacrylamide gel electrophoresis (12%) and transferred to a nitrocellulose membrane (85 mA for 90 min) (AppliChem). The membrane was treated overnight with 5% skimmed dry milk (suspended in Tris-buffered saline and 0.2% and tween 20), incubated with anti-GFP (1: 1500, mouse) and anti-TgHsp90 (1:1000, rabbit) antibodies (1 h at room temperature), washed 3x for 5 min each, and then incubated with IR dyes (680 RD, 800 CW, each at 1: 10000 for 1 h). Proteins were visualized using Li-Cor imaging system. Densitometry analysis was done using Image studio software. Expression of GCaMP6s was normalized to the loading of TgHsp90 in each sample lane.

Calcium measurements in intracellular parasites

HFF monolayers cultured in 24-well plates were infected with GCaMP6s-expressing parental and Δtgpts strains (24-50 hrs) with an MOI of 3 and 3.75 to counterbalance for the invasion defect in the mutant [2]. EGFP fluorescence in response to calcium was quantified using a microplate reader (BioTek Instruments; excitation, 485 nm; emission, 528 nm; area scan mode; 37°C). The uninfected (negative control) and infected cells exposed to 5 µM A23187 ionophore (positive control) were included alongside. Alternatively, we also performed live imaging using wide-field microscopy (Zeiss Axiovert 200M). EGFP signal was recorded for 1 min before adding ionophore (5 µM A23187) and then for 10 min after drug treatment. All assays were conducted in standard colorless culture medium containing ~1.8 mM calcium (without phenol red). No exogenous calcium or chelators were added during experiments. The pKa for calcium-bound and calcium-free GCaMP6s is ~6.2 and >9, respectively, and the pH titration curve is similar to that of EGFP [14]. Our own experiments did not reveal an apparent sensitivity of GCaMP6s to the pH variation (pH 5-8).


