The axonemal central pair (CP) are non-centrosomal microtubules critical for planar ciliary beat. How they form, however, is poorly understood. Here, we show that mammalian CP formation requires Wdr47, Camsaps, and microtubule-severing activity of Katanin. Katanin severs peripheral microtubules to produce central microtubule seeds in nascent cilia. Camsaps stabilize minus ends of the seeds to facilitate microtubule outgrowth, whereas Wdr47 concentrates Camsaps into the axonemal central lumen to properly position central microtubules. Wdr47 deficiency in mouse multicilia results in complete loss of CP, rotatory beat, and primary ciliary dyskinesia. Overexpression of Camsaps or their microtubule-binding regions induces central microtubules in Wdr47−/− ependymal cells but at the expense of low efficiency, abnormal numbers, and wrong location. Katanin levels and activity also impact the central microtubule number. We propose that Wdr47, Camsaps, and Katanin function together for the generation of non-centrosomal microtubule arrays in polarized subcellular compartments.
Microtubules (MTs) are organized into different arrays as cytoskeletons of subcellular structures such as the spindle, neurites, and cilia and as tracks for MT-based molecular motors dynein and kinesin1,2,3,4. Although the centrosome functions as a major MT-organizing center (MTOC) in most animal cells, non-centrosomal MTs also widely exist and are organized into unique arrays in certain cell types or subcellular compartments5,6,7. For instance, non-centrosomal MTs are constructed into parallel arrays perpendicular to the tissue plane in epithelial cells by anchoring their minus ends to adapters at the apical membrane domain8,9. They also form unidirectional and bidirectional bundles respectively in axons and dendrites following neuronal polarization1. Recently, calmodulin-regulated spectrin-associated proteins (Camsaps) have been found to stabilize free MT minus ends through direct binding to facilitate the rapid growth of the MT plus ends10,11,12,13,14. They function in the organization of non-centrosomal MT arrays in epithelial and neuronal cells15,16,17,18,19.
The majority of motile cilia, e.g. those on the surface of mammalian trachea and ependyma or forming the tail of sperms, contain a “9 + 2”-type axoneme with a pair of non-centrosomal central (C1; C2) MTs surrounded by nine MT doublets extended from the basal body20,21. Such a central pair (CP) of MTs are positioned over the center of the transition zone, with their plus ends pointing to the ciliary tip22,23,24. They are interconnected by bridges constituted by proteins such as Spag16 and coated with distinct repetitive arrays of proteinous projections. The resultant supramolecular structure, the CP apparatus, contacts directly with radial spokes emanated from peripheral MT doublets to coordinate axonemal dynein activities23,24,25. Tracheal and ependymal cilia beat in a back-and-forth, or planar, manner. Their loss of CP or CP-associated proteins, such as the C1-associated Spag6 or C2-associated Hydin, results in an abnormal beat pattern and in humans contributes to primary ciliary dyskinesia (PCD)3,21,26,27,28,29,30.
Centrosomal MTs are nucleated from and stabilized at their minus ends mainly by the γ-tubulin ring complex2,31. Usually, non-centrosomal MTs use MTs released from the centrosome as “seeds”5,6. Cilium, however, is a subcellular compartment gated by the transition zone32,33. While tubulin dimers are found to enter cilia through the intraflagellar transport (IFT) machinery, no evidence suggests that cytoplasmic MTs can pass the transition zone34,35. How the initial seeds of the central MTs are produced is thus an outstanding question. Furthermore, although we have previously reported that the mammalian CP formation requires Spef1-mediated MT stabilization in cilia36, how the number and the position of the central MTs are precisely controlled is still unknown.
In this work, we demonstrate that the WD40 repeat-containing Wdr47 (also called Nemitin)15,37, Camsaps, and the MT-severing enzyme Katanin12,38,39,40, co-operate to achieve the initial central MT formation in mammalian multicilia. Katanin produces central MT seeds by severing the peripheral MTs. Wdr47 concentrates Camsaps into the central lumen, where Camsaps stabilize the minus ends of the seeds to allow central MT elongation. As emerging evidence suggests that Wdr47, Camsaps, and Katanin also similarly impact neuronal polarization and axonal growth15,16,18,41,42, our findings indicate that the same pathway is used to properly generate and organize non-centrosomal MT arrays in polarized subcellular compartments such as the axon and motile cilium.
