Quantitative analysis of Plasmodium ookinete motion in three dimensions suggests a critical role for cell shape in the biomechanics of malaria parasite gliding motility

Authors

  • Andrey Kan,

    1. Victoria Research Laboratory, National ICT Australia (NICTA), Department of Computing and Information Systems, University of Melbourne, Melbourne, Vic., Australia
    Search for more papers by this author
    • These authors contributed equally.
  • Yan-Hong Tan,

    1. Infection and Immunity Division, The Walter and Eliza Hall of Institute of Medical Research, Parkville, Vic., Australia
    Search for more papers by this author
    • These authors contributed equally.
  • Fiona Angrisano,

    1. Infection and Immunity Division, The Walter and Eliza Hall of Institute of Medical Research, Parkville, Vic., Australia
    2. Department of Medical Biology, University of Melbourne, Vic., Australia
    Search for more papers by this author
  • Eric Hanssen,

    1. Electron Microscopy Unit Bio21 Molecular Science and Biotechnology Institute and Department of Biochemistry and Molecular Biology, University of Melbourne, Parkville, Vic., Australia
    Search for more papers by this author
  • Kelly L. Rogers,

    1. Centre for Dynamic Imaging, The Walter and Eliza Hall of Institute of Medical Research, Parkville, Vic., Australia
    2. Department of Medical Biology, University of Melbourne, Vic., Australia
    Search for more papers by this author
  • Lachlan Whitehead,

    1. Centre for Dynamic Imaging, The Walter and Eliza Hall of Institute of Medical Research, Parkville, Vic., Australia
    Search for more papers by this author
  • Vanessa P. Mollard,

    1. School of Botany, The University of Melbourne, Parkville, Vic., Australia
    Search for more papers by this author
  • Anton Cozijnsen,

    1. School of Botany, The University of Melbourne, Parkville, Vic., Australia
    Search for more papers by this author
  • Michael J. Delves,

    1. Department of Life Sciences, Imperial College of Science, Technology and Medicine, London, UK
    Search for more papers by this author
  • Simon Crawford,

    1. School of Botany, The University of Melbourne, Parkville, Vic., Australia
    Search for more papers by this author
  • Robert E. Sinden,

    1. Department of Life Sciences, Imperial College of Science, Technology and Medicine, London, UK
    Search for more papers by this author
  • Geoffrey I. McFadden,

    1. School of Botany, The University of Melbourne, Parkville, Vic., Australia
    Search for more papers by this author
  • Christopher Leckie,

    1. Victoria Research Laboratory, National ICT Australia (NICTA), Department of Computing and Information Systems, University of Melbourne, Melbourne, Vic., Australia
    Search for more papers by this author
  • James Bailey,

    1. Victoria Research Laboratory, National ICT Australia (NICTA), Department of Computing and Information Systems, University of Melbourne, Melbourne, Vic., Australia
    Search for more papers by this author
  • Jake Baum

    Corresponding author
    1. Infection and Immunity Division, The Walter and Eliza Hall of Institute of Medical Research, Parkville, Vic., Australia
    2. Department of Medical Biology, University of Melbourne, Vic., Australia
    3. Department of Life Sciences, Imperial College of Science, Technology and Medicine, London, UK
    Current affiliation:
    1. Department of Life Sciences, Sir Alexander Fleming Building, Imperial College London, London, UK
    Search for more papers by this author

Summary

Motility is a fundamental part of cellular life and survival, including for Plasmodium parasites – single-celled protozoan pathogens responsible for human malaria. The motile life cycle forms achieve motility, called gliding, via the activity of an internal actomyosin motor. Although gliding is based on the well-studied system of actin and myosin, its core biomechanics are not completely understood. Currently accepted models suggest it results from a specifically organized cellular motor that produces a rearward directional force. When linked to surface-bound adhesins, this force is passaged to the cell posterior, propelling the parasite forwards. Gliding motility is observed in all three life cycle stages of Plasmodium: sporozoites, merozoites and ookinetes. However, it is only the ookinetes – formed inside the midgut of infected mosquitoes – that display continuous gliding without the necessity of host cell entry. This makes them ideal candidates for invasion-free biomechanical analysis. Here we apply a plate-based imaging approach to study ookinete motion in three-dimensional (3D) space to understand Plasmodium cell motility and how movement facilitates midgut colonization. Using single-cell tracking and numerical analysis of parasite motion in 3D, our analysis demonstrates that ookinetes move with a conserved left-handed helical trajectory. Investigation of cell morphology suggests this trajectory may be based on the ookinete subpellicular cytoskeleton, with complementary whole and subcellular electron microscopy showing that, like their motion paths, ookinetes share a conserved left-handed corkscrew shape and underlying twisted microtubular architecture. Through comparisons of 3D movement between wild-type ookinetes and a cytoskeleton-knockout mutant we demonstrate that perturbation of cell shape changes motion from helical to broadly linear. Therefore, while the precise linkages between cellular architecture and actomyosin motor organization remain unknown, our analysis suggests that the molecular basis of cell shape may, in addition to motor force, be a key adaptive strategy for malaria parasite dissemination and, as such, transmission.

Introduction

Malaria is one of the leading causes of infant mortality in the developing world (WHO, 2013). The disease is caused by intracellular parasites from the genus Plasmodium, single-celled protozoa that are transmitted to a vertebrate host following the bite from an infected female mosquito. Its two-host life cycle – progressing from the midgut of an infected mosquito, through to a vertebrate host and back into the subsequent feeding mosquito – is dominated by cell motility. At every stage, the parasites must target and penetrate host tissues to establish the sequential steps of development (Prudencio et al., 2006; Vlachou et al., 2006; Cowman et al., 2012). Unlike other eukaryotic cells, however, cell motility in these parasites does not involve gross changes in cell morphology or the use of a flagellum [though they are certainly capable of generating one as is shown with male gametocytes (Sinden and Croll, 1975)], but is instead driven by an internal actomyosin motor, which allows the motile parasite to literally glide across substrate surfaces and invade host cells (Soldati et al., 2004; Baum et al., 2008; Farrow et al., 2011). The molecular basis for gliding motility in Plasmodium has been studied most intensively in the two life cycle stages associated with intracellular infection of the vertebrate host (host-cell invasion), the sporozoite and merozoite (Kappe et al., 1999; Baum et al., 2006). Work on these stages, drawing extensively on studies from the related apicomplexan parasite Toxoplasma gondii (Gaskins et al., 2004), has identified several core components of the gliding motor in addition to actin and myosin. This gliding-associated complex (or glideosome) anchors the myosin motor to the external membrane of a flattened leaflet that lies within the parasite pellicle, called the inner membrane complex (IMC) (Raibaud et al., 2001). The proteins that make up the glideosome are broadly conserved across the apicomplexan phylum to which Plasmodium parasites belong (Bergman et al., 2003; Gaskins et al., 2004; Baum et al., 2006; Green et al., 2006; Jones et al., 2006; Frénal et al., 2010). According to current thinking, these link through to the extracellular milieu via a series of linkages beginning with the short actin filament (Russell and Sinden, 1981; King, 1988), the glycolytic enzyme aldolase (Buscaglia et al., 2003; Jewett and Sibley, 2003), and finally surface-secreted transmembrane-associated adhesins (Buscaglia et al., 2003; Jewett and Sibley, 2003; Baum et al., 2006; Starnes et al., 2009). The combined rearward passage of linked adhesins, by the myosin motor, propels the parasite along substrate surfaces and/or into host cells (Pinder et al., 1998; Meissner et al., 2002; Siden-Kiamos et al., 2011).

