Skip to main content

Chlamydomonas fla mutants reveal a link between deflagellation and intraflagellar transport



Cilia and flagella are often lost in anticipation of mitosis or in response to stress. There are two ways that a cell can lose its flagella: resorption or deflagellation. Deflagellation involves active severing of the axoneme at the base of the flagellum; this process is defective in Chlamydomonas fa mutants. In contrast, resorption has been thought to occur as a consequence of constitutive disassembly at the tip in the absence of continued assembly, which requires intraflagellar transport (IFT). Chlamydomonas fla mutants are unable to build and maintain flagella due to defects in IFT.


fla10 cells, which are defective in kinesin-II, the anterograde IFT motor, resorb their flagella at the restrictive temperature (33°C), as previously reported. We find that in standard media containing ~300 microM calcium, fla10 cells lose flagella by deflagellation at 33°C. This temperature-induced deflagellation of a fla mutant is not predicted by the IFT-based model for flagellar length control. Other fla mutants behave similarly, losing their flagella by deflagellation instead of resorption, if adequate calcium is available. These data suggest a new model whereby flagellar resorption involves active disassembly at the base of the flagellum via a mechanism with components in common with the severing machinery of deflagellation. As predicted by this model, we discovered that deflagellation stimuli induce resorption if deflagellation is blocked either by mutation in a FA gene or by lack of calcium. Further support for this model comes from our discovery that fla10-fa double mutants resorb their flagella more slowly than fla10 mutants.


Deflagellation of the fla10 mutant at the restrictive temperature is indicative of an active disassembly signal, which can manifest as either resorption or deflagellation. We propose that when IFT is halted by either an inactivating mutation or a cellular signal, active flagellar disassembly is initiated. This active disassembly is distinct from the constitutive disassembly which plays a role in flagellar length control.


Intraflagellar transport (IFT) was first characterized in the unicellular green alga Chlamydomonas [1] and has since been shown to be required for flagellar assembly in a variety of systems [2, 3]. IFT is the bidirectional movement of large protein complexes (IFT particles) along the flagellar axoneme, and has anterograde and retrograde components mediated by the plus and minus-end directed microtubule motors kinesin-II and cytoplasmic dynein, respectively [reviewed in [4, 5]]. In Chlamydomonas, null mutations in genes necessary for activity of either kinesin-II or cytoplasmic dynein result in bald (flagella-less) cells or cells with very short, abnormal flagella [6, 7]. Retrograde IFT is not proposed to be directly involved in disassembly, but rather is necessary to recycle IFT particles [7, 8].

A model for flagellar length control has been proposed wherein anterograde IFT is required for transport of axonemal precursors to the distal tip of the flagellum; these precursors are necessary both for de novo flagellar assembly and to offset the constitutive disassembly that occurs at the tips of flagella [8]. This model suggests that the steady-state length of a flagellum is determined kinetically by the relative contributions of assembly, mediated by anterograde IFT, and disassembly at the tip, which is IFT-independent [9]. Thus, the phenotype of Chlamydomonas long flagella mutants could be a result of either an upregulation of anterograde IFT, or due to a decrease in the rate of disassembly at the tip [810].

A Chlamydomonas temperature-sensitive mutant for flagellar assembly, fla10, has been characterized as having a lesion in a subunit of kinesin-II [11]. fla10 cells have wild-type flagella at the permissive temperature (20°C), but are bald at the restrictive temperature (33°C) [12]. In agreement with the length control model, fla10 cells incubated at an intermediate temperature have intermediate-length flagella [8]. It has been accepted that the flagella of fla10 cells resorb at the restrictive temperature due to continued disassembly in the absence of anterograde IFT [e.g., [13]].

Several other temperature-sensitive flagellar assembly mutants (fla mutants) are available in Chlamydomonas [12, 14, 15]. Unlike fla10, the genes for these mutants have not yet been identified. However, like fla10, these fla mutants have been shown to have defects in IFT, even at the permissive temperature [15, 16]. The majority of the fla mutants have been reported to undergo flagellar resorption at 33°C [12, 15, 16], presumably due to defects at different points in the IFT cycle disrupting flagellar assembly. Most fla mutants are unable to regenerate flagella at 33°C, with the exception of fla2 [12]. fla2 is also exceptional in that it has been observed to deflagellate, rather than resorb, at the restrictive temperature [2, 12, 14].

Deflagellation, like IFT, is a conserved process in eukaryotic cilia and flagella [reviewed in [17]. Deflagellation/deciliation is the regulated severing of the axoneme, and has been shown to occur in response to a number of stimuli, including pH shock, 42°C heat shock, and treatment with dibucaine or alcian blue. Calcium plays a central role in signalling deflagellation: calcium influx mediates acid shock-induced deflagellation [18], and axonemal severing can be induced in vitro in response to calcium [19]. Our lab has cloned two essential components of the deflagellation pathway, the flagellar autotomy genes fa1 and fa2 [20, 21]. fa mutants do not undergo deflagellation in response to any known stimulus. We have also demonstrated that the microtubule-severing ATPase katanin is likely to mediate axonemal severing during deflagellation [19, 22]. We have localized both katanin and Fa1p to the site of deflagellation, the flagellar transition zone between the basal body and the flagellum proper [[20], M. Mahjoub and LMQ, unpublished observations].