Wdr47 is a CP-associated protein implicated in CP MT formation
Data mining in our cDNA array results43 and subsequent immunoblotting indicated that Wdr47 (Fig. 1a) was upregulated during multiciliation of mouse tracheal epithelial cells (mTECs) cultured at an air-liquid interface (ALI) (Fig. 1b). Wdr47 was highly expressed in mouse tissues abundant in the 9 + 2 type of cilia, such as the lung, the testis, the ependyma, and the oviduct (Fig. 1c). Consistently, immunostaining of cultured mouse ependymal cells (mEPCs) revealed a ciliary-shaft localization of Wdr47 in multicilia (Fig. 1d). Interestingly, Wdr47 was highly concentrated in short cilia, especially at the ciliary tip. Its ciliary-tip intensities declined following ciliary elongation, accompanied with the emergence of Wdr47-positive puncta along and especially at the bottom of the ciliary shaft above ciliary transition zone (TZ), when Cep162, a protein at the bottom region of TZ44, was used as marker (Fig. 1d)45. By contrast, Wdr47 was not detected in the shaft of primary cilium (Supplementary Fig. 1).
Super-resolution microscopy revealed that the ciliary Wdr47 was distributed at the CP region when Hydin23,28,29 was used as CP marker, with its bottommost distribution preceding that of Hydin (Fig. 1e). Interestingly, in short cilia decorated strongly with Wdr47, Hydin was sometimes weak or undetectable (Fig. 1e), suggesting that central MTs are either not yet formed or still in initial production stages. In such cilia, however, Wdr47 was still concentrated in the central lumen of axonemes in addition to its tip accumulation (Fig. 1e). When we pre-extracted the cells with Triton X-100 to remove soluble proteins prior to fixation, Wdr47 became undetectable in short cilia but still remained on CP in long cilia (Fig. 1e). Therefore, Wdr47 is a previously undocumented CP-associated protein preferentially enriched at the minus-end region of CP. More importantly, as CP MTs in Chlamydomonas are initially assembled at the ciliary distal region46, the strong enrichment of Wdr47 in short cilia lacking Hydin strongly implies a role in early stages of CP formation.
Wdr47 deficiency in mice abolishes CP formation
We generated Wdr47-deficient mice by crossing Wdr47 knockout-first (Wdr47Kof/+) mice with EIIa-Cre mice (Fig. 1f)15 and analyzed the ciliary motility of cultured mEPCs36. Comparing to the back-and-forth beat pattern of the Wdr47+/+ and Wdr47+/− multicilia, the Wdr47−/− multicilia moved in a rotatory manner but with similar frequency (Fig. 1g and Supplementary Movie 1). When fluorescent beads were added to the culture medium, the beating Wdr47+/+ or Wdr47+/− cilia drove rapid directional flows of the beads (Fig. 1h). The rotatory Wdr47−/− cilia, however, failed to do so (Fig. 1h).
To clarify whether the rotatory pattern of the Wdr47−/− multicilia was due to loss of the central MTs26,36, we examined the ciliary ultrastructure by transmission EM. While multicilia of Wdr47+/+ or Wdr47+/− mEPCs contained normal 9 + 2 axonemes, those of Wdr47−/− mEPCs completely lacked both CP MTs (Fig. 1i). Sometimes electron-dense materials were observed in the central lumen of Wdr47−/− cilia (Fig. 1i), similar to CP-free flagella of some Chlamydomonas mutants47,48. When ciliary cross-sections (n = 126) were classified into proximal ones, based on the presence of surrounding microvilli49,50, and distal ones, the luminal materials were observed in 71% of the distal sections and 23% of the proximal ones, possibly due to remnants of CP components. EM analyses indicated that Wdr47−/− respiratory multicilia were also CP-less (Supplementary Fig. 2). Wdr47 is thus essential to the CP MTs formation.
Wdr47 is critical for both ciliary localization of CP proteins and CP maintenance
We observed that the ciliary localizations of multiple CP proteins, including CP MTs-associated Spef1, C2 MT-associated Hydin, C1 MT-associated Spag6, and C1-C2 bridge-associated Spag16 (Fig. 2a and Supplementary Fig. 3)23,36,51, were abolished or markedly reduced in Wdr47−/− mEPCs, whereas Rsph4a, a radial spoke component49,52, was not affected (Fig. 2b and Supplementary Fig. 3). To further corroborate this, we purified multicilia from cultured Wdr47+/+ and Wdr47−/− mEPCs and performed label-free quantitative (LFQ) proteomic analysis53. In addition to Wdr47, 10 CP proteins were hit in the wild-type cilia. Their levels declined by at least 3.7-fold in the Wdr47−/− cilia (Fig. 2c, d). By contrast, subunits of intraflagellar transport (IFT) complexes A and B4 were either unchanged or only reduced by <2-fold (Fig. 2c, d). Therefore, CP proteins require Wdr47 for their ciliary localization.