Despite its extensive study, there is only limited evidence for the physical organization of the motor and glideosome components within the parasite cell other than their general spatial compartmentalization, or their specific membrane association (Frénal et al., 2010). A suggestion for organization in the IMC may be visible in cryoelectron microscopy (CryoEM) of the Plasmodium gallinaceum ookinete (Raibaud et al., 2001). Imaging of this life cycle stage, the motile polyploid zygote that colonizes the mosquito midgut (Angrisano et al., 2012c), reveals a periodic distribution of inner membrane particles (Raibaud et al., 2001) that would fit with an organized distribution of the motor in the pellicular space. Evidence for actual organization of each motor component has, however, relied primarily on immunoprecipitation of glideosome and associated constituents, stepwise links between which bridge the gap from the IMC inside through to the extracellular milieu (Kappe et al., 1999; Bergman et al., 2003; Gaskins et al., 2004; Baum et al., 2006; Green et al., 2006; Jones et al., 2006; Frénal et al., 2010). Critically, because of lack of evidence of organization, it is unclear how precise directional force is generated, for example whether it is via the orientation of actin filaments (F-actin), the myosin motor head or some other guiding constraint (Raibaud et al., 2001). A key limitation is that no study has been able to visualize F-actin in the pellicular space of a motile apicomplexan parasite, whose orientation would logically be a key determinant of effective cell movement (Wetzel et al., 2003; Kudryashev et al., 2010; Angrisano et al., 2012b). Reasons for this may be due to the short and highly dynamic nature of Plasmodium actin microfilaments (Schmitz et al., 2005; Schüler et al., 2005; Sahoo et al., 2006) coupled with the relatively small size of motile parasite cells that contain them, rendering current visualization techniques less feasible to utilize (Schmitz et al., 2005; Schüler et al., 2005; Sahoo et al., 2006). Myosin complex organization has not been addressed at sufficient resolution to assess its contribution. Thus, our understanding of how molecular changes inside the parasite translate into directional force remains speculative.

The fundamentals of gliding have instead been largely derived at whole cell level, exploring motile parasites in vitro and in vivo by video microscopy (King, 1981; 1988; Russell and Sinden, 1981; Wetzel et al., 2003). Cell shape in particular would be expected to play a significant role in the biomechanics of gliding, as found with other unicellular pathogens such as trypanosomatids and spirochaetes (Murphy et al., 2008; Heddergott et al., 2012). Towards this, studies on the ultrastructure of sporozoites have found that cellular asymmetry likely underlies chiral motion of this parasite stage (Kudryashev et al., 2012). Chiral shape does not appear to hold true for the merozoite beyond an asymmetrical distribution of microtubules (Hanssen et al., 2013) and the question of three-dimensional (3D) shape in the ookinete has not been fully explored.

Video microscopy has been instrumental in defining the key role of actin in Plasmodium and related parasite cell movement, such as via bead movement on the surface of parasites or their general arrest in the presence of actin inhibitors (King, 1988; Siden-Kiamos et al., 2006; Munter et al., 2009; Angrisano et al., 2012a). Most recently, detailed imaging of Plasmodium berghei sporozoites has revealed that cell adhesion to the substrate and a continuous sequence of actin-dependent stick-and-slip phases of motility underlies sporozoite actomyosin-based motility (Munter et al., 2009; Hegge et al., 2010) making a linkage between parasite molecular events and its effect on motion. Likewise, studies with a hydrogel system have made steps towards defining the first in vivo estimates of motor organization, such as actin filament length, by varying inter-particle spacing in these artificial grids (Perschmann et al., 2011). Despite these detailed studies, however, resolving the long-standing question of the interplay between motor organization, cell shape and directional motility has not been achieved and, as importantly, only a few studies have attempted to explore cell motility in a 3D context for any apicomplexan cell (Vlachou et al., 2004; Amino et al., 2006; Hellmann et al., 2011).

The ookinete while known to rely on the same basic actomyosin motor for movement (Dessens et al., 1999; Yuda et al., 1999; Siden-Kiamos et al., 2006; 2011; Angrisano et al., 2012a), has been much less investigated compared to its blood and liver-stage counterparts. Unlike sporozoite and merozoite stages, the ookinete relies on continuous motile forces to break through the epithelial cell layer of the midgut, during which the ‘invaded’ cell is lysed (Han et al., 2000; Vlachou et al., 2004). It may thus serve as an ideal representative cell for dissecting the mechanics of general motility in Plasmodium cells (and Apicomplexa more broadly) given the absence of potentially confounding influences of the host cell during invasion. Ookinetes form in the blood bolus 10 to 25 h post gamete fusion (syngamy) (Janse et al., 1985). They must reach the mosquito midgut epithelium and burrow through to the basal lamina, with very few completing development into an oocyst (Baton and Ranford-Cartwright, 2005; Sinden, 2009). Although some of the molecular events involved in midgut traversal have been defined (Kariu et al., 2006; Armistead et al., 2011; Mathias et al., 2012), the process of ookinete targeting of the epithelium is still incompletely understood. The distribution of gametocytes, forming zygotes and resulting ookinetes, would be expected to be approximately random within the blood bolus; however, targeting of the midgut could be either stochastic or involve a chemotactic or cellular trophic signal. While some studies have suggested the possibility of ookinete tropism for certain cells within the midgut epithelium (Shahabuddin et al., 1998; Cociancich et al., 1999), this hypothesis, or indeed any obvious chemotactic behaviour from the ookinete, is not supported from in vivo or ex vivo video microscopy of the colonization process (Freyvogel, 1966; Zieler and Dvorak, 2000; Vlachou et al., 2004). Thus, in the absence of cellular tropism, and given that digestion of the blood meal and ookinete colonization of the midgut epithelium basal layer largely coincide [at around 24 h post feeding (Graf et al., 1986)], we might expect exit from the central blood meal and oocyst formation to occur largely at random along the epithelial surface.