In many ciliated cells, including vertebrate cells and Chlamydomonas, flagella/cilia are shed or resorbed prior to mitosis [2326]. It has been proposed that mammalian primary cilia are important to maintain cells in a differentiated state; the best-characterized example is the role of kidney epithelial cilia in models of polycystic kidney disease [reviewed in [27]]. Therefore, as has already been demonstrated for flagellar assembly [3, 27], genes required for flagellar resorption or deflagellation may be implicated in disease and/or development.

It is unknown what determines whether a given cell type deflagellates or resorbs prior to mitosis. Indeed, even in the same organism, flagellar loss may occur via different mechanisms at different stages of the life cycle [23]. Flagellar resorption and deflagellation have been thought to occur by dramatically different mechanisms and at different locations: resorption via disassembly at the tip [8, 13] and deflagellation by severing at the base [28]. However, a role for severing activity at the base during resorption has been suggested by elegant EM studies performed on cells resorbing their flagella prior to mitosis [29]. We now provide further evidence that flagellar resorption involves severing activity at the base, and that active disassembly by resorption is distinct from the constitutive disassembly involved in flagellar length control.

Our examinations of the phenotypes of fla10 and fla2, reported here, lead us to the conclusion that flagellar resorption of fla mutants results from active disassembly, rather than constitutive disassembly in the absence of IFT. We show that in common culture medium for Chlamydomonas, the predominant mode of flagellar loss at 33°C for fla10 is deflagellation. Blocking the ability to deflagellate, either by lowering the extracellular calcium concentration or by genetically blocking the deflagellation pathway, causes fla10 cells to resorb their flagella at the restrictive temperature. Likewise, we demonstrate that fla2 cells undergo flagellar loss via deflagellation, and that resorption occurs in low calcium or by genetically introducing a fa mutation. Furthermore, fla10-fa1 and fla10-fa2 double mutant populations are defective for resorption, as many cells retain flagella past the time when fla10 mutants are bald. Finally, we find that flagellar resorption can be induced in cells unable to deflagellate in response to deflagellation stimuli. Our findings indicate that the deflagellation and resorption pathways are not separate, but that each can result from a disassembly signal which culminates at the flagellar transition zone. We propose that IFT and flagellar disassembly share common regulatory elements.

Results and Discussion

fla10 and fla2 deflagellate at the restrictive temperature

Cultures of fla2 cells in TAP medium contain free flagella after incubation at the restrictive temperature of 33°C. Due to their small size, and tendency to stick to each other and to attached flagella, free flagella are difficult to accurately identify; however, as fla2 cells can regenerate and re-deflagellate at 33°C, the appearance of abundant free flagella is quite obvious. Our initial observations of the fla10 temperature-sensitive phenotype led us directly to the conclusion that this mutant also deflagellates, as many free flagella are seen in the presence of calcium at 33°C in both fla10 and fla2 cultures (Figure 1).

Figure 1

Free flagella in Chlamydomonas media are indicative of deflagellation. Determination of free flagella under various conditions. Free flagella observed per 100 cells were counted after 0 and 6 hours at 20°C or 33°C, in either the presence (TAP medium or HEPES+Ca) or absence (HEPES buffer) of calcium, and the difference 6 h – 0 h was calculated. Each data point is the average of at least three experiments on independent cultures.

As fla10 has only been previously characterized as resorbing flagella at 33°C, and given our knowledge of the role played by calcium in the deflagellation pathway, we reasoned that deflagellation would be prevented if fla10 cells were incubated at 33°C in buffer lacking added calcium. We found this indeed to be the case; there is no indication of deflagellation by fla10 cells at 33°C in the absence of calcium, yet cultures are still mostly bald after ~6 hours (Figures 1, 2). We extended our observations by demonstrating that fla2 cells also do not deflagellate at 33°C in the absence of calcium (Figure 1). Adding calcium to minimal buffer to a concentration approximately that of TAP media (340 μM) [30] restored the deflagellation phenotype of both fla mutants. As a further control, blocking the deflagellation response by creating double mutants of either fla10 or fla2 with either of fa1 or fa2 also prevented the appearance of free flagella after six hours (Figure 1 and data not shown). Wild-type cells do not deflagellate under these conditions.

Figure 2

fla10 and fla2 average flagellar lengths decrease during incubation at 33°C. Cells were resuspended in pre-warmed buffer at t = 0 h. At least 70 cells were examined per timepoint. wild-type, fla2, fla10. (A) Incubation in HEPES, including contribution of bald and uniflagellate cells.(B) Incubation in HEPES+Ca, including contribution of bald and uniflagellate cells.(C) The same samples as (A), but averages exclude contributions of zero-length flagella.(D) The same samples as (B), but averages exclude contribution of zero-length flagella.