To further confirm the importance of Wdr47 in CP formation, we performed rescue experiments by expressing GFP-tagged Wdr47 or Centrin1 (negative control) into Wdr47−/− mEPCs. GFP-Wdr47 entered the Wdr47−/− multicilia and restored the ciliary localization of CP proteins (Fig. 2e and Supplementary Fig. 4). By contrast, the CP proteins still displayed no or weak ciliary localization in the cells expressing Centrin1-GFP (Fig. 2e and Supplementary Fig. 4). Live imaging revealed that multicilia in Wdr47−/− mEPCs expressing Centrin1-GFP were still rotatory, whereas those in Wdr47−/− mEPCs expressing GFP-Wdr47 displayed planar beat (Fig. 2f and Supplementary Movie 2). These results further attribute the lack of CP formation in Wdr47−/− multiciliated cells (Fig. 1i and Supplementary Fig. 2) to the loss of Wdr47.
Next we investigated whether Wdr47 was also required for the stability of pre-existing CP. To do this, we tried to deplete Wdr47 after the CP formation by expressing Cre recombinase in cultured Wdr47flox/flox mEPCs from day −4 or −1 and examined multicilia at day 5 or day 15 (Fig. 2g). The Cre expression at day −4 resulted in rotatory beat pattern and loss of ciliary Hydin even at day 5 (Fig. 2h and Supplementary Fig. 5), suggesting that under the condition Wdr47 was depleted prior to the CP formation in the cells. By contrast, in mEPCs expressing Cre from day −1, Wdr47 was depleted after the CP formation because the incidence of rotatory beat increased dramatically from day 5 to day 15, accompanied with a similar extent of reduction in Hydin-positive multicilia (Fig. 2h and Supplementary Fig. 5). Transmission EM confirmed a 3.5-fold increase of CP-less cilia from day 5 to day 15 (Fig. 2i). Therefore, the maintenance of CP also requires Wdr47.
Wdr47-deficient mice display PCD-like phenotypes hydrocephalus and sinusitis
Next, we investigated whether Wdr47 deficiency induced multicilia-related pathological disorders in mice. Wdr47-deficient mice die immediately after birth due to central nervous system defects15 and were not suitable for the investigation. The Wdr47Kof/Kof mice, however, are quite heterogeneous in viability: the majority of them die before P55 but the remaining mice live longer than P15354, probably due to variations in Wdr47 expression levels15. To maintain minimal levels of Wdr47 for mouse survival, we created Wdr47Kof/− mice and found that they were viable after birth. Wdr47Kof/− mice were considerably smaller in size than their wild-type littermates (Fig. 3a) and could only survive for <4 weeks. While Wdr47-deficient neonatal mice15 and Wdr47Kof/Kof adult mice54 only display slightly enlarged brain ventricles, the ventricles of Wdr47Kof/− mice expanded markedly when examined at P14 (Fig. 3b), indicating hydrocephalus21,28,55. Moreover, massive amounts of mucus were observed bilaterally in the paranasal cavity of P14 Wdr47Kof/− mice (Fig. 3b), indicating chronic sinusitis55. These phenotypes are hallmarks of primary ciliary dyskinesia (PCD)21,26,56.
To further clarify that the enlarged ventricles were not due to Wdr47 deficiency-induced neuronal death54, we removed the Kof cassette15 and generated Wdr47flox/flox;GFAP-Cre conditional knockout (cKO) mice to specifically knockout Wdr47 in GFAP-positive glial cells (Fig. 3c)57, including EPC progenitors58,59. The cKO mice were born normally but developed dome-shaped heads within 3 weeks (Fig. 3d) and died at ~4 weeks old. Coronal brain sections revealed dilated ventricles and magnetic resonance imaging further confirmed severe hydrocephalus of the mice (Fig. 3e). Scanning EM revealed that multicilia in individual ependymal cells tended to cluster together in Wdr47flox/flox mice but became scattered in the cKO mice (Fig. 3f). Live imaging of brain slices revealed planar beat of the Wdr47flox/flox ependymal cilia but rotatory beat of the cKO cilia (Fig. 3g). Wdr47 deficiency or insufficiency thus causes PCD.