Ookinete motility itself in vivo, ex vivo (Freyvogel, 1966; Zieler and Dvorak, 2000; Vlachou et al., 2004) and in vitro (Moon et al., 2009; Angrisano et al., 2012a; Volkmann et al., 2012) has been characterized as ranging from a general ‘snake-like’ helical pattern defining the most obvious motile event to other spiralling or linear forms of motion, the significance of which is not clear. However, no study to date has described a quantitative model for ookinete motility or defined how movement in 3D might correlate to traction and force from the internal actin-myosin motor. In addition, while the role of cell shape in ookinete motility is clearly important (Tremp and Dessens, 2011; Volkmann et al., 2012), links between the three key properties of motility, cell shape and directional motion have not been made.

Here, we combine insights about the spatial distribution of ookinete colonization of the mosquito midgut, a plate-based assay for in vitro motility and 3D structural microscopy to advance the ookinete as a powerful life cycle cell type to test the fundamental principles of Plasmodium cell motility and assess contributions of cell shape and motor force in determining the biomechanics of parasite movement that underpin successful transmission.

Results and discussion

Spatial distribution of ookinete exit from the midgut

It remains uncertain whether ookinetes in native infections target a subset of midgut cells (showing specific host-cell or tissue tropism) or exit the midgut stochastically as a result of random formation and exit from the blood meal (Sinden and Billingsley, 2001). One reason for confusion in this area is that the distribution of ookinete exit may be confounded by gravity, whereby oocysts preferentially develop at the posterior end of the midgut due to either the vertical (head-up) post-feed resting of engorged mosquitoes (Cociancich et al., 1999; Han et al., 2000; Sinden and Billingsley, 2001), the progression of digestion from posterior to anterior in the midgut (Graf et al., 1986) or any difference in density that they show when compared to the surrounding blood meal. Lack of clarity about this alters the expectation of whether ookinetes are expected to demonstrate classical foraging behaviour, such as random walks, tumbling or true chemotaxis to facilitate midgut exit (Berg, 1976), or follow a relatively simple (and energy efficient) strategy of moving along a straight line until they reach the epithelium. To explore which strategy may be in action, we determined the spatial distribution of P. berghei oocysts in multiple infected Anopheles stephensi mosquitoes 5 days post feeding. Although there will be some disconnect between ookinete crossing the midgut and oocyst formation – since ookinetes explore the midgut surface before crossing (Zieler and Dvorak, 2000; Vlachou et al., 2004) – oocyst distribution represents a good approximation for the spatial distribution of exit events. Previous studies have explored the question of cellular tropism in the midgut, by measuring oocyst distribution along the anterior–posterior axis in unconstrained mosquitoes versus those kept in a rotating chamber (Cociancich et al., 1999). We revisited these experiments by immobilizing mosquitoes in pipette tips in a restricted head-up, head-down or unconstrained (unbiased) position (Fig. 1A) using a P. berghei line constitutively expressing green fluorescent protein (GFP) (Franke-Fayard et al., 2004). Five days post feeding, the earliest time at which fluorescent oocysts could be adequately resolved and latest to which mosquitoes tolerated immobilization, GFP foci were counted. A frequency distribution of these oocysts along the anterior–posterior axis showed no statistically significant bias between the test and unconstrained feeding regimens (mean and SD: unconstrained = 0.61 ± 0.23; head up = 0.58 ± 0.23, head down = 0.62 ± 0.25, Mann–Whitney U-test between means, unconstrained versus head up or head down groups, P = 0.87 and 0.93, respectively, Fig. 1B). The broad spatial distribution, independent of immobilized-mosquito orientation, therefore suggests that ookinete exit from the midgut is not influenced by gravity or density. Furthermore, while a trend of the distribution towards the posterior midgut is consistent with most parasites developing within the bulk of the blood meal (that sits posteriorly), no other obvious tissue tropism or targeting is evident, consistent with the work of others (Han et al., 2000; Zieler and Dvorak, 2000). We therefore believe it is most likely that ookinetes exit the midgut in an unbiased or random fashion, dependent only on their site of formation within the blood meal itself.

Figure 1.

Colonization of the mosquito midgut by P. berghei ookinetes is effectively random.

A. Post-feed mosquitoes were allowed to rest unconstrained or immobilized in head-down or head-up orientations. The distribution of fluorescent oocysts was measured along the anterior–posterior axis 5 days post feeding.

B. Frequency distributions of individual oocysts along anterior–posterior axis is similar across the three groups of mosquitoes irrespective of immobilized orientation.

An in vitro, quantitative 3D ookinete motility assay

If exit is unbiased, for randomly oriented ookinetes that are unaware of their position within the midgut, a simple straight line exiting strategy would appear to be the most efficient way of reaching the midgut epithelium. For example, for a continuous time random walk (Metzler and Klafter, 2000) there is a probability that exiting would take a considerable amount of time, whereas straight line motion guarantees to find an exit within ∼ 2 h (given an average cross-section width or length of the midgut between ∼ 0.8 mm and 1.2 mm and apparent speed of ∼ 10 μm min−1, see next section). Previous video microscopy of motility, however, clearly demonstrates that ookinetes move with a complex non-linear motion trajectory. Ookinetes from several species have been found to move in a meandering helical fashion both in vitro and in vivo suggesting other factors influence epithelial targeting beyond a simple straight-line exit strategy (Freyvogel, 1966; Vlachou et al., 2004; Moon et al., 2009; Ramakrishnan et al., 2011; Volkmann et al., 2012). A single study described three distinct patterns of motility: stationary rotation, directional spiralling and straight-segment motility (Vlachou et al., 2004). However, there is still insufficient detail in these data to explore whether a general model for motility is applicable to ookinetes that could be used towards defining some of its underlying mechanisms.

