The movement of ciliary membrane proteins is directed by transient interactions with intraflagellar transport (IFT) trains. The green alga Chlamydomonas has adapted this process for gliding motility, using retrograde IFT motors to move adhesive glycoproteins in the flagella membrane. Ca2+ signalling contributes directly to the gliding process, although uncertainty remains over the mechanism through which it acts. Here, we show that flagella Ca2+ elevations initiate the movement of paused retrograde IFT trains, which accumulate at the distal end of adherent flagella, but do not influence other IFT processes. On highly adherent surfaces, flagella exhibit high-frequency Ca2+ elevations that prevent the accumulation of paused retrograde IFT trains. Flagella Ca2+ elevations disrupt the IFT-dependent movement of microspheres along the flagella membrane, suggesting that Ca2+ acts by directly disrupting an interaction between retrograde IFT trains and flagella membrane glycoproteins. By regulating the extent to which glycoproteins on the flagella surface interact with IFT motor proteins on the axoneme, this signalling mechanism allows precise control of traction force and gliding motility in adherent flagella.
Cilia and flagella are microtubule-rich organelles that extend from the surface of many eukaryote cell types and play important roles in motility and cell signalling. The elongated morphology of cilia (length 1–20 µm and diameter of 200 nm) requires specialised mechanisms to transport proteins along its length. This is achieved through the process of intraflagellar transport (IFT), in which cargo proteins required for the assembly, maintenance and sensory functions of cilia are attached to large protein complexes (IFT particles) and moved along the axoneme through the activity of microtubule motors (Pedersen and Rosenbaum, 2008). Kinesin-2 directs movement away from the cell body (anterograde), while dynein-1b (dynein 2 in mammals) mediates the return of IFT particles towards the cell (retrograde). The anterograde IFT particles are assembled into so-called trains, which move in a processive manner to the ciliary tip. Once the anterograde IFT particles reach the ciliary tip, kinesin dissociates from the IFT particle and returns to the cell body via diffusion. The diffusive return of kinesin to the cell body may play a critical role in regulating ciliary length, acting to limit the rate at which IFT particles can enter the flagellum (Chien et al., 2017; Hendel et al., 2018). IFT trains at the ciliary tip dissociate into multiple smaller trains and move back towards the cell body (Chien et al., 2017).
The import, export and movement of many ciliary proteins is determined by their interactions with IFT particles. IFT particles are composed of ∼20 proteins arranged into two sub-complexes (IFT-A and IFT-B). Proteins within the IFT-B complex have specific roles in binding to cargo proteins, including important structural components, such as tubulin and outer arm dynein (Bhogaraju et al., 2013a; Dai et al., 2018). IFT-A proteins interact with cargo proteins involved in signalling pathways, such as G-protein-coupled receptors (Mukhopadhyay et al., 2010; Picariello et al., 2019). An additional protein complex, known as the BBsome, acts as a cargo adapter and is implicated in the transport of a range of membrane-associated ciliary proteins (Liu and Lechtreck, 2018). However, improved knowledge of the factors regulating interactions between cargo proteins and IFT particles is required to better understand the mechanisms determining the movement and distribution of ciliary proteins.
There is evidence that loading and unloading of some ciliary proteins is a highly regulated process (Lechtreck, 2015). Second messengers such as Ca2+ and cAMP may also contribute to the regulation of cargo binding (Mukhopadhyay et al., 2013). For example, mice lacking the ciliary localised Ca2+-permeable ion channel PKD2L1 exhibit defects in the IFT-dependent trafficking of the Shh transcription factor Gli2 to the tip of the primary cilium (Delling et al., 2013). In Chlamydomonas, phosphorylation of the FLA8 kinesin subunit by the Ca2+-dependent protein kinase CDPK1 blocks FLA8 entry into the flagellum and promotes dissociation of kinesin from the IFT particles at the ciliary tip, suggesting a role for Ca2+ in cargo unloading (Liang et al., 2014).
Ca2+ has also been implicated in the movement of flagella membrane proteins in Chlamydomonas. An adhesive glycoprotein in the flagella membrane (FMG-1B) allows Chlamydomonas cells to adhere to substrates (Bloodgood, 1981, 2009; Bloodgood and Workman, 1984; Xu et al., 2020). Transient interactions between FMG-1B and IFT particles direct the movement of FMG-1B along the flagella, as demonstrated by the co-localisation of individual IFT trains with polystyrene microspheres moving along the flagella surface (Shih et al., 2013). This process is utilised to drive gliding motility in Chlamydomonas, where the cell moves along a surface on its adherent flagella. The motile force is provided by the retrograde movement of FMG-1B along the flagellum, which results in the flagellum pulling the cell body forward (Bloodgood, 1995, 2009). Gliding motility is therefore caused by transient associations between FMG-1B and retrograde IFT particles, representing an excellent system in which to study dynamic interactions between cargo proteins and IFT particles.
Gliding motility is regulated by Ca2+, requiring micromolar Ca2+ in the external medium (Bloodgood and Salomonsky, 1990). Bead movement is also inhibited by the absence of Ca2+ or by the presence of diltiazem, an inhibitor of voltage-gated Ca2+ channels (Bloodgood and Salomonsky, 1990). The implication that IFT motors are involved in gliding suggests that Ca2+ most likely acts to regulate the interaction between IFT and FMG-1B. Shih et al. (2013) found that chelating external Ca2+ reduced the pausing frequency of IFT trains, suggesting that Ca2+ was required for the interaction between FMG-1B and IFT particles. In contrast, Collingridge et al. (2013) found that the absence of external Ca2+ led to a substantial accumulation of IFT particles in adherent flagella, suggesting that Ca2+ acts to disrupt rather than promote the interaction between FMG-1B and the IFT particle. This was supported by simultaneous imaging of intraflagellar Ca2+ ([Ca2+]fla) and IFT using biolistically-loaded dextran-conjugated Ca2+-responsive fluorescent dyes, which showed that [Ca2+]fla elevations acted to initiate the movement of paused IFT particles.
The discrepancy between these two findings cannot easily be resolved, yet it clearly indicates that greater understanding of the interaction between [Ca2+]fla and IFT is required. In particular, the processes leading to the pausing and accumulation of IFT trains remain unclear. Direct evidence for a regulatory function for [Ca2+]fla in the interaction between FMG-1B and the IFT particle is also currently lacking. Detailed examination of the spatial and temporal organisation of Ca2+ elevations in relation to IFT events is therefore necessary, but requires a system in which flagella can be immobilised without inhibiting Ca2+ signalling. The potential requirement for Ca2+ in other aspects of IFT must also be examined.