Having examined the culture media under various conditions, we turned our attention to the cells themselves. The average flagellar lengths of fla10 and fla2 cells, but not wild-type cells, decrease at 33°C (Figure 2). We have shown that the fla mutants deflagellate at 33°C in the presence of added calcium, yet the differences in the average flagellar length plots are difficult to discern whether or not calcium was added, especially for fla10 (diamonds in Figure 2A,2B). This similarity of the average flagellar length plots holds whether or not zero-length flagella are included in the average length calculations (Figure 2C,2D).

To better illustrate the effects of calcium at the restrictive temperature on the fla mutants, we have chosen a novel means of presenting flagellar length data. By plotting the length of the longer flagellum versus the length of the shorter flagellum for fla10, fla2, and wild-type cells (Figures 3, 4, and 5, respectively), we can more clearly observe the states of individual cells during timecourses at the restrictive temperature. Points representing bald cells fall at the origin, while points representing uniflagellate cells are found on the x-axis. Additionally, we have plotted the percent of biflagellate, uniflagellate, and bald cells in the population for each timepoint as insets in the scatter plots. This presentation allows one to quickly assess the flagellation state of a population, and changes in that state over time.

Figure 3

Scatter plots of fla10 timecourses in HEPES and HEPES+Ca. Data shown is the same as fla10 data in Figure 2. Each flagellum from at least 70 cells was measured, and the lengths plotted as the length of the longer flagellum (in μm) on the X-axis and the length of the shorter flagellum (in μm) on the Y-axis, such that each point in a graph corresponds to a single cell (except where two points overlap, such as at the origin). Insets show the percent of biflagellate (white), uniflagellate (grey), and bald (black) cells in each sample.

Figure 4

Scatter plots of fla2 timecourses in HEPES and HEPES+Ca. See Figure 3 legend for further details.

Figure 5

Scatter plots of wild-type timecourses in HEPES and HEPES+Ca. See Figure 3 legend for further details.

Figure 3 presents timecourses for fla10 flagellar lengths at 33°C, in the absence or presence of added calcium. In both populations, cells begin with flagella of approximately equal lengths, and the distribution of flagellar lengths falls from ~8–11 μm. After one hour at the restrictive temperature, flagellar lengths of most cells in calcium remain unchanged, although a few cells now have flagella of unequal lengths. In contrast, the flagella of cells in calcium-free buffer have shortened to 5–10 μm (average length of 7.5 μm, Figure 2C).

After three hours at 33°C, cells in each population have shorter flagella, and there is an increase in the numbers of uniflagellate and bald cells in both populations. At this time in nominally calcium-free buffer, several cells with flagella shorter than 4 μm are observed. These short flagella indicate that resorption is occurring. Conversely, in the presence of calcium, no flagella <4 μm are seen, suggesting that cells deflagellate before flagellar resorption is complete. fla10 cells incubated at 20°C did not undergo significant flagellar loss or shortening, and after 6 hours at 20°C, populations resembled zero-hour timepoints (bottom panels in Figure 3).

Figure 4 is a timecourse for the fla2 mutant, which was previously reported to deflagellate at the restrictive temperature [2, 12, 14]. After 6 hours in HEPES at 33°C, but not at 20°C, over one-quarter of the fla2 cells are bald. Fewer cells with flagella >9 μm are seen after 6 hours at 33°C compared with earlier timepoints and 20°C controls. At the three hour timepoint in the presence of calcium, there is a dramatic increase in bald cells in the fla2 population (Figure 4, inset). In contrast to fla10, fla2 cells are able to regenerate flagella at the restrictive temperature [[12, 14], and data not shown]. This regeneration accounts for the increase in the number of cells with short flagella in the fla2 population at later timepoints. After overnight incubation at 33°C, fla2 cultures are often entirely bald.

Figure 5 shows the flagellar lengths of wild-type cells after a shift to 33°C. In contrast to the fla mutants, wild-type flagella do not undergo appreciable changes in length at 33°C. In principle, the resorption phenotype of fla10 at 33°C could be solely due to constitutive disassembly in the absence of anterograde IFT, and the deflagellation phenotype a secondary consequence due to the stress of elevated temperature. However, wild-type cells do not deflagellate at 33°C (Figures 1, 5), although they will deflagellate at 42°C (data not shown).

fla10-fa double mutants are slow to resorb flagella

The deflagellation phenotype of fla10 and fla2 at 33°C in calcium is blocked by either fa mutation (Figure 1 and data not shown). We wished to examine double mutant cell populations, and because fla2 is able to regenerate flagella at the restrictive temperature, we focused on fla10-fa mutants. We find that both fla10-fa1 and fla10-fa2 double mutants resorb flagella more slowly than fla10 at 33°C (Figure 6). This held true whether or not calcium was present in the medium, and, as for the fla10 single mutant, similar flagellar loss kinetics were observed regardless of calcium (Figure 3 and data not shown). This result is reminiscent of the partial block of fla10 flagellar resorption by six different extragenic suppressors [31]; it is unknown whether any of these suppressors are fa genes.