To explore whether ookinete movement can be described in general terms, we extended the current in vitro Matrigel assay (Ishino et al., 2006; Moon et al., 2009; Volkmann et al., 2012) towards a more quantitative format that could measure ookinete motion in 3D space and use the parameters of this movement to build a model for idealized ookinete motility (see Experimental procedures). Reconstruction of tracks in 3D clearly confirmed the characteristic helical motion paths for ookinetes (Fig. 2A and B and Supplementary Movies S1–S3). Re-centring motility tracks in each assay at a single point, demonstrated that motion is random in 3D space, showing no overall bias in directionality (Fig. 2C; Wilcoxon signed-rank test for the differences between x, y or z co-ordinates for each track at the beginning and end of movie P-values 0.30, 0.72 and 0.09, respectively, n = 52; see Supplementary Discussion for extended discussion). While obviously lacking potential host chemotactic cues in our assay format, the random distribution is consistent with our imaging of the entire infected midgut excluding gravitational forces in the colonization process. Finally, although predominantly focused on an in vitro description of motility, we wanted to explore whether motion in a Matrigel assay is qualitatively similar to in vivo ookinete motility. Towards assessing this, 3D tracks were reconstructed from real-time in vivo imaging of the same fluorescent ookinetes travelling through an explanted infected A. stephensi mosquito midgut. Because of difficulty in controlling the timing of ookinete development and mosquito infections, only a few events were captured that could facilitate detailed description (n = 4). However, of those captured, chiral motion was clearly apparent (Fig. 2D and E and Supplementary Movies S4 and S5) and, while speed was reduced (e.g. apparent speed ∼ 10.5 in vitro versus ∼ 7 μm min−1 in vivo), the approximate coherence between our in vitro and in vivo imaging data is consistent with motion paths seen with previous in vitro and in vivo work (Freyvogel, 1966; Vlachou et al., 2004; Volkmann et al., 2012).

Figure 2.

Parameterization of P. berghei ookinete cell movement by in vitro and in vivo three dimensional motility assays.

A and B. (A) A sample 3D ookinete track in Matrigel and (B) reconstructed 3D tracks from a single well Matrigel assay exhibiting characteristic helical motion paths.

C. Reconstructed tracks in vitro from panel (B) translocated to a common origin do not show any prominent bias in direction.

D and E. Imaging and single motion tracks for ookinetes imaged in an explanted Anopheles stephensi midgut. Red circles in tracks denote the initial position of fluorescent ookinetes (see also Supplementary Movies S1–S4).

In summary, following the absence of evidence for a preferred site of exit within the mosquito midgut (previous section) our in vitro motility assay did not reveal any apparent bias in directionality, nor the change in directionality over time, which combined are concordant with a ‘straight line’ exit strategy used by the ookinete.

Parameterization of ookinete motility

While variation in motility is clearly present, the mode of movement found in the majority of moving ookinetes could be adequately described by six parameters (see Supplementary Discussion, Supplementary Figs S1–S3 and Supplementary Code and Data, available on request): apparent speed (μm min−1), total displacement (μm), chirality (% of left-handed turns), period of the helix (min, time taken to make a loop), radius of the helix (μm) and pitch of the helix (μm) (Table 1).

Table 1. Numerical description of ookinete locomotion using six parameters
 Apparent speedTotal displacement (10 min)ChiralityPeriodRadiusPitch
(μm min−1)(μm)(% left turns)(min)(μm)(μm)
  1. If period estimation fails a track is considered erratic, and period is not reported. Furthermore, radius and pitch are not computed for erratic tracks. Numbers show mean ± SD.
Wild-type10.5 ± 2.366.3 ± 16.680.0 ± 20.81.6 ± 0.42.2 ± 0.512.6 ± 4.2
Total tracks = 52Helical tracks = 43
100 nM CD4.3 ± 1.1517.4 ± 11.211.8 ± 20.82.4 ± 0.12.1 ± 0.48.0 ± 1.5
Total tracks = 56Helical tracks = 6
IMC1h-KO7.5 ± 3.128.2 ± 16.418.8 ± 11.2
Total tracks = 39Helical tracks = 0
Wild-type in vivo7.0 ± 1.010.7 ± 6.278.6 ± 26.43.7 ± 1.12.9 ± 0.74.4 ± 2.9
Total tracks = 4Helical tracks = 4

Apparent speed is an estimation of the real (instantaneous) ookinete speed, calculated as a sum of distances between track locations in subsequent images divided by the total travel time (as opposed to the gross distance travelled by an ookinete over time, see Supplementary Discussion). In our assay, ookinetes moved with an estimated speed of 10.5 ± 2.3 μm min−1 (mean and SD, Table 1). This figure is faster than previous estimates for ookinete speed in Matrigel [5.8 μm min−1 (Moon et al., 2009), 6.8 μm min−1 (Volkmann et al., 2012)], insect cell co-culture [6 μm min−1 (Siden-Kiamos et al., 2006)] and in vivo midgut assays [5 μm min−1 (Vlachou et al., 2004) and 7 μm min−1 from our own in vivo imaging, Table 1]. Of note, these estimates (except our own in vivo analyses) were obtained using notably lower frame rates. Furthermore, some of these estimates reflect total displacement divided by time. Both factors will combine to underestimate total distance covered and thus reduce the actual speed determined (Supplementary Discussion). For example, in our assay total net displacement over 10 min was found to be 66.3 ± 16.6 μm (Table 1), implying an average speed of 6.6 μm min−1, directly comparable with previous measures. However, given our own slower speeds for in vivo imaging (Table 1) we cannot exclude the possibility that density of the extracellular environment may be inconsistent between our Matrigel assay and others described. Ultimately, while acknowledging the variance associated with our own measurements, a speed of approximately 10 μm min−1 is a good approximation of ookinete instantaneous speed in these artificial conditions.

Chirality measures how well tracks conform to a right-handed helix (values close to −100%) or to a left-handed helix (values close to +100%), where 0 would indicate an erratic track (i.e. no prominent helical pattern). Helical motion is left-handed when the path of motion along the helix's axis moves towards the observer following a clockwise screwing motion. In our assay, chirality was 80.0 ± 20.8% (Table 1) demonstrating that ookinetes almost exclusively move in a left-handed helix. Of note, studies with T. gondii have found a similar left-handed chirality to their 3D helical motion (Leung et al., 2014) suggesting general apicomplexan principles may be at work. Previous studies on Plasmodium sporozoite motion, focused on two-dimensional (2D) measurements of parasite motion on a glass slide, described motility in terms of clockwise or counter-clockwise motion (Vanderberg, 1974; Russell and Sinden, 1981; Hegge et al., 2010; Kudryashev et al., 2012). However, from 2D data alone it is not possible to determine chirality of the underlying 3D helix (Gurarie et al., 2011).

The last three parameters describe a helical motion model, where periodic motion is reliably established. Periodicity estimates the time it takes for an ookinete to make one complete loop, found to be on average 1.6 ± 0.4 min, while, radius (across the helical cylinder) and pitch (distance between loops) were found to be, 2.2 ± 0.5 μm and 12.6 ± 4.2 μm respectively (Table 1). These estimated statistics of helical motion can be presented as an idealized ookinete track describing the motion of the majority of motile parasite cells (Fig. 3). Where ookinetes move erratically or according to another unrelated gait (Vlachou et al., 2004), our periodicity estimation method cannot be applied (see Experimental procedures) and, logically, radius and pitch cannot be computed. Of note, radius and pitch estimates depend on computed period, but are independent of other parameters, while chirality, speed and displacement, are each computed independently. Chirality is internally based on the choice of step size (see Supplementary Discussion), but this does not affect any other parameter.