Ca2+-dependent signalling processes also contribute to many other flagella functions in Chlamydomonas, such as changes in flagella beat and waveform during motile responses, flagella adhesion during mating, flagella excision and flagella length control (Goodenough et al., 1993; Hegemann and Berthold, 2009; Quarmby, 1996; Wheeler, 2017). A detailed study of flagella Ca2+ dynamics will help us understand how specificity is achieved for a particular signalling role. In this study, we have analysed the interactions between [Ca2+]fla and IFT in adherent Chlamydomonas flagella, using genetically encoded Ca2+ reporters targeted to the flagella. We demonstrate that intraflagellar Ca2+ elevations act to regulate the accumulation of paused retrograde IFT particles, by promoting their dissociation from the flagella membrane, but we do not find evidence for a role for [Ca2+]fla elevations in other IFT processes. We also reveal complex spatiotemporal characteristics of Ca2+ in Chlamydomonas flagella, such as high-frequency repetitive Ca2+ spiking and the presence of localised or propagating [Ca2+]fla elevations, which indicate that Ca2+ acts locally in its interaction with IFT. By regulating the interaction between IFT and FMG-1B, [Ca2+]fla elevations play an important role in modulating flagella adhesion, in addition to regulating gliding motility.
Distinct forms of paused IFT particles in Chlamydomonas flagella
We have previously observed that accumulations of paused IFT trains are associated with gliding motility in adherent flagella (Collingridge et al., 2013). However, the origin and nature of the paused IFT trains was not examined in detail. Using total internal reflection fluorescence (TIRF) microscopy of a Chlamydomonas reporter strain expressing IFT54–mScarlet (strain IFT54-MS), we found that paused IFT trains could be designated into two clear categories (Fig. 1A–C). The first of these consisted of paused anterograde IFT particles, which remain highly localised and usually only paused for a short period before continuing in an anterograde direction (Fig. 1B). Paused anterograde IFT trains have been observed to disrupt the movement of other anterograde IFT trains, but do not interfere with retrograde transport (Stepanek and Pigino, 2016). The second category of paused IFT trains was primarily observed in the distal region of the flagellum and had a longer mean pausing duration (Fig. 1C; Fig. S1A,B). The region of paused IFT trains slowly expanded in size (mean±s.e.m. maximal length of 1.81±0.35 μm, n=9) and fluorescence intensity over time, indicating that additional IFT trains continue to pause in these regions. The paused IFT trains were periodically cleared by retrograde transport, suggesting that they represent paused retrograde IFT trains (Fig. 1C). This was supported by the presence of similar distal accumulations of IFT trains in a reporter strain for the dynein light intermediate chain (D1bLIC) of cytoplasmic dynein 1b (the retrograde IFT motor) (Reck et al., 2016) (Fig. 1D), whereas similar accumulations were absent in a reporter strain for the KAP subunit of kinesin (the anterograde IFT motor) (Collingridge et al., 2013; Mueller et al., 2005). As kinesin returns to the cell body via diffusion and is not present in retrograde IFT trains (Chien et al., 2017), the distal accumulations are likely to be formed by paused retrograde IFT trains.
The diffuse nature of the distal IFT accumulations and their formation in distal regions close to the flagella tip made it difficult to observe whether they are formed directly by paused retrograde IFT trains. However, it was possible to observe how additional IFT trains contributed to these accumulations, using a fluorescence recovery after photobleaching (FRAP) approach. Flagella exhibiting clear distal IFT accumulations were selected for photobleaching. After bleaching, individual anterograde IFT trains could be observed to proceed through the distal region to reach the flagella tip (examination of the three initial anterograde trains after each bleaching event showed that 42 out of 45 anterograde IFT trains clearly reached the flagella tip, n=15 flagella) (Fig. 1E; Fig. S1C,D). Following their arrival at the flagella tip, distinct retrograde transport of these IFT trains was not observed. However, accumulations of paused IFT trains began to form in the distal region close to the flagella tip immediately after their arrival. The increase in paused IFT trains is therefore due to additional IFT trains arriving at the distal end of the accumulation, rather than anterograde IFT trains adding to the accumulation at its proximal end. As the fluorescent IFT trains accumulate close to the flagella tip, we could not clearly determine whether they had undergone remodelling into retrograde IFT trains. However, as kinesin does not contribute to distal IFT accumulations, it seems likely that these IFT trains have transitioned into retrograde IFT trains, but cannot move away from the tip due to the large number of bleached retrograde IFT trains that have already paused in the distal region. The unimpeded progression of anterograde IFT trains through the distal region is consistent with observations that anterograde and retrograde IFT trains travel on distinct microtubules within each doublet (Stepanek and Pigino, 2016).
Development of a flagella-targeted Ca2+ sensor in Chlamydomonas
To further examine the role of [Ca2+]fla elevations in regulating IFT pausing and other events, we targeted a genetically encoded Ca2+-sensitive reporter protein (G-GECO1.1) to Chlamydomonas flagella. We fused G-GECO to the C-terminus of CAH6, an abundant carbonic anhydrase that is associated with the flagella membrane (Fig. 2A) (Engel et al., 2012; Liu and Lechtreck, 2018; Mackinder et al., 2017). CAH6 shows an even distribution along the length of the flagellum, although it is more abundant in the trans- rather than the cis-flagellum (Yu et al., 2020). Using this approach, we were able to successfully target G-GECO to the flagella of Chlamydomonas strain CC-5325 (to produce strain GG-WT). TIRF microscopy of adherent flagella revealed that [Ca2+]fla elevations were associated with gliding movement. [Ca2+]fla elevations were observed in 94.8% of trailing flagella at the onset of the gliding motility (n=116), but were largely absent from leading flagella (Fig. 2B–D; Movie 1), strongly supporting previous observations of gliding-related [Ca2+]fla elevations using biolistically loaded Ca2+-responsive fluorescent dyes (Oregon Green–BAPTA–dextran; OGB) (Collingridge et al., 2013). Cells expressing CAH6–Venus did not exhibit any changes in fluorescence during gliding motility, indicating that the rapid changes in G-GECO fluorescence were not due to motion artefacts (Fig. S2).
We next examined the influence of different surface properties on flagella Ca2+ signalling. We have previously used 0.01% poly-L-lysine to promote flagella adhesion without inhibiting gliding motility (Collingridge et al., 2013). Much higher concentrations of poly-L-lysine (>1%) can completely immobilise flagella, but can also lead to deflagellation, indicating that care is required when increasing adhesion (Dentler et al., 2009; Engel et al., 2009). On non-treated glass coverslips, many cells moved excessively or lifted their flagella from the surface within a relatively short period, although a proportion remained attached throughout the imaging period (2 min). We found that [Ca2+]fla elevations in these flagella were associated primarily with movement during gliding motility (Fig. 3A). Treatment of the glass coverslip with 0.1% poly-L-lysine greatly reduced gliding motility and flagella lifting, indicating that many of the flagella were unable to overcome the increased adhesion to the surface. The immobilised adherent flagella often exhibited repetitive [Ca2+]fla elevations, with frequencies up to 0.57 Hz (Fig. 3B); 63.6% of flagella on poly-L-lysine-treated coverslips exhibited high-frequency Ca2+ elevations (greater than 0.17 Hz), compared to 8.3% of flagella on untreated coverslips (Fig. 3C). The repetitive [Ca2+]fla elevations were not associated with motility, but occurred in immobilised flagella that were strongly adhered to the poly-L-lysine-treated surface. Removing external Ca2+ strongly inhibited the repetitive [Ca2+]fla elevations, indicating that they require Ca2+ influx across the flagella membrane (Fig. 3D). Removing external Ca2+ also inhibited gliding motility, as observed previously (Bloodgood and Salomonsky, 1990; Collingridge et al., 2013). The adhesive properties of the surface therefore have an important influence on Ca2+ signalling within Chlamydomonas flagella.