Camsaps are CP-associated proteins colocalizing with Wdr47
How does Wdr47 impact the CP formation? As Wdr47 can be recruited to MTs by MT-binding proteins such as Map8 and Camsap315,37, we speculated that it might function with certain MT-binding proteins for the nucleation or stabilization of central MT seeds. Interestingly, we noticed that all three mouse paralogues of Camsaps, Camsap1, Camsap2, and Camsap3, were readily identified from our purified wild-type multicilia samples by mass spectrometry (Fig. 4a). Camsap3 appeared to be the most abundant among the three Camsaps according to both their LFQ intensities and unique peptide counts (Fig. 4a). We have previously shown that all three Camsaps can associate with Wdr47. Moreover, Camsap1 and Camsap3 function as downstream effectors of Wdr47 in neuronal polarization15. Therefore, Camsaps might also function in multicilia with Wdr47.
Super-resolution imaging revealed that Camsaps were indeed CP-associated proteins with distribution patterns resembling those of Wdr47. In short cilia negative for Hydin, Camsaps were highly concentrated at the ciliary tip and also distributed in the axonemal central lumen (Fig. 4b). In long cilia they tended to concentrate in the bottom region of the central lumen complementary to Hydin (Fig. 4b). In addition, Camsap1 tended to display punctate distributions along the CP (Fig. 4b). Both endogenous and GFP-tagged Camsaps were distributed above TZ in ependymal cilia when Cep162 and Cep290 were used as TZ markers (Fig. 4c)44,60. When mEPCs were pre-extracted with Triton X-100 to remove soluble proteins prior to fixation, the enrichment of Camsaps at the base of the central lumen became more obvious (Fig. 4c). Such a distribution pattern of Camsaps (Fig. 4b, c) resembles proteins localized at the CP minus end region, or the CP-foot45. Therefore, similar to Wdr47, Camsaps are preferentially enriched at the tip of nascent short cilia and the minus end region of central MTs in long cilia.
As our antibodies did not allow co-immunostaining with Wdr47, we examined GFP-Camsaps. In mEPCs expressing Centrin1-GFP, immunofluorescent signals of Wdr47 were independent of those of Centrin1-GFP (Fig. 4d), indicating no fluorescent bleed between the two channels. In contrast, GFP-Camsaps co-localized nicely with endogenous Wdr47 in multicilia (Fig. 4d), confirming their interplays with Wdr47 in ependymal cilia.
Although the levels of Camsaps in mEPCs were not affected by the Wdr47 deficiency (Fig. 4e), immunostaining confirmed that the ciliary localization of Camsaps was largely dependent on Wdr47 (Fig. 4f, g). Therefore, Camsaps could be downstream effectors of Wdr47 in the CP formation.
Overexpression of Camsaps induces central MT formation in Wdr47 −/− multicilia
We have recently reported that overexpression of Camsap1 or −3 rescues the polarization defects of Wdr47-deficient neurons15. To understand whether excessive Camsaps could also functionally compensate for the Wdr47 deficiency in mEPCs, we overexpressed GFP-tagged Camsaps or Centrin1 (negative control) in Wdr47−/− mEPCs through lentiviral infection (Fig. 5a). Wdr47−/− mEPCs expressing Centrin1-GFP still displayed rotatory multicilia, whereas the majority of the GFP-Camsap1-expressing cells displayed planar ciliary beat (Fig. 5b, c and Supplementary Movie 3). Different cilia, however, tended to beat towards different directions (Fig. 5b and Supplementary Movie 3). The GFP-Camsap1 overexpression also increased the percentage of cells with mixed ciliary beat patterns by 3.1-fold (Fig. 5b, c). Although GFP-Camsap2 and GFP-Camsap3 were expressed in low levels (Fig. 5a), percentages of mEPCs with planar and mixed beat patterns still increased by 6.5-fold and 10.9-fold, respectively, as compared to the Centrin1-GFP-positive cells (Fig. 5b, c). When fixed cells were examined, GFP-Camsaps markedly rescued the ciliary Hydin localization as compared to Centrin1-GFP (Fig. 5d, e). These results suggest a partial rescue of CP by Camsaps overexpression.