Figure 3.

The left-handed helical motion of P. berghei ookinetes. An idealized model of left-handed helical motion using the empirically defined parameters inferred from reconstructed tracks.

Effects of actin inhibition on ookinete motility parameters

Ookinete motion has been extensively described as being dependent on actin and myosin (Siden-Kiamos et al., 2006; 2011; Angrisano et al., 2012a). To date, specific inhibitors of apicomplexan myosin have not been described. However, ookinete motility is sensitive to actin destabilizing drugs such as cytochalasin D (CD) (Siden-Kiamos et al., 2006; 2011; Angrisano et al., 2012a). Ookinete average speed (estimated from net displacement) over a range of CD concentrations compared to dimethyl sulfoxide (DMSO) untreated controls was measured and found to lead to a ∼ 50% reduction in speed at 100 nM (Fig. 4A and B), in line with previous reports (Siden-Kiamos et al., 2006; Angrisano et al., 2012a). At this concentration apparent speed was reduced from 10.5 ± 2.3 μm min−1 to 4.3 ± 1.2 μm min−1 compared to DMSO controls (Fig. 4C, Table 1). Total displacement under these conditions was markedly reduced compared to controls and chirality dropped down to 11.8 ± 20.8%. However, a reduction in chirality may primarily arise from a difficulty in assessing this parameter in immotile parasites. Of note, from the 56 tracks analysed, only six could be defined as predominantly chiral (Fig. 4, Table 1). These tracks, though short, were all left-handed, had a very similar radius to those of untreated parasites (Mann–Whitney U-test, P > 0.05) but had a lengthened period and reduced pitch (Mann–Whitney test, P < 0.001). Thus, while CD clearly ablates motility, it would seem that curtailing motor function does not change all gross parameters of ookinete motion.

Figure 4.

Cytochalasin D ablates P. berghei ookinete motion.

A. Dosage response curve of average ookinete speed (calculated from net displacement) in the presence of cytochalasin D, used to determine an effective concentration at which speed is reduced to 50% (∼ 100 nM). Data from three independent replicates, with mean and SD (error bars) shown.

B. Representative 2D motion tracks for 10 nM, 100 nM (IC50) and 5 μM cytochalasin D treatment. Scale bar = 40 μm.

C. Reconstructed 3D motion tracks from a representative motility assay well using 100 nM cytochalasin D.

Assessing the cellular basis for ookinete chirality

Of all parameterized features of ookinete motion, the strict handedness of ookinetes in 3D space (80.0 ± 20.8%) is the most striking. This feature has been described in several previous reports of Plasmodium parasite cellular motility, although detail of image capture conditions and different nomenclatures used (clockwise instead of handedness for example) make it hard to correlate whether strict handedness of ookinetes (Speer et al., 1975; Vlachou et al., 2004) or sporozoites (Vanderberg, 1974; Kudryashev et al., 2012) is a conserved Plasmodium feature. Chirality as a cell motility phenomenon can arise from two (interdependent) cellular factors. Strict organization of the motor force that provides a consistently directed rotational force will give rise to generalized chiral, helical motion (Jennings, 1901; Jahn and Votta, 1972; Crenshaw, 1996). Alternatively, the shape of a motile cell will also give rise to chiral motion as it does with trypanosomes or spirochaetes (Murphy et al., 2008; Heddergott et al., 2012) irrespective of how the force is produced. In apicomplexan parasites, shape and motor organization are both inter-linked by their dependence on the pellicular cytoskeleton, i.e. the subpellicular microtubules and subpellicular network (Mann and Beckers, 2001; Morrissette and Sibley, 2002), composed of alveolins (or IMC proteins) and other protein components (Raibaud et al., 2001; Gould et al., 2008; Bullen et al., 2009). Although the precise nature of linkages is not known, myosin motor and glideosome specifically connect with the subpellicular network (Bullen et al., 2009). At present, there is no clear way of disrupting glideosome organization without affecting its function to test whether it is the precise organization/anchorage of motor force, such as the myosin head or actin filament polarity, that drives directional parasite chiral motion or whether it is the general parasite shape or both.

Towards exploring the contribution of cell shape, we first sought to determine an accurate 3D reconstruction of an ookinete. Logically, like a corkscrew, the twist of the cell will generate a similar chiral motion of the parasite through 3D space with the same handedness. However, to date, precise exploration of ookinete 3D shape has been limited to scanning electron microscopy (SEM) studies that describe an overall twisting along the longitudinal axis of these motile cells (Speer et al., 1974; Sinden et al., 1987). The twist, while clearly obvious in prior SEM work and our own images (Fig. 5A), is ambiguous with respect to handedness because of the difficulty in determining whether the system used for image capture is mirrored (see also Supplementary Discussion). Given these challenges, we used serial section Focused Ion Beam (FIB)-EM (Bushby et al., 2011), a methodology that allows reconstruction of whole cells from electron micrograph sections. Reconstruction at 50 nm serial sections confirmed the twisted shape of ookinetes seen in SEM (Fig. 5B and C). With knowledge of the handedness of our imaging system and analysis (both its mirroring of the individual sections and the handedness of the Cartesian system used in assembling the 3D image) we determined that ookinete shape confirms to a left-handed helical twist (Fig. 5C and Supplementary Movie S6).

Figure 5.

P. berghei ookinetes have a distinctive 3D shape and underlying twisted microtubule lattice.

A. Scanning electron microscopy (SEM) of ookinetes.

B. 3D shape of ookinetes reconstructed using Focused Ion Beam-Electron Microscopy (FIB-EM) reveals chiral shape of ookinetes. Note, a pseudo-skeletonized rod-shaped line is traced along the ookinete central axis to help visualize curvature (i.e. twist or curl) of cell shape.

C. A single ookinete from (B) conforming to a left-handed helical element, where four consecutive points define three vectors (a, b, c) with a distinct spatial orientation (see Supplementary Discussion and Supplementary Fig. S2).

D. Transmission electron microscopy (TEM) section showing circular array of subpellicular microtubules (zoom, white arrowheads point to microtubules, mt).

E. As D showing electron dense linkages between subpellicular microtubules and inner membrane complex (IMC). PM: plasma membrane.

F. Critical point-dried cytoskeleton of a P. berghei ookinete visualized by negative staining electron microscopy reveals the underlying twisted microtubule lattice. Distinct transitions in twisting can be seen midway along the ookinete from the apical pole where twisting becomes less marked.