[Ca2+]fla elevations coincide with the movement of paused retrograde IFT accumulations
Previously, we have demonstrated that the [Ca2+]fla elevations observed in trailing flagella during the onset of gliding motility are associated with the retrograde movement of paused IFT trains (Collingridge et al., 2013). However, flagella exhibiting extensive gliding movements are difficult to image over longer periods, preventing detailed assessment of the interactions between [Ca2+]fla elevations and IFT. To address this, we expressed G-GECO in the IFT54-MS reporter strain and imaged flagella immobilised on 0.1% poly-L-lysine-treated coverslips. Flagella exhibiting a very high frequency of [Ca2+]fla elevations (>0.25 Hz) were excluded from this initial analysis to prevent false correlations with high-frequency IFT events (e.g. entry of IFT trains occurs at 1–1.3 Hz; Wingfield et al., 2017). Regular IFT events, such as the entry of anterograde IFT trains into the flagellum, the arrival of anterograde IFT trains at the flagella tip and the departure of retrograde IFT trains from the flagella tip, did not show a close relationship with [Ca2+]fla, as they occurred both in the presence and absence of [Ca2+]fla elevations (Fig. 4A,B). We also found no evidence for a correlation between elevated [Ca2+]fla and the pausing or restarting of anterograde IFT trains. We were unable to clearly resolve the timing at which individual retrograde IFT trains paused, although it was clear that the initiation of the distal IFT accumulations occurs in periods lacking [Ca2+]fla elevations (Fig. 4A). However, the restart of paused retrograde IFT trains showed a close association with elevated [Ca2+]fla (Fig. 4A,B); 90.2% of these events coincided with the onset of a [Ca2+]fla elevation (defined as occurring within 0.5 s, n=41 events), whereas other IFT events only rarely coincided with the onset of [Ca2+]fla elevations (Fig. 4C,D).
We also examined the impact of [Ca2+]fla elevations on the velocity of IFT trains. The mean velocity of anterograde IFT trains was not influenced by elevated [Ca2+]fla, but there was a slight increase (+12.4%) in the velocity of retrograde IFT trains in the presence of elevated [Ca2+]fla (Fig. 4E). This may indicate a reduction in transient pausing of retrograde IFT trains during [Ca2+]fla elevations.
We conclude that [Ca2+]fla elevations in adherent flagella play an important role in initiating the movement of paused retrograde IFT trains. We find no evidence for a direct requirement for [Ca2+]fla elevations in other IFT processes, such as the entry and turnaround of IFT trains or the pausing of anterograde IFT trains. This suggests that rapid [Ca2+]fla elevations do not directly regulate these other IFT processes, although our analyses cannot rule out a potential regulatory role for Ca2+ via alternative mechanisms. For example, Ca2+-dependent protein kinases have been implicated in the dissociation of kinesin from IFT particles at the flagella tip during IFT turnover (Liang et al., 2014). As gradients in resting cytosolic Ca2+ can be observed in some cells, notably in polarised plant cells such as root hairs or pollen tubes (Foreman et al., 2003; Steinhorst and Kudla, 2013), we investigated whether resting [Ca2+]fla differed at the flagella tip. The median intensity of CAH6–G-GECO or CAH6–Venus (as a non-Ca2+-responsive control) did not differ along the length of the flagellum (Fig. S3A,B). We also examined cells that had been biolistically loaded with the Ca2+-responsive dye OGB and the non-Ca2+-responsive dye Texas Red dextran (TR), enabling ratiometric imaging of [Ca2+]fla. The ratio of OGB/TR was similar along the length of the flagellum, indicating that resting [Ca2+]fla is not consistently elevated at the flagella tip relative to the rest of the flagellum (Fig. S3C).
Repetitive [Ca2+]fla elevations prevent distal IFT accumulations in adherent flagella
We previously observed a correlation between the frequency of [Ca2+]fla elevations and the frequency of retrograde IFT, with retrograde IFT trains less frequent in flagella exhibiting few [Ca2+]fla elevations (Collingridge et al., 2013). This suggests that the observed differences in Ca2+ signalling between flagella on untreated and poly-L-lysine-treated surfaces (Fig. 3) may also influence the dynamics of IFT. Simultaneous observation of [Ca2+]fla and IFT showed that the movement of IFT trains was highly regular in flagella on a 0.1% poly-L-lysine-treated surface, with a high frequency of anterograde and retrograde IFT trains, corresponding to the high frequency of [Ca2+]fla elevations (Fig. 5A–C). In contrast, flagella on an untreated surface exhibited distal accumulations of paused IFT trains, and IFT appeared more disordered, with a lower frequency of anterograde and retrograde IFT trains. The accumulation of paused retrograde IFT trains likely contributes to the reduced frequency of retrograde IFT.
Examination of flagella on a 0.1% poly-L-lysine-treated surface exhibiting intermittent periods of repetitive [Ca2+]fla elevations, allowed us to observe how transitions from quiescence to high-frequency Ca2+ spiking influenced pausing of retrograde IFT. Distal accumulations of retrograde IFT trains were observed in all flagella during the quiescent period (n=10) (Fig. 5D,E; Movies 2, 3). These were rapidly dispersed at the onset of high-frequency [Ca2+]fla elevations and further retrograde IFT trains did not pause and accumulated in flagella where high-frequency [Ca2+]fla elevations persisted. The pausing and restarting of anterograde IFT trains was not affected by the transition between quiescence and rapid Ca2+ spiking (Fig. 5D,E). The results indicate that paused retrograde IFT trains accumulate in the distal region of the flagellum in the absence of [Ca2+]fla elevations and that high-frequency [Ca2+]fla elevations prevent this accumulation.
To test this hypothesis, we inhibited flagella Ca2+ signalling through the removal of external Ca2+. Paused retrograde IFT trains did not accumulate in the distal region of flagella exhibiting repetitive [Ca2+]fla elevations (Fig. 6A,B; Fig. S4). Perfusion with a Ca2+-free buffer resulted in the cessation of the [Ca2+]fla elevations within 60 s of the onset of the perfusion. The inhibition of Ca2+ signalling led to a rapid accumulation of IFT trains in the distal region of the flagella, with a 2.58±0.25-fold (mean±s.e.m.) increase in IFT20–mCherry fluorescence in this region observed 60 s after the inhibition of signalling (n=8 flagella). These observations confirm that high-frequency [Ca2+]fla elevations act to prevent paused retrograde IFT trains accumulating in the distal regions of adherent flagella.