Figure 6

Double mutants of fla10 with fa1 or fa2 are slower to disassemble flagella at the restrictive temperature than fla10 single mutants. Scatter plots of 33°C timecourses for fla10, fla10-fa1 and fla10-fa2; plots prepared as described in the legend to Figure 3. TAP cultures were resuspended in pre-warmed TAP media at t = 0 h. No free flagella were seen in fla10-fa1 or fla10-fa2 cultures at any timepoint.

fla10 mutant populations are >90% bald after 6 hours at 33°C (Figures 3, 6), whereas only ~1/3 of fla10-fa cells are bald at this time (Figure 6). Moreover, at later timepoints when fla10 cells are all bald, many double mutant cells still retain flagella. Strikingly, at all timepoints, the double mutant populations are enriched in cells with unequal length flagella as well as uniflagellate cells. Resorbing populations of fla10 cells also have a few uniflagellate cells, but cells with unequal length flagella are not often observed (Figure 3). Thus, the appearance of cells with flagella of unequal length in double mutant populations correlates with an overall decrease in the resorption rate.

The prevalence of uniflagellate cells, as well as flagella of unequal lengths, is at odds with the classical picture of Chlamydomonas long-zero flagellar dynamics [8, 32]. This model predicts that cells with flagella of unequal length should be rarely seen: the combination of length-control kinetics, and the fact that the two flagella share a common pool of precursors, means that any length imbalance between the flagella of a single cell will be corrected [8]. However, long-zero experiments are typically carried out in conditions permissive for flagellar regeneration, which is not the case for fla10 mutants at the restrictive temperature. In agreement with this, fla2 cultures contain fewer uniflagellate cells than fla10 cultures at the restrictive temperature, and this is likely due to the ability of fla2, but not fla10, to reassemble flagella at the restrictive temperature.

The observation of unequal shortening of flagella in a resorbing population (Figure 6) parallels the observation that one flagellum is prone to deflagellate before the other (Figures 3, 4, 6 and data not shown). Loss of one flagellum at a time is not observed in response to a strong deflagellation signal, but is observed after treatment with weaker stimuli such as a mild acid shock (data not shown) or threshold concentrations of alcian blue [33]. The two flagella of Chlamydomonas are not equivalent; the cis flagellum is defined as the one closest to the eyespot. Rather than the random loss of either flagellum, we hypothesize that the cis and trans flagella are differentially sensitive to disassembly signals, as they are to motility-related calcium signals [34]. This hypothesis predicts that disassembly will be initiated earlier and/or proceed more rapidly in one flagellum, which could explain the abundance of unequal length flagella observed in Figure 6.

Resorption is mediated at the transition zone

On the basis of a survey of the modes of flagellar loss in unicellular algae and fungi, Bloodgood divided flagellar loss into several categories [23]. Examples were cited of the same organism (or even the same cell) undergoing flagellar loss sometimes by resorption and sometimes by deflagellation [23]. Rather than supposing that organisms undergo flagellar loss by different mechanisms at different stages of their life cycles, we contend that the mechanism of flagellar loss is conserved, and that subtle variations in signaling leads to the appearance of either deflagellation or various forms of resorption. This conserved mechanism would involve severing of the axoneme at the base of the flagellum.

We now summarize specific experimental data suggesting that resorption is mediated at the transition zone, the site of deflagellation, rather than by constitutive disassembly at flagellar tips. First, fla10 and fla2 mutant cells disassemble their flagella at the restrictive temperature via deflagellation in the presence of calcium, and via resorption in the absence of added calcium. Second, fa mutants, which are unable to deflagellate, are slow to resorb; this effect would not be predicted if resorption were entirely due to dynamics at flagellar tips. The slow resorption phenotype of fa1 is especially informative, as this mutant is slow to assemble flagella (JDKP, Ben Montpetit, LMQ, unpublished observations), in which case the length-control theory predicts that fa1 should be fast to resorb. Third, the slow resorption of fla10-fa double mutant cells produces uniflagellate cells in the absence of deflagellation, a consequence not predicted by the dynamic length control model but in accordance with the results of mild deflagellation treatments. Fourth, while Chlamydomonas cells resorb their flagella prior to mitosis [24], EM studies have provided evidence that flagella are detached from basal bodies, but not lost from cells, during pre-mitotic resorption [29]. This seeming contradiction may be explained by our proposal that resorption requires microtubule severing activity at the flagellar transition zone.

There are also some theoretical considerations. Not only the tips of the outer doublet microtubules, but rather the whole axoneme, has been shown to undergo turnover in sea urchin embryos [35]. If this turnover occurs in all eukaryotic flagella, then flagellar tip dynamics alone [8] or lattice translocation models [36] could potentially account for this turnover. However, we believe a regulated ratcheting of the axoneme at the transition zone, coupled with dynamic activity at the tip, provides the most satisfying explanation for the occurrence of axonemal turnover even while a flagellum remains functional. Additionally, there is the consideration that flagellar length in Chlamydomonas is cell-cycle dependent, and flagella undergo a period of slow resorption prior to a period of fast resorption preceding cell division [8]. We hypothesize that the slow phase of resorption is mediated by the length-control mechanism, while the fast phase of resorption is mediated by severing of axonemal microtubules in the transition zone.