  1. M.W. Black, and J.C. Boothroyd, "Lytic cycle of Toxoplasma gondii.", Microbiology and molecular biology reviews : MMBR, 2000.
  2. R.D. Arroyo-Olarte, J.F. Brouwers, A. Kuchipudi, J.B. Helms, A. Biswas, I.R. Dunay, R. Lucius, and N. Gupta, "Phosphatidylthreonine and Lipid-Mediated Control of Parasite Virulence", PLOS Biology, vol. 13, pp. e1002288, 2015.
  3. V.B. Carruthers, and L.D. Sibley, "Mobilization of intracellular calcium stimulates microneme discharge in Toxoplasma gondii", Molecular Microbiology, vol. 31, pp. 421-428, 1999.
  4. M.C. Vieira, and S.N. Moreno, "Mobilization of intracellular calcium upon attachment of Toxoplasma gondii tachyzoites to human fibroblasts is required for invasion", Molecular and Biochemical Parasitology, vol. 106, pp. 157-162, 2000.
  5. M. Meissner, D. Schlüter, and D. Soldati, "Role of Toxoplasma gondii Myosin A in Powering Parasite Gliding and Host Cell Invasion", Science, vol. 298, pp. 837-840, 2002.
  6. J.L. Lovett, and L.D. Sibley, "Intracellular calcium stores in Toxoplasma gondii govern invasion of host cells", Journal of Cell Science, vol. 116, pp. 3009-3016, 2003.
  7. E. Garrison, M. Treeck, E. Ehret, H. Butz, T. Garbuz, B.P. Oswald, M. Settles, J. Boothroyd, and G. Arrizabalaga, "A Forward Genetic Screen Reveals that Calcium-dependent Protein Kinase 3 Regulates Egress in Toxoplasma", PLoS Pathogens, vol. 8, pp. e1003049, 2012.
  8. D.A. Pace, C.A. McKnight, J. Liu, V. Jimenez, and S.N. Moreno, "Calcium Entry in Toxoplasma gondii and Its Enhancing Effect of Invasion-linked Traits", Journal of Biological Chemistry, vol. 289, pp. 19637-19647, 2014.
  9. R. Moudy, T.J. Manning, and C.J. Beckers, "The Loss of Cytoplasmic Potassium upon Host Cell Breakdown Triggers Egress of Toxoplasma gondii", Journal of Biological Chemistry, vol. 276, pp. 41492-41501, 2001.
  10. G. Arrizabalaga, and J.C. Boothroyd, "Role of calcium during Toxoplasma gondii invasion and egress", International Journal for Parasitology, vol. 34, pp. 361-368, 2004.
  11. S.N. Moreno, L. Ayong, and D.A. Pace, "Calcium storage and function in apicomplexan parasites", Essays in Biochemistry, vol. 51, pp. 97-110, 2011.
  12. P. Rohrbach, O. Friedrich, J. Hentschel, H. Plattner, R.H. Fink, and M. Lanzer, "Quantitative Calcium Measurements in Subcellular Compartments of Plasmodium falciparum-infected Erythrocytes", Journal of Biological Chemistry, vol. 280, pp. 27960-27969, 2005.
  13. L. Borges-Pereira, A. Budu, C.A. McKnight, C.A. Moore, S.A. Vella, M.A. Hortua Triana, J. Liu, C.R. Garcia, D.A. Pace, and S.N. Moreno, "Calcium Signaling throughout the Toxoplasma gondii Lytic Cycle", Journal of Biological Chemistry, vol. 290, pp. 26914-26926, 2015.
  14. T. Chen, T.J. Wardill, Y. Sun, S.R. Pulver, S.L. Renninger, A. Baohan, E.R. Schreiter, R.A. Kerr, M.B. Orger, V. Jayaraman, L.L. Looger, K. Svoboda, and D.S. Kim, "Ultrasensitive fluorescent proteins for imaging neuronal activity", Nature, vol. 499, pp. 295-300, 2013.
  15. J. Akerboom, T. Chen, T.J. Wardill, L. Tian, J.S. Marvin, S. Mutlu, N.C. Calderón, F. Esposti, B.G. Borghuis, X.R. Sun, A. Gordus, M.B. Orger, R. Portugues, F. Engert, J.J. Macklin, A. Filosa, A. Aggarwal, R.A. Kerr, R. Takagi, S. Kracun, E. Shigetomi, B.S. Khakh, H. Baier, L. Lagnado, S.S. Wang, C.I. Bargmann, B.E. Kimmel, V. Jayaraman, K. Svoboda, D.S. Kim, E.R. Schreiter, and L.L. Looger, "Optimization of a GCaMP Calcium Indicator for Neural Activity Imaging", The Journal of Neuroscience, vol. 32, pp. 13819-13840, 2012.
  16. J. Akerboom, N. Carreras Calderón, L. Tian, S. Wabnig, M. Prigge, J. Tolö, A. Gordus, M.B. Orger, K.E. Severi, J.J. Macklin, R. Patel, S.R. Pulver, T.J. Wardill, E. Fischer, C. Schüler, T. Chen, K.S. Sarkisyan, J.S. Marvin, C.I. Bargmann, D.S. Kim, S. Kügler, L. Lagnado, P. Hegemann, A. Gottschalk, E.R. Schreiter, and L.L. Looger, "Genetically encoded calcium indicators for multi-color neural activity imaging and combination with optogenetics", Frontiers in Molecular Neuroscience, vol. 6, 2013.
  17. T. Nagai, A. Sawano, E.S. Park, and A. Miyawaki, "Circularly permuted green fluorescent proteins engineered to sense Ca 2+", Proceedings of the National Academy of Sciences, vol. 98, pp. 3197-3202, 2001.
  18. F. Plattner, F. Yarovinsky, S. Romero, D. Didry, M. Carlier, A. Sher, and D. Soldati-Favre, "Toxoplasma Profilin Is Essential for Host Cell Invasion and TLR11-Dependent Induction of an Interleukin-12 Response", Cell Host & Microbe, vol. 3, pp. 77-87, 2008.
  19. P.C. Echeverria, M.J. Figueras, M. Vogler, T. Kriehuber, N. de Miguel, B. Deng, M.C. Dalmasso, D.E. Matthews, M. Matrajt, M. Haslbeck, J. Buchner, and S.O. Angel, "The Hsp90 co-chaperone p23 of Toxoplasma gondii: Identification, functional analysis and dynamic interactome determination", Molecular and Biochemical Parasitology, vol. 172, pp. 129-140, 2010.