Whereas the frequency of retrograde IFT trains rapidly decreased following the inhibition of [Ca2+]fla elevations, the frequency of anterograde IFT was not reduced initially (Fig. 6B). However, inhibition of flagella Ca2+ signalling over longer periods does lead to a reduced frequency of anterograde IFT (Collingridge et al., 2013). As removing external Ca2+ causes a substantial overaccumulation of retrograde IFT trains in adherent flagella (Collingridge et al., 2013) (Fig. S5A,B), these retrograde IFT trains may accumulate to the extent that they impede the progression of anterograde IFT trains. This conclusion is seemingly at odds with the finding that anterograde and retrograde IFT trains travel on distinct microtubules and do not collide (Stepanek and Pigino, 2016). We therefore examined the nature of these large distal IFT accumulations using transmission electron microscopy (TEM) of flat-embedded adherent flagella. After the removal of external Ca2+ for 5 min, TEM of adherent flagella revealed large accumulations of IFT particles in the distal region, close to the flagella tip (Fig. S5C). This phenotype is similar to, but distinct from, the phenotype of mutants defective in retrograde IFT, which exhibit large accumulations of IFT trains at the flagella tip (Engel et al., 2012; Pazour et al., 1999). We propose that prolonged inhibition of flagella Ca2+ signalling results in a massive accumulation of retrograde IFT trains behind the retrograde IFT trains that have already paused. In the absence of a mechanism to clear the paused retrograde IFT trains, they accumulate to an extent where they significantly impede the progress of anterograde IFT trains, even if these IFT trains move along a distinct microtubule track.
[Ca2+]fla elevations disrupt microsphere movement along the flagellum
The pausing and accumulation of retrograde IFT trains likely reflects a direct interaction between the IFT particle and adhesive glycoproteins (predominately FMG-1B) in the flagella membrane. This interaction therefore represents a mechanism through which membrane proteins in contact with a surface can be tethered to the axoneme, allowing the generation of propulsive force via the retrograde motor, cytoplasmic dynein 1b. Our results strongly suggest that Ca2+ acts by regulating this interaction, thereby modulating the propulsive force generated by adherent flagella. The interaction between FMG-1B and IFT trains can be readily visualised by following the movement of fluorescent microspheres along the flagellum (Shih et al., 2013). Through simultaneous imaging of fluorescent microspheres and IFT27–GFP, we observed that microspheres stopped moving in a particular direction when the microsphere switched to an IFT train moving in the opposite direction or reached the end of the flagellum (Fig. 7A). However, on some occasions the microspheres could be observed to dissociate from the IFT train (anterograde or retrograde) and exhibit diffusional movement in the flagella membrane. We hypothesised that these events represent a disruption of the interaction between the IFT particle and FMG-1B, which could be mediated by [Ca2+]fla elevations.
We therefore observed microsphere movements along a flagellum while simultaneously monitoring [Ca2+]fla. A total of 12 out of 25 flagella exhibiting IFT-driven microsphere movement also exhibited a [Ca2+]fla elevation during this period. In each of these flagella, the [Ca2+]fla elevation coincided directly with the cessation of microsphere movement, with the microsphere either subsequently exhibiting diffusional movement or becoming detached from the flagellum entirely (Fig. 7B–D; Movies 4, 5). We attribute the latter events to a strong attraction between the microsphere and the poly-L-lysine-treated surface. [Ca2+]fla elevations disrupted microsphere movement at any position along the entire length of the flagellum, and the effect of Ca2+ was not restricted to microspheres in the distal region (Fig. 7B). Moreover, we did not observe microspheres moving on flagella that exhibited high-frequency [Ca2+]fla elevations. We conclude that [Ca2+]fla elevations act directly to disrupt the interaction between IFT trains and FMG-1B.
[Ca2+]fla elevations have distinct spatial properties
Our findings indicate that the [Ca2+]fla elevations observed in Chlamydomonas show complex temporal patterns that directly influence the movement of IFT trains. However, it is clear that [Ca2+]fla elevations also demonstrate distinct spatial properties. In cells exhibiting lower frequency Ca2+ elevations (<0.25 Hz), 35.7% of the [Ca2+]fla elevations were restricted to either the proximal or the distal region of the flagellum (Fig. 8A,B). Moreover, 28.1% of the [Ca2+]fla elevations that spanned the length of the flagellum exhibited a substantial difference in the timing of their onset (>0.2 s) between the distal and proximal regions (Fig. 8C). Closer examination of these signalling events indicated that they resembled a Ca2+ wave that propagated along the length of the flagellum in either direction, with 43.8% propagating in a retrograde direction and 56.2% propagating in an anterograde direction. The mean rate of propagation was 28.7±4.3 μm s−1 (mean±s.e.m., n=10) (Fig. 8D).
The identification of spatially localised [Ca2+]fla elevations allowed us to determine whether Ca2+ acted in a local or global manner to initiate the movement of paused retrograde IFT trains. We used the propagating [Ca2+]fla elevations to examine whether the onset of movement of paused IFT trains in the distal region corresponded with the elevation of [Ca2+]fla in either the distal or proximal region. We found that the movement of paused retrograde IFT trains corresponded closely to the time at which [Ca2+]fla became elevated in the distal region, irrespective of whether the [Ca2+]fla wave initiated in the distal or proximal region (Fig. 8E,F). This indicates that [Ca2+]fla elevations act locally, requiring colocalisation with the paused retrograde IFT trains in order to initiate their movement.
Detachment from a surface requires external Ca2+
Recent observations indicate that the adhesive properties of Chlamydomonas flagella are highly dynamic, with blue light promoting rapid changes in flagella adhesion to a surface (Kreis et al., 2019, 2018). As light-dependent modulation of adhesion appears to involve a redistribution of FMG-1B along the flagella surface (Kreis et al., 2018), interactions between FMG-1B and IFT may also contribute to adhesion. Lifting of flagella from a surface is often initiated by axonemal bending in the non-adherent region of the flagellum, resulting in the flagellum being dragged towards the cell body so that only the tip remains adherent. We found that flagella lifting was strongly associated with [Ca2+]fla elevations, with both the GG-WT and GG-IFT54-MS strains routinely exhibiting a [Ca2+]fla elevation at the onset of each lifting event (Fig. S6A,B). Detailed examination of the timing of lifting events revealed that, in all cases, the [Ca2+]fla elevation immediately preceded the initial movement of the flagellum towards the cell body (Fig. S6C). We propose that the [Ca2+]fla elevations act to release FMG-1B from paused retrograde IFT trains, which removes resistance to the pulling force generated by axonemal bending and allows the flagellum to be drawn towards the cell body and lifted from the surface.