The flagellar disassembly pathway

The deflagellation phenotype of fla10 is significant, as it implies an active signalling event is at work. We predicted that if the deflagellation severing complex is responsible for resorption, then providing a deflagellation stimulus to a cell unable to deflagellate should induce resorption. Indeed, this is consistent with temperature-sensitive resorption of fla10 in the absence of added calcium, and with temperature-induced resorption of fla10-fa double mutants with or without added calcium. To investigate whether this effect is more general, or only due to some special nature of the fla phenotype, we examined the effect of pH shock on mutants unable to respond by deflagellation. As previously shown, acid treatment of fa1, fa2, or adf1 mutants does not lead to deflagellation as it does for wild-type cells [37, 38]. However, as predicted by our model, these mutants do indeed resorb their flagella within one hour after a 30 s acid shock (Figure 7). This resorption is not necessarily complete, and is complicated by the tendency of the acid-treated fa cells to coil their flagella starting from the distal ends. These coiled flagella get smaller over time, and before disappearing entirely they become dense, stumpy structures. Sanders and Salisbury noted that the Chlamydomonas centrin mutant, vfl-2, will sometimes resorb rather than deflagellate in response to the deflagellation agent, dibucaine [39]. We have further extended these results by performing deflagellation experiments on wild-type cells in low-calcium buffer. Acid shock, dibucaine treatment, and 42°C heat shock all induce flagellar resorption of wild-type cells in low calcium buffer (data not shown).

Figure 7

Acid shock causes resorption of mutants unable to deflagellate. At the indicated times post-acid shock, flagellar length distributions were determined and percents of cells with long flagella (flagella longer than 7 μm) were plotted.

We conclude that resorption and deflagellation both may result from a "flagellar disassembly" signal. If the fast phase of flagellar resorption results from disassembly mediated by the severing complex at the transition zone, as we have argued, then a new picture of deflagellation emerges: calcium-mediated hyperactivation of the severing complex following a disassembly signal leads to deflagellation. This model exposes our lack of understanding of the endogenous signaling pathways that lead to flagellar disassembly. Flagellar disassembly occurring prior to mitosis or meiosis in Chlamydomonas must occur via resorption, even in medium containing calcium, as cultures typically contain few free flagella. If agents such as intracellular acidification, dibucaine, and heat shock induce deflagellation by hyperactivation of an endogenous disassembly pathway by causing an increase in intracellular calcium, then why should similar treatments in low calcium cause resorption? Two nonexclusive possibilities present themselves: either the severing apparatus has progressively greater activity at higher calcium thresholds, and has partial activity sufficient to mediate resorption without full calcium activation; or there is a calcium-independent signaling pathway which is induced by treatments such as intracellular acidification.

A candidate for providing such a signal is the IFT pathway. Recent work has suggested that IFT has signaling functions [40], and it has been suggested that these signalling functions are perhaps more important for flagellar assembly than the physical transport of flagellar components [5]. Halting IFT in the presence of calcium induces deflagellation, as we have shown with the IFT mutant fla10, in which IFT halts quickly after shift to the restrictive temperature [41]. fla10 and fla2 are not the only IFT mutants which deflagellate; we have observed deflagellation at the restrictive temperature for several other fla mutants (data not shown). As most fla mutants have defects at some point in the IFT cycle at the permissive temperature [16], it is likely that IFT is disrupted in these mutants at the restrictive temperature. As first mentioned anecdotally by Kozminski et al. [41], halting IFT seems to lead to deflagellation.

As IFT is so intimately involved in flagellar assembly, it should not come as a surprise that it may play a role in flagellar disassembly. It is intuitive that a cell should not attempt to continue building a flagellum at a time when it is actively disassembling a flagellum, and this logic suggests that signalling events that regulate IFT should be related to flagellar disassembly signals. Deflagellation of fla10 at the restrictive temperature, when anterograde IFT is halted, raises the possibility that functional IFT counteracts a constitutive disassembly signal. This could be adaptive. For example, for cells with damaged flagella, deflagellation would be the favored disassembly response, due to its speed and ability of Chlamydomonas to upregulate genes required for flagellar assembly post-deflagellation. If deflagellation is blocked, flagellar disassembly will instead occur via resorption.


We find that temperature-sensitive flagellar loss in the Chlamydomonas IFT mutants fla10 and fla2 is not due to constitutive resorption at flagellar tips, which plays a crucial role in flagellar length control, but rather due to activation of a disassembly pathway (Figure 8). We also find that flagellar disassembly can occur either by deflagellation or resorption in response to the same stimuli, and that deflagellation is preferred if sufficient calcium is available. Mutants unable to deflagellate are also slow to resorb flagella. We propose that resorption is actively mediated in the transition zone at the base of the flagellum, and that cellular signals which regulate IFT may also regulate flagellar disassembly.