G. As (F) using cryoelectron microscopy.

To explore the underlying basis of this dominant left-handed chiral shape, we attempted visualization of the intact cytoskeleton of the ookinete to determine its contribution to cell twisting. Subpellicular microtubules lie under the outer pellicle of the ookinete and are arrayed, evenly spaced, around the circumference in cross-sectional slices through an ookinete (Fig. 5D), where they attach through to the IMC via short electron dense extensions of unknown origin (Fig. 5E, yellow arrows) (Raibaud et al., 2001). Previous studies with sporozoites from the related apicomplexan parasite Eimeria acervulina revealed a twisted or spiralling lattice of subpellicular microtubules when visualized in critical-point-dried whole cytoskeletal preparations (Russell and Burns, 1984). Using the same approach, visualized by negative stain and CryoEM (see Experimental procedures), we were able to extract the ookinete microtubule cytoskeleton and demonstrate that it too has an inherent twisted/spiral lattice made up from angled filaments (Fig. 5F and G). While chirality could not be determined (since images are by nature only two-dimensional), the observation that the lattice spirals is consistent with an inherent linkage between intracellular architecture and a gross helical morphology.

Apicomplexan microtubules, including those of ookinetes, contain 13-protofilaments (Raibaud et al., 2001; Cyrklaff et al., 2007), a configuration expected to give rise to straight longitudinal filaments (Amos, 2004). Their angled, spiral arrangement could conceivably arise from a skewed anchorage of each filament to the microtubule organizing centre at the ookinete apex, much like that seen in the sporozoite (Kudryashev et al., 2012) and/or the addition of specific protofilament-binding proteins or linkages with the IMC (Raibaud et al., 2001) (Fig. 5E, yellow arrows) which would alter the direction of the overall microtubule from straight to angular (Cyrklaff et al., 2007). Such an organization away from longitudinal expectations would be consistent with the adaptation of the microtubule lattice for cell shape, and by extension to its role in chiral cell motion.

Ookinete cell shape correlates with their movement in 3D space

To address the contribution of cell shape to the parameters of ookinete movement in 3D space, disruption of parasite cytoskeleton was attempted, while leaving motor functionality unchanged. Use of microtubule-disrupting drugs to target the microtubule cytoskeleton were precluded because of the general stability of subpellicular microtubules in Apicomplexa, their non-dynamic nature and resistance to classical drugs such as colchicine and oryzalin (Russell and Sinden, 1981; Morrissette and Sibley, 2002) despite use at concentrations of up to 1 mM (Supplementary Fig. S1). As an alternative strategy we explored the role of proteins of the subpellicular network implicated in shaping the pellicular architecture of malaria parasites (Mann and Beckers, 2001). Recent knockout of IMC1h, an inner membrane complex protein in P. berghei, revealed their role in defining shape in the ookinete. Furthermore, knockout parasites gave rise to clear changes in gross cell movement (Tremp and Dessens, 2011; Volkmann et al., 2012). Confirming previous reports, imaging of the knockout parasite line in our 3D assay demonstrated that lack of IMC1h does not prevent movement, certainly not to the extent seen with inhibition of actin dynamics with CD. Instead IMC1h-KO ookinetes showed a slightly reduced average apparent speed of 7.5 ± 3.1 μm min−1 and total displacement of 28.2 ± 16.4 μm when compared to wild-type parasites (Table 1). IMC1h-KO cells did not, however, follow helical motility with their chirality decreased down to effectively random (18.8 ± 11.2%). Of most interest, and unlike CD treatment, of 39 tracks analysed with the knockout none exhibited any detectable helical motion that could be used to determine properties of chiral motion (Fig. 6A and B and Table 1). Thus, changing ookinete shape markedly altered the gross parameters of motility from chiral to linear without ablating directional motility.

Figure 6.

Absence of IMC1h ablates the parameters of P. berghei ookinete motility.

A. Reconstructed 3D tracks of IMC1h-KO ookinetes in vitro demonstrate cell motility without a helical motion path.

B. Mean parameters of IMC1h-KO parasite motility in comparison to wild-type and cytochalasin D (CD)-treated cells. Data from three independent replicates. Boxplot error bars indicate 5th to 95th percentiles with outliers shown individually.

C–E. FIB-EM of IMC1h-KO ookinetes reveals an absence in chiral shape.

F and G. Critical point dried negative stain EM comparing wild-type (F) and IMC1h-KO ookinetes (G) reveals a less organized but still twisted microtubular lattice in the knockout parasites.

The shape of ookinetes following IMC disruption is visibly much rounder than that seen in wild-type parasites (Tremp and Dessens, 2011; Volkmann et al., 2012) with mean length to width ratios of 2.1 ± 0.6 and 4.7 ± 4.6 respectively (Figs 5B and 6C). In support of the linkage between shape and chirality, whole-cell FIB-EM revealed that while an apparent curve could be detected for some parasites, no left-handed (or any handed) twist was observable in parasite reconstructions (Fig. 6C–E, Supplementary Movies S7 and S8). Attempts at electron microscopy of critical-point-dried cytoskeletons were hampered by the fragility of IMC1h-KO ookinetes to purification. Where knockout ookinetes were visible by negative stain, however, the helical lattice of the cytoskeleton was still apparent, though seemingly less organized than wild-type (Fig. 6F and G). Given that microtubules link to the underside of the IMC (Raibaud et al., 2001), the breakdown in shape observed in the knockout parasite line supports the general model linking IMC and subpellicular microtubules as the core architecture framework of an apicomplexan parasites (Morrissette and Sibley, 2002), likely with IMC recruiting microtubule rather than the reverse (Morrissette and Sibley, 2002). Confounding a clear interpretation of our results with respect to how cytoskeletal organization affects motility, IMC proteins have also been linked directly to the gliding motor complex itself (Bullen et al., 2009). Thus, the absence of chiral motion could be derived from the gross changes in ookinete shape as well as a breakdown in motor organization. However, since directional motion is still observed (IMC1h-KO still move along straight lines, Fig. 6A), the knockout parasite's lack of chiral motion strongly implies that cell shape, as determined by cytoskeletal architecture, is the primary driver of ookinete chiral motion.

Why move with helical motion?

A helical trajectory results when an organism moves with constant rotational (ω) and translational velocity (V) such that these two vectors are neither parallel nor perpendicular to each other (Crenshaw, 1996). V is always tangential to the trajectory of the forward moving object, and ω is parallel to the axis of the helix (Fig. S3). While helical motion is very commonly seen across microorganisms, it is normally associated with flagellar beats or shape changes (Jahn and Votta, 1972; Crenshaw, 1996). For the ookinete, our analyses suggest it is instead defined by an, approximately, fixed chiral shape of the parasite. This relationship between shape and motion may relax some of the perceived constraints in gliding motor organization. For example, if force is entirely sideways/lateral (Flat red arrows, Fig. S3), then parasite shape can alone still lead to progressive forward motion by the ookinete in a similar fashion to a corkscrew. Any increase in the degree of rearward force (Frear blue arrows, Fig. S3), as envisaged by current thinking of the motor (Frénal et al., 2010), would then add to the efficiency of forward movement. Thus while the actomyosin motor may still be largely rearward directed, incorporating cell shape into the mechanics of ookinete motion may relax some of the envisaged constraints on its precise organization.