We therefore examined whether Ca2+-dependent removal of paused retrograde IFT trains was required for light-modulated flagella detachment. Chlamydomonas cells suspended on a micropipette lift their flagella from a surface within 30 s after removing blue light (Kreis et al., 2018). We found that removing blue light illumination from adherent IFT54-MS cells also promoted flagella detachment, with 11 out of 14 flagella lifting from the surface entirely or remaining only attached at the flagella tips within 30 s (Fig. S6D). Flagella movements prior to lifting were preceded by the removal of paused retrograde IFT trains (Fig. S6E). Note that it was not possible to measure [Ca2+]fla directly while using blue light to modulate adhesion, as G-GECO requires excitation with blue light. However, removing blue light illumination in the absence of external Ca2+ did not lead to flagella lifting (0 out of 17 cells) and paused retrograde IFT trains remained in the distal regions (Fig. S6F). The removal of external Ca2+ did not act to simply immobilise flagella, as non-adherent cells continued to actively swim in this period. Together, the results suggest that light-dependent detachment of flagella from a surface requires the Ca2+-dependent release of flagella membrane glycoproteins from paused retrograde IFT trains.
Our results help to provide a mechanistic understanding of the requirement for Ca2+ in flagella surface motility and gliding in Chlamydomonas. We previously demonstrated that [Ca2+]fla elevations are linked to the movement of paused retrograde IFT trains (Collingridge et al., 2013), although alternative roles for Ca2+ in promoting the pausing of retrograde IFT have also been proposed (Shih et al., 2013). By using improved techniques to visualise [Ca2+]fla elevations in Chlamydomonas, our results demonstrate that [Ca2+]fla elevations act to initiate the movement of paused retrograde IFT trains by disrupting an interaction between the IFT particle and flagella membrane glycoproteins. By regulating the accumulation of paused retrograde IFT motors, this process modulates the generation of motive force in individual adherent flagella. We did not find evidence for a requirement for [Ca2+]fla elevations in regulating other aspects of IFT, for example, by promoting the pausing of anterograde and/or retrograde IFT trains or influencing their velocity. Chien et al. (2017) found that the removal of external Ca2+ increased the residency of IFT trains at the flagella tip, suggesting that Ca2+ may also have a regulatory role in the assembly or departure of retrograde trains. We were not able to directly assess the turnaround of IFT trains in our analyses. However, our experiments show that retrograde IFT trains continue to accumulate in the absence of external Ca2+, indicating that IFT turnaround continues in the absence of [Ca2+]fla elevations.
These findings allow us to further develop the proposed model for gliding motility in Chlamydomonas (Bloodgood, 2009; Collingridge et al., 2013; Shih et al., 2013) (Fig. S7). When a cell first encounters a solid surface, often only the distal regions of the flagella adhere to the surface. Both flagella subsequently glide forward, which brings the entire length of each flagellum into contact with the surface. The gliding movement is driven by retrograde IFT motors engaging with FMG-1B in the flagella membrane, which adheres to the surface (Shih et al., 2013). Once the flagella become fully extended in the gliding configuration, the two flagella are arranged at 180° to each other and are pulling in opposite directions. If the traction forces generated by each flagella are balanced, neither flagellum can move forward and there is no net movement of the cell. The traction forces increase as further retrograde IFT trains engage with FMG-1B in each flagellum. When the membrane tension reaches a critical threshold in one flagellum, a Ca2+ elevation is generated, which disrupts the interaction between the retrograde IFT trains and FMG-1B, selectively disrupting the traction force in this flagellum. The trailing flagellum therefore no longer resists the force generated by the opposing flagellum (the leading flagellum), which is able to pull the cell forward along the surface.
The Ca2+-dependent regulation of the interactions between IFT and the flagella membrane should also be considered in the context of flagella adhesion. As flagella lifting requires the flagellum to be pulled towards the cell body, modulation of the traction force generated by each flagellum will influence its ability to resist this pulling force. When retrograde IFT trains engage with FMG-1B, they act to resist movement of the flagellum in the direction of the cell body. However, when not in contact with anterograde or retrograde IFT trains, FMG-1B can diffuse freely along the flagellum, as demonstrated by microsphere movements (Bloodgood et al., 2019). This allows an adherent flagellum to slide along a surface while maintaining contact with the surface. During this movement, some of the FMG-1B is shed onto the surface (Kamiya et al., 2018) (Fig. S8). As [Ca2+]fla elevations act to disengage FMG-1B from retrograde IFT trains, they allow unrestricted movement of FMG-1B along the membrane. [Ca2+]fla elevations therefore do not modify adhesion directly, but influence the ability of flagella to resist a pulling force.
[Ca2+]fla elevations on an untreated surface are primarily observed in flagella under tension, i.e. immediately prior to trailing or lifting movements. By disrupting the interaction between IFT and the flagella membrane, the [Ca2+]fla elevations act to reduce the membrane tension. On a highly adherent surface, [Ca2+]fla elevations are observed in the absence of movement, suggesting that flagella immobilisation itself causes membrane tension. Although the repetitive [Ca2+]fla elevations act to prevent the accumulation of retrograde IFT trains, in this situation the membrane tension is not relieved and the flagella remain immobilised due to the highly adherent nature of the surface.
The proposed model for gliding motility illustrates how the cell is able to coordinate interactions between retrograde IFT motors and flagella membrane glycoproteins in order to modulate the traction force in individual flagella while they are adhered to a surface. However, some important questions remain regarding the underlying molecular mechanisms. How does [Ca2+]fla act to disrupt the interaction between IFT and FMG-1B? How is the [Ca2+]fla elevation generated in a single flagellum? What mechanisms enable the generation of repetitive [Ca2+]fla elevations? These questions represent important avenues for future investigation.
The interaction between the IFT particle and FMG-1B is implied from the coordinated movement of fluorescent microspheres and IFT trains (Shih et al., 2013), but biochemical characterisation of this interaction is lacking. Recent characterisation of an fmg-1b mutant line (Bloodgood et al., 2019) supports previous observations that FMG-1B is the primary protein in the flagellum mediating contact with solid substrates (Bloodgood, 1982, 1984), although an additional flagella membrane glycoprotein, FAP113, was recently identified as interacting with microspheres (Kamiya et al., 2018). It seems likely that surface contact, which induces cross-linking of FMG-1B (Bloodgood and Salomonsky, 1998), acts to promote an interaction between FMG-1B and retrograde IFT trains, as retrograde IFT trains do not accumulate in non-adherent flagella (Collingridge et al., 2013). We propose that the increase in [Ca2+]fla likely leads to a direct conformational shift in a Ca2+-sensitive protein within the putative IFT–FMG-1B complex, disrupting the interaction. This mechanism would be analogous to the Ca2+-regulated movement of mitochondria along microtubules in neurons and other animal cell types, where the interaction between the mitochondrion and kinesin or dynein is mediated by the Ca2+-binding Rho-GTPase Miro (Saotome et al., 2008). Elevated cytosolic Ca2+ triggers a conformational change in Miro, which possesses two Ca2+-binding EF-hands, leading to the dissociation of the mitochondrion from the microtubule motor complex (Wang and Schwarz, 2009). [Ca2+]fla elevations in adherent flagella are most likely initiated by the activation of mechanosensitive ion channels in the flagella membrane. Chlamydomonas flagella contain a number of candidate ion channels that may contribute to signalling in response to changes in membrane tension (Bezares-Calderon et al., 2020; Wheeler, 2017; Yoshimura, 1996). The transient receptor potential (TRP) channel TRP11 is required for the mechanoshock response of swimming Chlamydomonas cells (Fujiu et al., 2011). Chlamydomonas flagella also possess a homologue of polycystin-2 (PKD2), which has been implicated in mechanosensation in mammalian cilia, although direct evidence for mechanosensory Ca2+ signalling in primary cilia is lacking (Delling et al., 2016; Lee et al., 2015). Chlamydomonas PKD2 localises to the flagella membrane, but is also bound to the axoneme and to extracellular glycoprotein polymers known as mastigonemes, which resemble hair-like appendages along the distal regions of the flagella (Huang et al., 2007; Liu et al., 2020). The tethering of PKD2 to mastigonemes and the axoneme supports a mechanosensory role for this ion channel in Chlamydomonas (Liu et al., 2020).