  20. T. Endo, K. Sethi, and G. Piekarski, "Toxoplasma gondii: Calcium lonophore A23187-mediated exit of trophozoites from infected murine macrophages", Experimental Parasitology, vol. 53, pp. 179-188, 1982.
  21. V.B. Carruthers, O.K. Giddings, and L.D. Sibley, "Secretion of micronemal proteins is associated with toxoplasma invasion of host cells", Cellular Microbiology, vol. 1, pp. 225-235, 1999.
  22. R. Mondragon, and E. Frixione, "Ca(2+)-dependence of conoid extrusion in Toxoplasma gondii tachyzoites.", The Journal of eukaryotic microbiology, 1996.
  23. J.B. Hoek, A.P. Thomas, R. Rubin, and E. Rubin, "Ethanol-induced mobilization of calcium by activation of phosphoinositide-specific phospholipase C in intact hepatocytes.", The Journal of biological chemistry, 1987.
  24. J.L. Lovett, N. Marchesini, S.N. Moreno, and L.D. Sibley, "Toxoplasma gondii Microneme Secretion Involves Intracellular Ca2+ Release from Inositol 1,4,5-Triphosphate (IP3)/Ryanodine-sensitive Stores", Journal of Biological Chemistry, vol. 277, pp. 25870-25876, 2002.
  25. E. Chini, K. Nagamune, D. Wetzel, and L. Sibley, "Evidence that the cADPR signalling pathway controls calcium-mediated microneme secretion in Toxoplasma gondii", Biochemical Journal, vol. 389, pp. 269-277, 2005.
  26. S. Lourido, J. Shuman, C. Zhang, K.M. Shokat, R. Hui, and L.D. Sibley, "Calcium-dependent protein kinase 1 is an essential regulator of exocytosis in Toxoplasma", Nature, vol. 465, pp. 359-362, 2010.
  27. J.M. McCoy, L. Whitehead, G.G. van Dooren, and C.J. Tonkin, "TgCDPK3 Regulates Calcium-Dependent Egress of Toxoplasma gondii from Host Cells", PLoS Pathogens, vol. 8, pp. e1003066, 2012.
  28. T.W. Martin, and D. Lagunoff, "Inhibition of mast cell histamine secretion by N-substituteed derivatives of phosphatidylserine.", Science (New York, N.Y.), 1979.
  29. T.W. Martin, and D. Lagunoff, "Interactions of lysophospholipids and mast cells.", Nature, 1979.
  30. Z. Zhang, E. Hui, E.R. Chapman, and M.B. Jackson, "Phosphatidylserine Regulation of Ca2+-triggered Exocytosis and Fusion Pores in PC12 Cells", Molecular Biology of the Cell, vol. 20, pp. 5086-5095, 2009.
  31. Z. Zhang, and M.B. Jackson, "Membrane Bending Energy and Fusion Pore Kinetics in Ca2+-Triggered Exocytosis", Biophysical Journal, vol. 98, pp. 2524-2534, 2010.
  32. T.P. Rogasevskaia, M.A. Churchward, and J.R. Coorssen, "Anionic lipids in Ca2+-triggered fusion", Cell Calcium, vol. 52, pp. 259-269, 2012.
  33. J.W. Lomasney, H. Cheng, M. Kobayashi, and K. King, "Structural Basis for Calcium and Phosphatidylserine Regulation of Phospholipase C δ1", Biochemistry, vol. 51, pp. 2246-2257, 2012.
  34. K.A. Dalton, J.D. Pilot, S. Mall, J.M. East, and A.G. Lee, "Anionic phospholipids decrease the rate of slippage on the Ca(2+)-ATPase of sarcoplasmic reticulum.", The Biochemical journal, 1999.
  35. M. Iwashita, K. Makide, T. Nonomura, Y. Misumi, Y. Otani, M. Ishida, R. Taguchi, M. Tsujimoto, J. Aoki, H. Arai, and T. Ohwada, "Synthesis and Evaluation of Lysophosphatidylserine Analogues as Inducers of Mast Cell Degranulation. Potent Activities of Lysophosphatidylthreonine and Its 2-Deoxy Derivative", Journal of Medicinal Chemistry, vol. 52, pp. 5837-5863, 2009.
  36. A. Bonhomme, A. Bouchot, N. Pezzella, J. Gomez, H. Le Moal, and J. Pinon, "Signaling during the invasion of host cells byToxoplasma gondii", FEMS Microbiology Reviews, vol. 23, pp. 551-561, 1999.
  37. M. Huynh, and V.B. Carruthers, "Tagging of Endogenous Genes in aToxoplasma gondiiStrain Lacking Ku80", Eukaryotic Cell, vol. 8, pp. 530-539, 2009.
  38. J.F. Dubremetz, C. Rodriguez, and E. Ferreira, "Toxoplasma gondii: redistribution of monoclonal antibodies on tachyzoites during host cell invasion.", Experimental parasitology, 1985.
  39. N. Gupta, M.M. Zahn, I. Coppens, K.A. Joiner, and D.R. Voelker, "Selective disruption of phosphatidylcholine metabolism of the intracellular parasite Toxoplasma gondii arrests its growth.", The Journal of biological chemistry, 2005.
  40. R.G. Donald, and D.S. Roos, "Insertional mutagenesis and marker rescue in a protozoan parasite: cloning of the uracil phosphoribosyltransferase locus from Toxoplasma gondii.", Proceedings of the National Academy of Sciences of the United States of America, 1995.
  41. A.T. Heaslip, M. Nishi, B. Stein, and K. Hu, "The Motility of a Human Parasite, Toxoplasma gondii, Is Regulated by a Novel Lysine Methyltransferase", PLoS Pathogens, vol. 7, pp. e1002201, 2011.


We thank Grit Meusel (Humboldt University) for her technical and research assistance. The work was funded by independent research grants awarded to NG (SFB618/C7, GU1100/4-1) by German Research Foundation (DFG).


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Optogenetic monitoring identifies phosphatidylthreonine-regulated calcium homeostasis in Toxoplasma gondii by Kuchipudi et al. is licensed under a Creative Commons Attribution 4.0 International License.

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