Figure 8

Flagella: to have or to have not. Model for the co-regulation of flagellar assembly (mediated by IFT) and active flagellar disassembly by a common signal, X. Under conditions either permissive or nonpermissive for flagellar assembly, IFT and disassembly are proposed to be mutually antagonistic. Under conditions appropriate for flagellar assembly (Yes), the decision is made to activate IFT and block disassembly at the transition zone. Active IFT could provide a signal to inhibit active disassembly. When flagella are to be disassembled (No), IFT is inactivated. In the absence of IFT, an inhibitory signal would be removed, allowing disassembly to proceed. There may also be direct activation of disassembly.



Chlamydomonas reinhardtii mutants fla2 (CC-1390) and fla10-1 (CC-1919) were provided by the Chlamydomonas Genetics Center. Wild-type strain B214 was provided by Dr. G. Pazour (University of Massachusetts). The fa1-1 mutant was isolated by R.A. Lewin [42]; the fa2-1 and adf1-5 mutants were isolated in our lab [38]. Genetic crosses to obtain the double mutants fla10-fa1-1, fla10-fa2-1, fla2 - fa1-1, and fla2 - fa2-1 were performed by standard techniques [30]. All cells were maintained on TAP (Tris-Acetate-Phosphate) media [30] under constant illumination at 20°C.

Since Chlamydomonas cells transiently resorb their flagella after resuspension in HEPES buffer (10 mM HEPES-KOH, pH 7.2) (with or without added calcium), cultures were incubated overnight in HEPES prior to HEPES experiments. No chelators were used in the preparation of low-calcium HEPES buffer as trace amounts of calcium are required for cell viability over the length of the experiments.

Timecourses and flagella length measurements

Cells were resuspended at 3 × 106 cells/mL in buffer or media, pre-warmed to the temperature of the incubation, at time zero. We find that the flagellar loss phenotypes of fla10 are very temperature-sensitive, and a 1°C temperature difference can have a large effect on the kinetics of the experiment; this likely accounts for varying reports on the time required for fla10 cultures to become bald. Thus, the same culture of cells was used for both +/- calcium at each temperature. Samples were fixed in 2% gluteraldehyde for flagellar length measurements and free flagella determinations. Cells were examined under DIC on an Olympus IX70 microscope (Carsen Group Inc., Ontario, Canada) and lengths of both flagella on at least 70 cells were measured using software provided with the DeltaVision system (Applied Precision, Seattle, Washington). All experiments were repeated on at least three independent cultures.


  1. 1.

    Kozminski KG, Johnson KA, Forscher P, Rosenbaum JL: A motility in the eukaryotic flagellum unrelated to flagellar beating. Proc Natl Acad Sci USA. 1993, 90: 5519-5523.

    PubMed Central  CAS  Article  PubMed  Google Scholar 

  2. 2.

    Cole DG, Diener DR, Himelblau AL, Beech PL, Fuster JC, Rosenbaum JL: Chlamydomonas kinesin-II-dependent intraflagellar transport (IFT): IFT particles contain proteins required for ciliary assembly in Caenorhabditis elegans sensory neurons. J Cell Biol. 1998, 141: 993-1008. 10.1083/jcb.141.4.993.

    PubMed Central  CAS  Article  PubMed  Google Scholar 

  3. 3.

    Pazour GJ, Dickert BL, Vucica Y, Seeley ES, Rosenbaum JL, Witman GB, Cole DG: Chlamydomonas IFT88 and its mouse homologue polycystic kidney disease gene tg737 are required for assembly of cilia and flagella. J Cell Biol. 2000, 151: 709-718. 10.1083/jcb.151.3.709.

    PubMed Central  CAS  Article  PubMed  Google Scholar 

  4. 4.

    Rosenbaum JL, Witman GB: Intraflagellar transport. Nat Rev Mol Cell Biol. 2002, 3: 813-825. 10.1038/nrm952.

    CAS  Article  PubMed  Google Scholar 

  5. 5.

    Cole DG: The intraflagellar transport machinery of Chlamydomonas reinhardtii. Traffic. 2003, 4: 435-442. 10.1034/j.1600-0854.2003.t01-1-00103.x.

    CAS  Article  PubMed  Google Scholar 

  6. 6.

    Matsuura K, Lefebvre PA, Kamiya R, Hirono M: Kinesis-II is not essential for mitosis and cell growth in Chlamydomonas. Cell Motil Cytoskel. 2002, 52: 195-201. 10.1002/cm.10051.

    CAS  Article  Google Scholar 

  7. 7.

    Pazour GJ, Wilkerson CG, Witman GB: A dynein light chain is essential for the retrograde particle movement of intraflagellar transport (IFT). J Cell Biol. 1998, 141: 979-992. 10.1083/jcb.141.4.979.

    PubMed Central  CAS  Article  PubMed  Google Scholar 

  8. 8.

    Marshall WF, Rosenbaum JL: Intraflagellar transport balances continuous turnover of outer doublet microtubules: implications for flagellar length control. J Cell Biol. 2001, 155: 405-414. 10.1083/jcb.200106141.

    PubMed Central  CAS  Article  PubMed  Google Scholar 

  9. 9.