Although mechanosensitive ion channels may contribute to [Ca2+]fla elevations directly, the permeation of cations through these channels will also act to depolarise the flagella membrane, which may activate voltage-gated Ca2+ channels along the length of the flagellum. The presence of voltage-gated Ca2+ channels in Chlamydomonas flagella is well documented (Fujiu et al., 2009; Holland et al., 1996), and we have previously observed transient depolarisations in the flagella membrane during gliding motility (Collingridge et al., 2013). If the stimulus (i.e. membrane tension) persists, the voltage-gated Ca2+ channels can activate again following a refractory period, leading to a series of repetitive Ca2+ elevations. Increasing membrane tension could shorten this refractory period, increasing the frequency of the [Ca2+]fla elevations. Repetitive Ca2+ elevations generated by the activity of voltage-gated Ca2+ channels can be observed in many excitable cell types, including sperm flagella, in the continued presence of a stimulus (Kaupp et al., 2008; Kotov et al., 2011).
The presence of localised or propagating [Ca2+]fla elevations suggests that flagella Ca2+ signalling may also exhibit greater complexity. It is possible that the propagating [Ca2+]fla elevations represent simple diffusion of Ca2+ in the flagella matrix following a localised [Ca2+]fla elevation. Ca2+ elevations initiating in the cytosol can diffuse along the cilia of mammalian ependymal cells at a rate of ∼20 µm s−1 (Doerner et al., 2015). However, cytosolic Ca2+ elevations are not directly coupled to [Ca2+]fla elevations in Chlamydomonas (Bickerton et al., 2016). Moreover, Chlamydomonas flagella possess ion channels typically associated with propagating Ca2+ elevations in animal cells. Inositol triphosphate receptors (IP3Rs) typically localise to endomembranes in mammalian cells, where they contribute to fast cytosolic Ca2+ waves through Ca2+-activated Ca2+ release. A homologue of mammalian IP3Rs is present in Chlamydomonas flagella (Pazour et al., 2005), which could potentially mediate propagation of localised [Ca2+]fla elevations through Ca2+-activated Ca2+ influx.
The development of flagella-localised Ca2+-reporters in Chlamydomonas should aid the identification of ion channels responsible for Ca2+ signalling in adherent flagella. However, the nature of flagella adhesion and membrane tension will be a critical consideration for future studies of flagella Ca2+ signalling, particularly when comparing phenotypes between strains. Gliding motility is often markedly different between strains and rapid light-dependent modulation of flagella adhesion can occur within seconds in individual cells (Kreis et al., 2018). The lack of mastigonemes in pkd2 mutants indicates that loss of ion channel function may also influence the arrangement of flagella glycoproteins (Liu et al., 2020). Although mastigonemes are not thought to be involved in microsphere movements or gliding motility in Chlamydomonas (Bloodgood, 1977; Nakamura et al., 1996), they have been implicated in flagella-dependent gliding motility in Peranema (Saito et al., 2003). Thus, knockout of an ion channel could influence the processes that trigger [Ca2+]fla elevations (i.e. flagella adhesion), as well as the signalling processes themselves. Without direct measurements of the degree of adhesion and/or membrane tension in these mutant strains, it may be difficult to ascertain whether any effects on Ca2+ signalling result from direct mechanistic inhibition of [Ca2+]fla elevations or relate to indirect effects on flagella adhesion.
It is becoming clear that the nature of ciliary Ca2+ signalling differs markedly between organisms and cell types (Pablo et al., 2017). Rapid changes in flagella Ca2+ have a well-characterised role in the swimming motility of Chlamydomonas, in addition to their role in gliding motility (Holland et al., 1997). Ca2+-dependent signalling mechanisms also regulate swimming of ciliates such as Paramecium (Eckert and Brehm, 1979) and metazoan sperm (Kaupp et al., 2008). While it is likely that flagella-localised voltage-gated Ca2+ channels contribute directly to [Ca2+]fla elevations in Chlamydomonas and Paramecium (Eckert and Brehm, 1979; Fujiu et al., 2009), their role in mammalian sperm flagella are less clear, where the weakly-voltage-gated CatSper channels are primary contributors to flagella Ca2+ elevations (Lishko et al., 2012). Although CatSpers are also found in some protist lineages (e.g. glaucophytes), they are absent from Chlamydomonas (Cai et al., 2014). Furthermore, although voltage-gated Ca2+ channels are present in motile ependymal cilia of mammalian cells, ciliary Ca2+ in these cells appears to be passively coupled to [Ca2+]cyt rather than being independently controlled (Doerner et al., 2015). The nature of Ca2+ signalling in the non-motile primary cilia of mammalian cells is also highly distinct from the excitable cilia of unicellular protists (Delling et al., 2013). Therefore, although Ca2+-dependent signalling mechanisms appear to be ubiquitous in cilia and flagella, the nature of these mechanisms and their underlying molecular components differ considerably between eukaryotes.
Interactions between IFT complexes and their cargo proteins underpin many aspects of ciliary function (Bhogaraju et al., 2013b). Our results indicate that Ca2+ plays an important regulatory role in the interactions between IFT trains and flagella membrane glycoproteins in Chlamydomonas. As FMG-1B is a highly abundant protein in Chlamydomonas flagella, these transient interactions can be detected through the movement of microspheres or during gliding motility. However, it is likely that similar regulatory mechanisms direct the movement of many other flagella membrane proteins. Future biochemical characterisation of the FMG-1B–IFT complex, and in particular the identification of the Ca2+-sensitive components that mediate the response to [Ca2+]fla elevations, will help identify whether these mechanisms are conserved in other ciliated organisms.