Next, we examined the ciliary ultrastructure. As we were unable to recognize GFP-positive cells in EM, we extensively examined the GFP-Camsap1 samples due to their high viral infection efficiency (>80%), exogenous expression levels (Fig. 5a), and rescue effects on the planar beat pattern and ciliary Hydin localization (Fig. 5b–e). 48.9% of their axonemal cross-sections displayed two central MTs; 3.5% displayed abnormal central MT numbers (1 or 3-to-6) (Fig. 5f, g). Occasionally we observed one dislocated central MT outside the central lumen (n = 2), (Fig. 5f) or extra doublet-like MTs (n = 3) (Supplementary Fig. 6a). Central MTs were observed to extend from the ciliary base to the tip in longitudinal sections (Fig. 5f). We also observed multiple short MTs at the tip (Fig. 5f), suggesting that the incidence of axonemes with extra central MTs (2.6%; Fig. 5g) is probably underestimated due to quantifications on cross-sections. By contrast, none of the axonemal cross-sections (total n = 307) from the Centrin1-GFP samples displayed visible central MT(s). We also examined a set of samples for GFP-Camsap2 and GFP-Camsap3. In all, 27% of axonemal cross-sections from the Camsap3 sample contained either one (1/173) or two (46/173) central MTs (Fig. 5g). All cross-sections from the Camsap2 sample (n = 239), however, were CP-less, possibly due to its low expression level and efficacy because EM does not allow choosing cells expressing relative high levels of GFP-Camsap2.
Taken together, we conclude that increasing the total levels of Camsaps partially compensate for Wdr47 deficiency in the central MT formation.
Wdr47 recruits Camsaps to the central lumen for proper CP formation
As the partial rescue effects of overexpressed Camsaps (Fig. 5a–g) suggested a role of Wdr47 for efficient production and proper positioning of central MTs, we speculated that Wdr47 might function by increasing the regional ciliary concentration of Camsaps. We have previously shown that Wdr47 interacts with Camsaps through its N-terminal region (WdrN) but not the C-terminal WD40 repeats (WdrC) (Fig. 5h)15. When expressed in Wdr47−/− mEPCs, GFP-Wdr47 entered multicilia and rescued the ciliary localizations of endogenous Camsap1 and Hydin, the CP marker (Fig. 5i; also see Fig. 2e). GFP-WdrC, but not GFP-WdrN, strongly localized into multicilia (Fig. 5i). Neither construct, however, was able to function as the full-length to restore ciliary Camsap1 and Hydin (Fig. 5i) or the planar ciliary beat (Fig. 5j vs. Fig. 2f). Wdr47 thus requires both its Camsap-interacting and cilia-localization regions for the ciliary enrichment of endogenous Camsaps and, consequently, proper CP formation.
We further examined the detailed localization of GFP-WdrC through super-resolution microscopy and found that GFP-WdrC was distributed in the ciliary central lumen (Fig. 5k). As Wdr47−/− multicilia are CP-less (Fig. 1i), such a result suggests that this C-terminal region can target Wdr47 to the central lumen independently of central MTs. Taken together, we conclude that Wdr47 binds to Camsaps through its N-terminal region and targets them to the ciliary central lumen through its C-terminal region for efficient and proper CP formation.
Camsaps promote the central MT formation by stabilizing the MT minus end
We have previously shown that Camsap3 can recruit Wdr47 to MT minus ends15, implying that Wdr47 might target Camsaps by binding to regions outside their MT-binding domains. To clarify this, we mapped the Wdr47-interacting region of Camsap1 by co-immunoprecipitation. Indeed, the linker region between the CH and the first coiled coil (CC) domains of Camsap1 (312-858 aa) strongly interacted with Wdr47, whereas the CC-containing region and the CKK domain involved in the MT association10,11,12,13 were dispensable (Fig. 6a, b).
Camsaps function in MT dynamics by stabilizing the minus end of pre-existing MTs10,12,13. It is known that, although the CKK domain alone is sufficient for binding to the MT minus end, a longer fragment containing the CC region displays markedly increased lattice-binding and minus end-stabilization ability10,11,12,13. To understand whether Camsaps used the similar mechanism to induce central MT formation, we overexpressed constructs containing the CKK domain and a longer CC-containing fragment (LC) as GFP fusion proteins in Wdr47−/− mEPCs (Fig. 6c, d). Both types of constructs displayed significant rescue effects on ciliary beat patterns as compared to Centrin1-GFP (Fig. 6e and Supplementary Movie 4), suggesting that the CKK domain alone is already functional. Consistently, all the constructs displayed ciliary localizations as well as an ability to rescue the ciliary localization of Hydin in the Wdr47−/− mEPCs (Fig. 6f and Supplementary Fig. 7). The LC constructs generally yielded higher percentages of ciliary Hydin-positive mEPCs than the CKK constructs (Fig. 6f and Supplementary Fig. 7).