    Marshall WF: Size control in dynamic organelles. Trends Cell Biol. 2002, 12: 414-419. 10.1016/S0962-8924(02)02341-3.

    CAS  Article  PubMed  Google Scholar 

  10. 10.

    Berman SA, Wilson NF, Haas NA, Lefebvre PA: A novel MAP kinase regulates flagellar length in Chlamydomonas. Curr Biol. 2003, 13: 1145-1149. 10.1016/S0960-9822(03)00415-9.

    CAS  Article  PubMed  Google Scholar 

  11. 11.

    Vashishtha M, Walther Z, Hall JL: The kinesin-homologous protein encoded by the Chlamydomonas FLA10 gene is associated with basal bodies and centrioles. J Cell Biol. 1994, 126: 175-188.

    Article  PubMed  Google Scholar 

  12. 12.

    Adams GMW, Huang B, Luck DJL: Temperature-sensitive assembly-defective flagella mutants of Chlamydomonas reinhardtii. Genetics. 1982, 100: 579-586.

    PubMed Central  CAS  PubMed  Google Scholar 

  13. 13.

    Vale RD: The molecular motor toolbox for intracellular transport. Cell. 2003, 112: 467-480.

    CAS  Article  PubMed  Google Scholar 

  14. 14.

    Huang B, Rifkin MR, Luck DJL: Temperature-sensitive mutations affecting flagellar assembly and function in Chlamydomonas reinhardtii. J Cell Biol. 1977, 72: 67-85.

    CAS  Article  PubMed  Google Scholar 

  15. 15.

    Piperno G, Siuda E, Henderson S, Segil M, Vaananen H, Sassaroli M: Distinct mutants of retrograde intraflagellar transport (IFT) share similar morphological and molecular defects. J Cell Biol. 1998, 143: 1591-601. 10.1083/jcb.143.6.1591.

    PubMed Central  CAS  Article  PubMed  Google Scholar 

  16. 16.

    Iomini C, Babaev-Khaimov V, Sassaroli M, Piperno G: Protein particles in Chlamydomonas flagella undergo a transport cycle consisting of four phases. J Cell Biol. 2001, 153: 13-24. 10.1083/jcb.153.1.13.

    PubMed Central  CAS  Article  PubMed  Google Scholar 

  17. 17.

    Quarmby LM: Cellular deflagellation. Int Rev Cytology. 2003,

    Google Scholar 

  18. 18.

    Quarmby LM: Ca2+ influx activated by low pH in Chlamydomonas. J Gen Physiol. 1996, 108: 351-361.

    CAS  Article  PubMed  Google Scholar 

  19. 19.

    Lohret TA, McNally FJ, Quarmby LM: A role for katanin-mediated axonemal severing during Chlamydomonas deflagellation. Mol Biol Cell. 1998, 9: 1195-1207.

    PubMed Central  CAS  Article  PubMed  Google Scholar 

  20. 20.

    Finst RJ, Kim PJ, Griffis ER, Quarmby LM: Fa1p is a 171 kDa protein essential for axonemal microtubule severing in Chlamydomonas. J Cell Sci. 2000, 113: 1963-1971.

    CAS  PubMed  Google Scholar 

  21. 21.

    Mahjoub MR, Montpetit B, Zhao L, Finst RJ, Goh B, Kim AC, Quarmby LM: The FA2 gene of Chlamydomonas encodes a NIMA family kinase with roles in cell cycle progression and microtubule severing during deflagellation. J Cell Sci. 2002, 115: 1759-1768.

    CAS  PubMed  Google Scholar 

  22. 22.

    Lohret TA, Zhao L, Quarmby LM: Cloning of the Chlamydomonas p60 katanin and localization to the site of outer doublet severing during deflagellation. Cell Motil Cytoskel. 1999, 43: 221-231. 10.1002/(SICI)1097-0169(1999)43:3<221::AID-CM5>3.3.CO;2-5.

    CAS  Article  Google Scholar 

  23. 23.

    Bloodgood RA: Resorption of organelles containing microtubules. Cytobios. 1974, 9: 143-161.

    Google Scholar 

  24. 24.

    Cavalier-Smith T: Basal body and flagellar development during the vegetative cell cycle and the sexual cycle of Chlamydomonas reinhardii. J Cell Sci. 1974, 16: 529-556.

    CAS  PubMed  Google Scholar 

  25. 25.

    Rieder CL, Jensen CG, Jensen LCW: The resorption of primary cilia during mitosis in a vertebrate (PtK)1 cell line. J Ultrastr Res. 1979, 68: 173-185.

    CAS  Article  Google Scholar 

  26. 26.

    Tucker RW, Pardee AB: Centriole ciliation is related to quiescence and DNA synthesis in 3T3 cells. Cell. 1979, 17: 527-535.

    CAS  Article  PubMed  Google Scholar 

  27. 27.

    Pazour GJ, Witman GB: The vertebrate primary cilium is a sensory organelle. Curr Opin Cell Biol. 2003, 15: 105-10. 10.1016/S0955-0674(02)00012-1.

    CAS  Article  PubMed  Google Scholar 

  28. 28.