MATERIALS AND METHODS
Strains and culture conditions
Chlamydomonas reinhardtii cells were grown in standard Tris-acetate-phosphate (TAP) medium at 21°C on a 16 h light–8 h dark cycle with a photosynthetic photon flux density of 80 μmol m−2 s−1. Wild-type strains CC-125 and CC-5325 and the IFT reporter strains D1bLIC-GFP (CC-4488) (Reck et al., 2016) and KAP–GFP [CC-4296 - fla3-1 background (Mueller et al., 2005)] strain were obtained from the Chlamydomonas Resource Centre (http://chlamycollection.org/). Chlamydomonas strains expressing CAH6–Venus and IFT27–GFP (CC-125 background) were obtained from Luke Mackinder (University of York, UK) and Joel Rosenbaum (Yale University, CT), respectively (Mackinder et al., 2017; Qin et al., 2007). IFT20–mCherry [null ift20 background (Lechtreck et al., 2009)] and the IFT54-mScarlet reporter strain (IFT54-MS) were provided by Karl Lechtreck (University of Georgia, Atlanta, GA). The IFT54-MS strain was constructed by expressing IFT54-mScarlet in an ift54-2 background (Wingfield et al., 2017). The IFT54–mScarlet vector was made by cutting out mNeonGreen from pBR25-mNG-IFT54 using XhoI and BamHI and replaced with a PCR product encoding IFT54-mScarlet using the mammalian codon usage trimmed with the same enzymes (Wingfield et al., 2017).
Development of a flagella-targeted Ca2+ sensor
The flagella-targeted Ca2+ reporter was prepared by modifying the pLM005-CAH6-Venus vector (obtained from Luke Mackinder, University of York, UK) used to express the flagella-localised carbonic anhydrase CAH6 (Mackinder et al., 2017). Codon-optimised G-GECO1.1 was synthesised (Genscript) and introduced into the pLM005-CAH6-Venus expression vector via the sites BglII and EcoRI, resulting in a C-terminal fusion of G-GECO to CAH6, separated by a short amino acid linker sequence. The GG-WT and GG-IFT54-MS strains were produced by transforming C. reinhardtii strains CC-5325 (wild type) and IFT54-MS by electroporation using a NEPA21 Super Electroporator (NepaGene, Japan) (Yamano et al., 2013). Cells were grown to a cell density of 1×107–2×107 cells ml−1. The cultured cells were collected by centrifugation (400 g, 3 min) and re-suspended in TAP media containing 40 mM sucrose to a final density of 1×108–1.5×108 cells ml−1. 1×107 cells and 350 ng of plasmid DNA (pLM005-CAH6-G-GECO construct linearized with EcoRV) were suspended in a total volume of 20–30 μl and placed into an electroporation cuvette (2 mm). The measured value of electric impedance was within 500–650 Ω. Electroporation utilised a first pulse (Pp) at 250 V with 8 ms pulse length, 50 ms pulse interval and 40% decay rates. The second pulse consisted of multiple transfer pulses (Tp) of 20 V with 50 ms pulse length, 50 ms pulse interval and 40% decay rate (two iterations). Cells were transferred into 10 ml TAP medium containing 40 mM sucrose and incubated in dim light (2–3 µmol photons m−2 s−1) for 24 h. The cells were collected by centrifugation (400 g, 3 min) and plated onto 1.5% agar TAP plate containing 10 µg ml−1 hygromycin B (Roche) and 20 µg ml−1 of paromomycin sulfate (Fisher BioReagents).
Biolistic loading of Ca2+ dyes
For experiments where flagella Ca2+ was measured using fluorescent dyes, dyes were loaded into cells using a biolistic approach (Collingridge et al., 2013). For this, 0.9 mg of 0.6 µm diameter gold microcarriers (Bio-Rad) were coated in 40 µg Oregon Green–BAPTA–dextran (10,000 molecular mass) and 24 µg Texas Red–dextran (10,000 molecular mass) (Invitrogen). Oregon Green–BAPTA is Ca2+-responsive, whereas Texas Red acts as a non-responsive reference dye. Texas Red was omitted for simultaneous imaging of Ca2+ and IFT20–mCherry. Chlamydomonas cells (strain CC-125) were harvested in mid-exponential phase by gentle centrifugation (400 g for 3 min) and resuspended in loading buffer (10 mM HEPES pH 7.4, 20 µM K+ glutamate and 50 mM sorbitol). Then, 5×106 cells were spread onto a 0.45 µm nitrocellulose membrane filter (Millipore) and loaded biolistically using a PDS-1000 delivery system (Bio-Rad) (1100 psi rupture disc). After loading, cells were washed and resuspended in TAP medium and allowed to recover for at least 2 h prior to imaging.
TIRF imaging of flagella
For all experiments, Chlamydomonas cells were suspended in a HEPES/NMG buffer consisting of 5 mM HEPES, 1 mM KCl, 1 mM HCl, 500 µM CaCl2, 200 µM EGTA (free Ca2+ 301 µM) and pH adjusted to 7.4 with N-methyl-D-glucamine (Holland et al., 1997). To remove external Ca2+, cells were perfused with a Ca2+-free buffer in which CaCl2 had been omitted. Cells were added to 35 mm glass bottom dishes (In Vitro Scientific), which in some cases were treated with 0.1% poly-L-lysine to promote flagella adhesion. TIRF microscopy was performed at room-temperature using a Nikon Eclipse Ti with 100× (1.49 NA) TIRF oil immersion objective and an EM-CCD camera (Photometrics Evolve). TIRF was achieved via through-the-lens laser illumination. Wavelength compensation was not applied. IFT20–mCherry and IFT54–mScarlet were excited using a 561 nm laser (Coherent), with emission at 575–625 nm. IFT27–GFP, Venus and G-GECO were excited using a 488 nm laser (Coherent), with emission at 500–550 nm. For two-channel imaging, simultaneous TIRF excitation was performed at 488 and 561 nm and a dual-view beam-splitter device was used to detect emission at 505–535 and 605–655 nm. Images were captured using NIS-Elements software (v3.1) at 100 ms per frame unless otherwise stated. Imaging of OGB was at 300 ms per frame. We found that dual channel imaging of G-GECO and IFT54–mScarlet led to some photobleaching of mScarlet in paused IFT trains, unless laser emission intensities were reduced. Therefore, to quantify the accumulation of paused IFT trains (Fig. 6; Fig. S4) we used Oregon Green–BAPTA in the IFT20–mCherry reporter strain, as photobleaching of paused IFT trains was not observed in these imaging conditions.
Fluorescence emission from single wavelength indicators, such as G-GECO, can be influenced by imaging artefacts such as flagella movement in the TIRF field of illumination. The use of a single emission wavelength Ca2+ indicator was necessary for simultaneous imaging of IFT processes. We therefore performed a series of validation experiments to confirm that G-GECO was a reliable reporter of flagella Ca2+ elevations as follows: (1) Rapid transient elevations in G-GECO fluorescence were not seen in the absence of external Ca2+ (Fig. 3D). (2) G-GECO has a high dynamic range, exhibiting large changes in fluorescence emission on Ca2+ binding. Similar elevations in fluorescence were never observed in cells expressing CAH6–Venus, even during gliding motility (Fig. S2), indicating that motion artefacts do not give rise to large increases in fluorescence. (3) The nature of the [Ca2+]fla elevations (e.g. duration, frequency) observed using G-GECO were very similar to those observed using ratiometric imaging of the fluorescent dyes OGB and Texas Red–Dextran (Collingridge et al., 2013). Key findings using G-GECO were also verified using OGB (e.g. Fig. S3). (4) For detailed examination of [Ca2+]fla and IFT, imaging of G-GECO was performed primarily in flagella immobilised with 0.1% poly-L-lysine to ensure that motion artefacts were minimised. (5) Dual-channel imaging of G-GECO and IFT54–mScarlet enabled visual confirmation that changes in the intensity of G-GECO fluorescence were not replicated in the IFT54–mScarlet channel and were therefore due to changes in [Ca2+]fla (Fig. S6C). This was particularly important for confirming that localised [Ca2+]fla elevations were not artefacts due to flagella movement (e.g. Fig. 7A).