EM further confirmed that all the constructs of Camsaps induced central MT formation in the Wdr47−/− multicilia (Fig. 6g, h). Notably, 70% of the axonemal cross-sections from the GFP-Ca1LC samples contained one or more central MTs and 21% contained >2 (up to 13) central MTs (Fig. 6g, h). Furthermore, 28 sections (8%) contained dislocated central MTs outside the central lumen (Fig. 6h). By contrast, 25% of the cross-sections from the GFP-Ca1CKK samples contained central MTs (Fig. 6g). Among them, three sections (2%) contained dislocated central MT(s). In addition, axonemes with an extra MT doublet were also observed for both constructs (Supplementary Fig. 6b, c). We observed both long and short central MTs in longitudinal axonemal sections (Supplementary Fig. 6d). In comparison, 38% and 44% of the cross-sections respectively from the GFP-Ca2LC and GFP-Ca3LC samples contained one or more central MTs, with 3% and 18% of the total cross-sections containing >2 (up to 10) central MTs (Fig. 6g, h). The incidences of central MT-containing cross-sections from the GFP-Ca2CKK and GFP-Ca3CKK samples were 15% and 38%, respectively (Fig. 6g).
These results further strongly support a direct role of Camsaps in the CP formation by binding and stabilizing the minus ends of central MTs. The prominent rescue effects of GFP-Ca2LC and GFP-Ca2CKK (Fig. 6e–g), despite their low expression levels relative to the corresponding constructs of Camsap1 and Camsap3 (Fig. 6d), also confirm that Camsap2 is involved in the CP formation. Furthermore, as Camsaps are unable to nucleate MTs10,11,12,13, the formation of extra and even 13 central MTs indicates that the available central MT seeds in an axoneme can largely exceed two.
Central MT formation requires the MT-severing activity of Katanin
The seeds for non-centrosomal MTs usually come from severed MTs or MTs released from the γ-tubulin ring complex5,6,12,13. As the MT-severing enzyme Katanin directly binds to Camsap2 and −312,40 and protozoan Katanin is essential for the CP formation and has been shown to bind to and severing axonemal MT doublets61,62,63, we speculated that Katanin might function to generate the central MT seeds for mammalian multicilia. Immunostaining revealed that Katanin p60 displayed multiciliary localizations in mEPCs, abundant at the tip of short cilia (Fig. 7a). GFP-p60 also displayed similar ciliary localizations and co-localized with Camsaps at the ciliary tip, when Camsap1 was used as marker (Fig. 7b).
To investigate whether the MT severing activity of Katanin is required for the central MT formation, we overexpressed GFP-p60 or GFP-p60K257A, a point mutant acting as a dominant inhibitor64, in wild-type mEPCs (Fig. 7c). Like p60, the dominant mutant p60K257A also entered multicilia (Fig. 7d). Wild-type mEPCs overexpressing Centrin1-GFP rarely had Hydin-negative cilia (0.9%; n = 117) (Fig. 7d). The GFP-p60 overexpression moderately increased the incidence (8.9%; n = 90). By contrast, multicilia in 46.7% of mEPCs positive for GFP-p60K257A (n = 105) lacked Hydin (Fig. 7d). Consistently, the percentage of mEPCs with rotatory ciliary beat pattern increased moderately (5.3-fold) in the GFP-p60 populations and markedly (40.7-fold) in the GFP-p60K257A populations as compared to the Centrin1-GFP populations (Fig. 7e and Supplementary Movie 5). EM analyses revealed increased incidences of CP-less cross-sections (2.3-fold in the GFP-p60 samples and 9.3-fold in the GFP-p60K257A samples) as well (Fig. 7f). Notably, cross-sections containing 1 (3%) and >2 (4%) central MTs emerged in the GFP-p60 samples, which were not observed in either the Centrin1-GFP or the GFP-p60K257A samples (Fig. 7f). The MT-severing activity of Katanin is thus critical for proper mammalian CP formation.