    Lewin RA, Lee KW: Autotomy of algal flagella: electron microscope studies of Chlamydomonsa (Chlorophyceae) and Tetraselmis (Prasinophyceae). Phycologia. 1985, 24: 311-316.

    Article  Google Scholar 

  29. 29.

    Johnson UG, Porter KR: Fine structure of cell division in Chlamydomonas reinhardi basal bodies and microtubules. J Cell Biol. 1968, 38: 403-425.

    PubMed Central  CAS  Article  PubMed  Google Scholar 

  30. 30.

    Harris EH: The Chlamydomonas Sourcebook. Berkeley: Academic Press. 1989

    Google Scholar 

  31. 31.

    Lux FG, Dutcher SK: Genetic interactions at the FLA10 locus: suppressors and synthetic phenotypes that affect the cell cycle and flagellar function in Chlamydomonas reinhardtii. Genetics. 1991, 128: 549-561.

    CAS  PubMed  Google Scholar 

  32. 32.

    Rosenbaum JL, Moulder JE, Ringo DL: Flagellar elongation and shortening in Chlamydomonas. J Cell Biol. 1969, 41: 600-619.

    PubMed Central  CAS  Article  PubMed  Google Scholar 

  33. 33.

    Evans JH, Keller LR: Receptor-mediated calcium influx in Chlamydomonas reinhardtii. J Euk Microbiol. 1997, 44: 237-245.

    CAS  Article  Google Scholar 

  34. 34.

    Kamiya R, Witman GB: Submicromolar levels of calcium control the balance of beating between the two flagella in demembranated models of Chlamydomonas. J Cell Biol. 98: 97-107.

  35. 35.

    Stephens RE: Synthesis and turnover of embryonic sea urchin ciliary proteins during selective inhibition of tubulin synthesis and assembly. Mol Biol Cell. 1997, 8: 2187-2198.

    PubMed Central  CAS  Article  PubMed  Google Scholar 

  36. 36.

    Stephens RE: Preferential incorporation of tubulin into the junctional region of ciliary outer doublet microtubules: a model for treadmilling by lattice dislocation. Cell Motil Cytoskel. 2000, 47: 130-140. 10.1002/1097-0169(200010)47:2<130::AID-CM4>3.0.CO;2-0.

    CAS  Article  Google Scholar 

  37. 37.

    Quarmby LM, Hartzell HC: Two distinct calcium-mediated signal transduction pathways can trigger deflagellation in Chlamydomonas reinhardtii. J Cell Biol. 1994, 124: 807-15.

    CAS  Article  PubMed  Google Scholar 

  38. 38.

    Finst RJ, Kim PJ, Quarmby LM: Genetics of the deflagellation pathway in Chlamydomonas. Genetics. 1998, 149: 927-936.

    PubMed Central  CAS  PubMed  Google Scholar 

  39. 39.

    Sanders MA, Salisbury JL: Centrin plays an essential role in microtubule severing during flagellar excision in Chlamydomonas reinhardtii. J Cell Biol. 1994, 124: 795-805.

    CAS  Article  PubMed  Google Scholar 

  40. 40.

    Pan J, Snell WJ: Kinesin-II is required for flagellar sensory transduction during fertilization in Chlamydomonas. Mol Biol Cell. 2002, 13: 1417-26. 10.1091/mbc.01-11-0531.

    PubMed Central  CAS  Article  PubMed  Google Scholar 

  41. 41.

    Kozminski KG, Beech PL, Rosenbaum JL: The Chlamydomonas kinesin-like protein FLA10 is involved in motility associated with the flagellar membrane. J Cell Biol. 1995, 131: 1517-1527.

    CAS  Article  PubMed  Google Scholar 

  42. 42.

    Lewin RA, Burrascano C: Another new kind of Chlamydomonas mutant, with impaired flagellar autotomy. Experimentia. 1983, 39: 1397-1398.

    Article  Google Scholar 

Download references


We thank Doug Cole for directing our interest towards fla2; Arden Ma for initial analysis of the fla2 deflagellation phenotype in our lab; Elizabeth Harris and the Chlamydomonas Genetics Center for strains; our colleagues at SFU for illuminating discussions; and an anonymous reviewer for several helpful remarks. JDKP thanks Rosemary Redfield for inspiration. This work was funded by the Natural Sciences and Engineering Research Council (NSERC, RGPIN 227132).

Author information



Corresponding author

Correspondence to Lynne Marie Quarmby.

Additional information

Authors' Contributions

JDKP carried out all experiments described in this work and drafted the manuscript. LMQ assisted in the design of the study, analysis of the data, and finalization of the manuscript.

Authors’ original submitted files for images

Rights and permissions

Reprints and Permissions

About this article

Cite this article

Parker, J.D.K., Quarmby, L.M. Chlamydomonas fla mutants reveal a link between deflagellation and intraflagellar transport. BMC Cell Biol 4, 11 (2003).

Download citation


  • Restrictive Temperature
  • Cytoplasmic Dynein
  • Dibucaine
  • Unequal Length
  • Intraflagellar Transport