There are other benefits of helical motility, which may be key evolutionary drivers for ookinete helical motion. While we cannot exclude the possibility that helical motion is a developmental constraint (i.e. independent of motility), we can consider its influence on ookinete movement by conceptualizing a parasite well inside the midgut that can either move in a helical manner or follow a straight line along the helix axis. Given the dimensions of the midgut and the helix (midgut cross-section width ∼ 800 μm, helix radius 2 μm), the exit points for both strategies will match closely. Seen like this, a true straight-line strategy would appear to be beneficial: it reaches the same exit more quickly without making extra turns. With the ookinete having to battle against digestive forces of the midgut, which activate during the first 24 h (Gass and Yeates, 1979) such a delay would not be trivial. What then are the benefits of helical motion? Foremost, chiral motion is more energy efficient than linear motion through 3D space in a viscous environment (Purcell, 1977) where the chiral shape of the parasite prevents rearward slip and provides a more energy-efficient transduction of motor force to the extracellular milieu. Helical motion is also a very good way of maintaining a straight trajectory (Jennings, 1901; Crenshaw, 1996) since the act of moving with a revolving helical axis can compensate for any external force that could influence the motile cell to deviate from a linear course (Jennings, 1901). We might therefore conclude that ookinete shape and chiral motion are beneficial for reaching the midgut epithelium both as quickly as possible and with greatest energy efficiency, while still being as close as possible to the ideal of a true straight line exit strategy.

Attempts to change viscosity parameters in the Matrigel assay here were unsuccessful (motion was ablated entirely). However, previous reports have demonstrated that ookinetes from different Plasmodium species move with different twisting properties (Freyvogel, 1966). Thus, the different vector-host combinations (and associated differences in timing of maturity with respect to blood bolus viscosity, formation and density of the peritrophic matrix or properties of host epithelium) may have selected for different ookinete cell motion properties. It would be of interest to assess the pitch differences between the ookinetes from different species to test this hypothesis. Shape-dependent left-handed helical motion through viscous space has recently also been shown for T. gondii tachyzoites using a similar Matrigel matrix environment (Leung et al., 2014). This would suggest that the features of 3D helical motion, and its underlying cellular basis, may be a common theme across apicomplexan parasites.

While rearward force is still in action when ookinete shape is changed (Fig. 6), the potential for relaxation of constraints on motor organization clearly demands that the precise biomechanics and biophysics of force are determined for a motile ookinete, and more broadly across apicomplexan parasites in general. Specifically, studies that can directly demonstrate the precise underlying organization of the myosin motor and actin filaments are now clearly needed to enable a precise understanding of the linkage between cytoskeleton, motor force and cell shape that leads to helical motion. Ultimately, refining our understanding of how parasites move through 3D space will improve strategies for developing compounds that can hinder them, either as transmission blocking drugs or as effective treatment drugs that target other stages of the life cycle. Indeed, the precise definition of parameters of motion in the context of an in vitro multi-well assay should be readily adaptable towards cellular-based drug-screening to explore specific inhibitors of ookinete motility or beyond to other motile apicomplexan parasite stages.

Experimental procedures

Parasites and mice

Four to six-week-old Swiss mice, housed at 22°C to 25°C on a 12 h light/dark cycle were treated with phenyldrazine (PHZ; 6 mg ml−1) 3 days prior to infection. Infections were carried out by intraperitonial (I.P.) inoculation using a P. berghei ANKA stain expressing green fluorescent protein (GFP) con (Franke-Fayard et al., 2004) obtained from a donor mouse between first and fourth passages from cryopreserved stock. Parasitaemia was monitored by Giemsa smear and exflagellation quantified 3 days post infection by adding a drop of blood from a tail vein to 20 μl ookinetes medium (Moon et al., 2009). Percentage of gametocytaemia and number of exflagellation events were assessed in 10 viewing fields. Infected blood was collected from mice with a parasitaemia > 4% via cardiac puncture into a heparinized syringe. Ookinete cultures were produced in vitro by culturing in 10 ml flasks using ookinete media (Moon et al., 2009) and incubated at 19°C for 18 h. All experiments were conducted in compliance with local Animal Ethics Committee requirements [Baum laboratory, Animal Ethics Committees (AEC) Project 2009-023].

Ookinete plate-based motility assays

GFPcon P. berghei ookinete cultures were allowed to settle on and invade the gel surface of 96-well imaging plates (clear bottom, black; BD Bioscience) pre-coated with Matrigel (BD Bioscience) diluted at a 1:1 ratio with ookinete medium (thus filtering out non-motile fluorescent material). These were incubated at 19°C for 1 h. For drug treatments, after incubation, inhibitors made up in DMSO [100 nM Cytochalasin D (Sigma), 1 mM Oryzalin (Sigma), 1 mM Colchicine (Sigma)] were added onto the plates and parasites were incubated at 19°C for another hour. 1% DMSO was used as the negative control for all the experiments. Imaging was performed using a line-scanning confocal LSM 5 live microscope (Zeiss) at room temperature. Fluorescence time-lapse videos were acquired using a 20×/0.8 Plan Apochromat objective. In each video, 1 frame was taken every 2 s over a z depth of 40 μm (with 2.5 μm intervals) for the total video duration of 10 min. Laser source (488 nm) was used at transmission of 5%. The microscope was controlled by Zen v.2008 software. Videos were imported to Imaris v.7.5.1 (Bitplane) for analysis. All motility assays were recorded in triplicate wells, on at least three independent occasions (blood derived from independent mouse infections). A dosage curve for cytochalasin D treatment was determined using a Live Cell Observer microscope (Zeiss) and plate-based Matrigel assay with average speed calculated (estimated only from net displacement) relative to DMSO control to derive an approximate ∼IC50 for motility inhibition.

For in vivo ookinete motility imaging, A. stephensi mosquitoes were fed with a P. berghei GFPcon infected blood meal. Eighteen hours post feed, mosquito midguts were dissected in phosphate buffer saline (PBS) and imaged in a poly-d-lysine-coated slide chamber. Imaging settings were as above using the LSM5 Live (Zeiss).