Next we explored whether the rescue effect of Camsaps in Wdr47−/− mEPCs required Katanin activity by co-expressing RFP-p60K257A or RFP-p60. We initially performed the experiments with GFP-Camsap1 because it displayed the strongest rescue effect (Fig. 5a–g). Moreover, as Camsap1 does not interact with Katanin1, its overexpression would not influence the effects of RPF-p60 and RFP-p60K257A. Compared to Centrin1-RFP, co-expression of RFP-p60K257A with GFP-Camsap1 induced a 3.3-fold decrease in percentage of cells with planar ciliary beat and a 2.8-fold increase in that with rotatory ciliary beat (Fig. 7g and Supplementary Movie 6). In comparison, co-expression of RFP-p60 did not significantly alter the rescue effects of GFP-Camsap1 in Wdr47-deficient mEPCs (Fig. 7g and Supplementary Movie 6). We then examined GFP-Ca3LC, the Camsap3 deletion mutant displaying a remarkable rescue effect (Fig. 6d–h) and lacking Katanin-binding region (Fig. 6c)40. Compared to Centrin1-RFP, co-expression of RFP- p60K257A also similarly compromised the rescue efficiency of GFP-Ca3LC (Fig. 7g). Therefore, Katanin activity is important for the Camsap overexpression-induced central MT formation.
Therefore, like protozoan Katanin61,62,63, mammalian Katanin also functions in the CP formation. As tubulin dimers can be transported into cilia through intraflagellar transport35, we modified the model by Sharma and colleagues63 and propose that Katanin provides central MT seeds by severing the tip region of axonemal MT doublets (Fig. 7h).
Our results indicate that Wdr47 ensures the efficient formation and accurate positioning of central MTs by concentrating Camsaps into cilia. Wdr47 is a prerequisite because CP completely failed to form upon Wdr47 deficiency (Figs. 1 and 2, and Supplementary Figs. 2 and 3). Ciliary Camsaps co-localized with Wdr47 mainly at the tip of nascent short cilia and the base of central lumen in long cilia and became markedly reduced in Wdr47-deficient mEPCs (Figs. 1d, e and 4b–g). Although central MTs can form in Wdr47−/− mEPC when the total levels of Camsaps were increased through overexpression (Figs. 5a–g and 6, and Supplementary Fig. 7), they emerged with low efficiency and abnormal numbers, and sometimes at a wrong location: comparing to a near 100% efficiency of the CP formation in wild-type ependymal and airway multiciliated cells (Fig. 1i and Supplementary Fig. 2)28,30,65, only <50% of ependymal ciliary cross-sections were rescued to two central MTs and at least 30% were still CP-less (Figs. 5f, g and 6g, h). Furthermore, up to 21% contained more than two central MTs, and dislocated singlet MT(s) outside the central lumen were also observed (Figs. 5f, g and 6g, h, and Supplementary Fig. 6d). As Camsaps do not induce MT nucleation10,11,12,13, the emergence of excessive numbers (up to 13 in our EM results) of central MTs (Figs. 5f, g and 6g, h) indicate that Camsaps function by stabilizing the minus ends of pre-existing MT seeds whose number can largely exceed two in a cilium. Our interaction and localization analyses (Figs. 5i, k and 6a, b) further suggest that Wdr47 binds to the N2 region of Camsaps through its N-terminal region and recruits them to the ciliary central lumen through its C-terminal region. Therefore, the Wdr47-Camsap interaction allows Camsaps to function at low physiological concentrations to avoid production of extra central MTs. How a cilium manages to produce precisely two central MTs, however, still requires future quantitative studies.
Camsap1-3 appear to function redundantly and contribute collectively to the central MT formation. Different Camsaps share common and also display individual properties10,11,12,13,14. As mEPCs express all three proteins concomitantly (Fig. 4), the contribution of each Camsap may be affected by both expression level and efficacy relative to the others (Figs. 5 and 6). Although multicilia-related defects have not been documented for Camsap1- or Camsap2-deficient mice14,18, during the revision process we noticed that a recent publication reports that Camsap3 localizes to the base of axonemes in murine nasal multiciliated cells and Camsap3 deficiency results in the CP loss in 77.4% axonemal cross-sections of the cells66. Consistently, Camsap3-deficient mice display severe nasal airway blockage66, similar to our Wdr47Kof/- mice (Fig. 3b). In sharp contrast to the severe hydrocephalus of our Wdr47flox/flox;GFAP-Cre cKO mice (Fig. 3c–e), Camsap3-deficient mice display only mild or no hydrocephalus phenotypes66. Two subsequent publications report that Camsap3-deficient mice have normal beating cilia in ependymal cells67 and normal CP formation in oviduct multicilia68. These results also echo our proposed redundant and collective effects of Camsaps. Future systematic analyses using single, double, and triple gene knockout mice of Camsaps will be still required to determine detailed contributions of individual Camsaps and their collective effects on ciliary CP formation of different tissue cells.