Red fluorescent carboxylate-modified microspheres (0.1 μm diameter, Thermo Fisher) were used to image flagellar surface motility. Microspheres diluted in HEPES/NMG buffer were added to adherent cells and imaged by TIRF microscopy. Excitation with a 488 nm laser alone was sufficient to simultaneously image G-GECO and microspheres due to the very high fluorescence emission of the microspheres. A dual-view beam-splitter device was used to detect emission at 505–535 nm (G-GECO or IFT27-GFP) and 605–655 nm (microspheres). Flagella exhibiting microsphere movements greater than 1 µm were examined for the presence of [Ca2+]fla elevations during the course of microsphere movement.
For modulation of flagella adhesion with blue light, IFT54-MS cells were imaged by TIRF microscopy as described above, but a 488 nm laser was used to provide stimulation with blue light. Blue light was applied for 2 min to allow flagella to attach to the glass surface and then flagella lifting was examined after removing blue light for 30 s (defined as the removal of flagella from the surface, or a >50% decrease in flagella area in contact with the surface).
For imaging of flagella membrane glycoproteins, cells were stained with the fluorescent lectin concanavalin A (ConA) (100 μg ml−1) conjugated to fluorescein isothiocyanate (FITC) (Invitrogen, UK) for 5 min. Cells were then centrifuged (400 g, 1 min) and resuspended in HEPES/NMG buffer prior to TIRF imaging.
Images were smoothed using a 3×3 pixel filter (NIS elements) and kymographs were generated using ImageJ software (version 1.45 s; http://rsb.info.nih.gov/ij/). To identity [Ca2+]fla elevations, we calculated the mean pixel intensity of G-GECO within a region of interest encompassing the whole flagellum, unless stated otherwise. Distal and proximal regions of interest were defined as regions 1 μm in length at either end of the flagellum. For quantitative analysis, the baseline intensity was calculated using an asymmetric least squares smoothing algorithm (Origin Pro software, Northampton, MA) and changes in fluorescence emission were calculated using the ratio of fluorescence to the calculated baseline. Peaks were detected using Origin Pro software (peak finding method, local maximum with five local points), using a threshold value that differed from the baseline by 20%. IFT was monitored using TIRF microscopy of fluorescently tagged IFT proteins. A kymograph of 60 s duration was used to determine the mean velocity of IFT particles and the frequency at which they were observed within this time period. Entry of anterograde IFT trains was defined as the time at which the IFT train was first detected, as the region of the flagellum closest to the cell body may not be illuminated by TIRF excitation. IFT train velocity and frequency were quantified from the kymographs by measuring the slope and number of traces, respectively using ICY software (de Chaumont et al., 2012). The interaction between IFT events and [Ca2+]fla was examined by measuring relative G-GECO fluorescence coinciding with each event. To identify IFT events coinciding with the onset of [Ca2+]fla elevations, a derivative Ca2+ trace was calculated by dividing the fluorescence in each frame by the median of the three preceding frames. The onset of each [Ca2+]fla elevation was defined as the frame which displayed the greatest rate of change in fluorescence, and coinciding IFT events were defined as those events occurring within 0.5 s of this rise.
All statistical analyses were performed in Origin Pro Software (Northampton, MA). For the box plots, the box indicates the 25–75th percentiles with median, mean is the open square and whiskers represent 10–90th percentiles.
Fluorescence recovery after photobleaching
For FRAP analysis of IFT, IFT54-MS cells were observed with a Nikon Eclipse Ti E inverted fluorescence microscope, equipped with a dual View DV2 (Photometrics) to detect emission at 505–535 nm and 605–655 nm, a iLAS FRAP module (Roper Scientifics) and Hamamatsu Flash 04 LT camera. Images were acquired using Metamorph software (version 7.7, Molecular Devices). IFT54-MS cells were placed in a poly-L-lysine (0.01%) treated dish and kept at room temperature during the acquisition. A segment of a flagellum was bleached by irradiation with a 150 mW green laser (Vortran), delivered through the 100× TIRF oil objective lens (100×, APO TIRF oil immersion, NA 1,49, Nikon) used for observation and focused on the specimen. The position to be photobleached was set at 50–70% of the flagellar length from the tip. The intensity of laser beam was 30%. Laser light for photobleaching was usually irradiated for about 1 s. Images were recorded continuously for 15 s before bleaching and then recovery was monitored for 45 s by continuously recording videos with a 100 ms exposure.
Transmission electron microscopy
For chemical fixation of adherent Chlamydomonas flagella, cells were allowed to settle directly onto 0.01% poly-L-lysine-coated coverslips for 5 min. Excess cells were removed and cells were fixed with 1% glutaraldehyde in 0.1 M sodium cacodylate (pH 7.2) buffer for 10 min. Coverslips were washed three times for 5 min each in 0.1 M cacodylate buffer and then stained with 1% uranyl acetate in distilled water for 1 h at 4°C. Coverslips were washed three times for 10 min each in distilled water. After serial dehydration with ethanol solution (30%, 50%, 70%, 90% and three times at 100%), samples were embedded in Agar 100 resin (Agar Scientific). Coverslips were mounted in Agar 100 capsule and left to polymerize at 60°C for 2 days. To detach the coverslip, the sample was plunged into liquid nitrogen. First 200 nm ultrathin sections (50–70 nm) were collected in nickel grids Leica EM Uc 7 Ultramicrotome and stained with uranyl acetate (1%) and lead citrate (80 mM). Observations were made on a Jeol 1400 TEM electron microscope. Images were processed with ImageJ.
We thank Karl Lechtreck (Georgia), Joel Rosenbaum (Yale) and Luke Mackinder (York) for the supply of Chlamydomonas strains. We thank Glenn Harper and Peter Bond from the Plymouth Electron Microscopy Centre (Plymouth University, UK) for assistance in the preparation of electron micrographs.
Conceptualization: C.F., G.L.W.; Methodology: C.F., P.C., G.L.W.; Investigation: C.F., P.C., G.L.W.; Writing - original draft: G.L.W.; Writing - review & editing: C.F., C.B., G.L.W.; Visualization: G.L.W.; Supervision: C.B., G.L.W.; Project administration: C.B., G.L.W.; Funding acquisition: C.B., G.L.W.
The work was supported by a Biotechnology and Biological Sciences Research Council award to G.W. (BB/M02508X/1) and a European Research Council Advanced Grant to C.B. (ERC-ADG-670390).
Peer review history
The peer review history is available online at https://jcs.biologists.org/lookup/doi/10.1242/jcs.253492.reviewer-comments.pdf
The authors declare no competing or financial interests.