Cell tracking and data pre-processing

Imaris v.7.5.1 (Bitplane) was used for automated cell localization and tracking. Spot tracking algorithm with Brownian motion model was used with the diameter of the spot set to 5 μm. A random selection of automatically reconstructed tracks was manually verified for tracking errors. Resulting 3D co-ordinates of reconstructed tracks were exported into a Microsoft Excel file. The data were then analysed using scripts written in MATLAB v.R2012b (Supplementary Code and Data, available on request).

Tracks spanning less than 9 min (out of 10 min of total recording time) were discarded. Furthermore, only uninterrupted tracks, i.e. tracks that had no missing co-ordinates between start and end-points were considered for analysis. The Field Of View (FOV) spanned 40 μm in z-direction. For analysis, tracks with all z co-ordinates located within (2 μm; 38 μm) were considered. This was done because some ookinetes outside of the FOV along the z-direction were incorrectly detected as being located at the FOV boundary, due to the registration of out-of-focus fluorescent signal.

Parameterization of ookinete locomotion

An expanded discussion on motion path parameterization is included as Supplementary Discussion.

Apparent speed is defined as the sum of the Euclidean distances between consecutive track locations (x, y, z) divided by the duration of the track. Total displacement after 10 min is defined as the Euclidean distance between the first and the last track location. If the track spans less than 10 min (e.g. 9 min), then the distance is adjusted accordingly (e.g. multiplied by 10/9).

Chirality is the proportion of left-handed helical primitives (l-primitives), where the primitive is a sequence of four track points P(i) = (x, y, z) taken d steps apart, i.e. {P(i), P(i + d), P(i + 2d), P(i + 3d)}. These four points define three vectors A = P(i + d) – P(i), B = P(i + 2d) – P(i + d), and C = P(i + 3d) – P(i + 2d), and a cross product X = A × B. If the angle  (X, C) < π/2, then the primitive is l-primitive (Supplementary Fig. S2). For a given step d, a track with N points has N-3d primitives, and d-chirality of the track is the proportion of l-primitives. Furthermore, different steps d = 1, … , 10 were used and maximum d-chirality was noted as the track chirality.

Track period was estimated based on the Fast Fourier Transform (FFT): (i) signed differences between the x, y and z co-ordinates of subsequent locations were computed, (ii) the FFT was computed for each sequence, and frequencies corresponding to periods larger than 1/4 of the experiment duration were discarded, (iii) the frequency component with the largest magnitude was selected, and the ratio of the maximum magnitude to the mean magnitude R of all components was computed for each sequence, and (iv) the frequency that had the largest ratio was selected, and the period was computed from this frequency. However, period estimation was considered failed if ratio R for this frequency was lower than empirically defined threshold (7 in our analysis). This could happen for tracks that do not exhibit periodicity.

In the case when period estimation succeeded, radius and pitch for a track were computed by taking three point samples from the track. A sample comprises points P(i), P(i + T/2), and P(i + T), where T is the estimated track period, N is the number of points in the track, and i = 1, …, N – T. Furthermore, for sample, the radius and pitch were estimated from the point co-ordinates (Supplementary Fig. S2), and the median values of the radius and pitch were noted as the estimated radius and pitch for the track.

Ookinete tracks from in vivo imaging had a greater associated noise, likely arising from the background fluorescence deriving from the blood meal and immature sexual or asexual stages, making their precise parameterization more challenging. In general they were found to have longer helical periods. As such, the maximum step d for chirality was set to a value of 75 (in vitro was 10), while maximum allowed period and ratio threshold for period estimation were set to 1/2 of the experimental duration and 3 respectively, adjusted from in vitro observations (see above).

Mosquito oocyst distribution imaging and analysis

Anopheles stephensi mosquitoes were fed on P. berghei infected GFPcon blood meal and sorted into pipette tips either head up or head down or left unconstrained in cages. Five days post feeding midguts were dissected into PBS and imaged for oocyst distribution with a 5× objective on a Leica widefield fluorescent microscope (Leica). Images were all orientated from anterior to posterior, oocysts positions were marked using a FIJI script and frequency distributions of oocysts along this axis were calculated.

Electron microcopy (EM)

Ookinetes were produced in vitro as above and purified by nycodenz density gradient (Carter et al., 2003). Scanning EM and transmission EM were both as previously described (Sinden et al., 1987). For automated serial section using focused ion beam EM, purified ookinetes were prepared using a Glutaraldehyde/reduced osmium tetroxide/thiocarbohydrazide/OsO4 (ROTO) fixation method as described (Hanssen et al., 2013). Resin blocks were mounted on an SEM stub and placed inside the chamber of the Nova Nanolab 200 (FEI, Eindhoven, the Netherlands). Regions of interest (ROI) were located using mixed signal back scattered/secondary electrons. A 1 μm layer of platinum was deposited on top of the regions of interest and trenches cut around ROI. Data were then collected using the FEI Slice and View process with sections of 50 nm thickness. Serial sections were then re-aligned, scaled in the Y direction to account for the data acquisition at 52° angles and segmented using the IMOD package (Kremer et al., 1996).

Negative staining and CryoEM of whole pellicular complexes

Purified ookinetes were settled on a holey carbon formvar/carbon coated grid and subjected to hypotonic lysis according to a previously described method (Russell and Burns, 1984). For negative staining the ookinetes were then stained with uranyl acetate and critical point dried. For CryoEM ookinetes were plunge frozen in liquid ethane and observed under low dose condition (total electron dose of 20 e/A2). Micrographs were recorded on a Tecnai F30 (FEI, Eindhoven, the Netherlands) at 300 kV using a Ultrascan 1000 2k × 2k camera (Gatan, Pleasanton, USA).

Acknowledgements

We thank Mathieu Brochet and Oliver Billker for generously providing us with the IMC1hKO parasite line. We are grateful to the Department of Histology at Walter and Eliza Hall of Medical Research Institute for sectioning assistance. We are grateful to Friedrich Frischknecht, Naomi Morrissette and Raphael Kim for helpful discussion and critical reading of the manuscript and to Gary Ward for sharing pre-publication data. Experimental data presented here was made possible through Victorian State Government Operational Infrastructure Support and Australian Government NHMRC IRIISS. The research was directly supported by a National Health and Medical Research Council of Australia (NHMRC) Project Grant (637341 JB & GIM), a Human Frontier Science Program (HFSP) Young Investigator Program Grant (JB RGY0071/2011) and National ICT Australia (NICTA). FA is supported through an NHMRC Dora Lush Scholarship (APP1055246). JB was supported through a Future Fellowship (FT100100112) from the Australian Research Council (ARC) and is currently supported by the Wellcome Trust, through a New Investigator Award (100993/Z/13/Z). The authors declare no conflict of interest.

Ancillary