Our results suggest that Katanin is involved in the production of central MT seeds. p60 and p80 subunits of Katanin are in fact the only two proteins known to be essential to the CP formation in protozoa48,61,62,63. Chlamydomonas p80 specifically distributes in ciliary outer doublet compartment61, whereas overexpressed GFP-p60 has been shown to specifically bind to and sever outer doublets in Tetrahymena63. Protozoan Katanin has also been proposed to provide central MT seeds by severing MTs nucleated from intraflagellar γ-tubulin62 or free tubulin dimers for CP assembly by severing outer doublets63. We found that both endogenous p60 and GFP-p60 display ciliary localization and also enrich at the tip of short cilia (Fig. 7a, b). Katanin activity is also important for Camsaps-mediated CP formation (Fig. 7e–g). As overexpression of GFP-p60 induced CP loss in a portion of ependymal axonemes (Fig. 7e, f), mammalian Katanin unlikely functions by providing tubulin dimers for the CP formation. On the other hand, no evidence to date suggests a localization of γ-tubulin in mammalian multicilia69,70,71. As the observations of up to 13 central MTs in our rescue experiments (Figs. 5f, g and 6g, h) provide solid evidence for the presence of excessive central MT seeds and nascent central MTs have been shown to emerge initially from the top region of Chlamydomonas flagella46, we modified the previous models and propose that mammalian Katanin severs the tip of axonemal outer MTs to generate central MT seeds for Camsaps to bind and stabilize at early stages of ciliogenesis (Fig. 7h). Consistently, we observed doublet-like MTs additional to the nine outer doublets upon the overexpression of Camsap1 or its deletion constructs (Supplementary Fig. 6a–c). Future studies will be required to verify whether Katanin p60/p80 enters multicilia by binding to Camsap2 and Camsap312,40. In addition, two paralogues of Katanin p60, Katnal1 and Katnal2, also affect the growth and motility of multicilia38,72,73. Katnal1 has also been shown to sever MTs to build the dense MT arrays in Drosophila mechanosensory cilia38,72,73,74. As the overexpress of p60K257A did not completely abolish the CP formation in mEPCs (Fig. 7e, f), whether Katnal1 and Katnal2 have a role in metazoan central MT seeds production also needs to be clarified in the future.
Taken together, we propose a model that Wdr47, Camsaps, and Katanin function together to produce the CP of mammalian multicilia: Katanin severs the tip of outer MTs to generate central MT seeds in nascent short cilia, Camsaps stabilize the seeds by binding to their minus ends, and Wdr47 concentrates Camsaps and facilitates their targeting into ciliary central lumen so that the Camsaps-bound MT seeds eventually develop into CP following the elongation of cilia (Fig. 7h). In addition to the CP formation, emerging clues of their corporative actions are reported in neurons15,16,18,41,42,75 and epithelial cells17,19,76. Other non-centrosomal MT arrays requiring Camsaps5,6,7 could involve Katanin and Wdr47 as well. Both Katanin and Wdr47 are expected to bind between the CH domain and the first CC region of Camsap2 and -3 (Fig. 6a, b)40. Therefore, these three groups of proteins might similarly constitute a team for the formation of non-centrosomal MT arrays in polarized subcellular compartments. It will thus be interesting to clarify their detailed interplays and consequences of the interactions as well in other types of cells.
The full-length or partial cDNAs for mouse Wdr47 (NM_181400), mouse Camsap1 (XM_006497897), mouse Camsap2 (NM_001347109), and mouse Katanin p60 (NM_011835) were amplified by PCR from total cDNAs from mouse testis, brain or mTECs. The full-length of mouse Camsap3 (NM_027171) was amplified by PCR from the GFP-Nezha plasmid (kindly provided by Dr. Wenxiang Meng, Institute of Genetics and Developmental Biology, Chinese Academy of Sciences)77. To express GFP- or RFP- fusion proteins, the cDNA fragments were constructed into the lentiviral expression vector, pLV-EGFP-C1 or pLV-RFP-C178, respectively. The cDNAs of WdrN (1-400 aa) and WdrC (401-920 aa) were PCR amplified from the pLV-EGFP-Wdr47 plasmid and constructed into pLV-EGFP-C1. The cDNAs of Camsaps: Ca1N1 (1-311 aa), Ca1N2 (312-858 aa), Ca1CC (859-1442 aa), Ca1CKK (1443-1583 aa), Ca1LC (859-1583 aa), Ca2CKK (1333-1472 aa), Ca2LC (739-1472 aa), Ca3CKK (1113-1252 aa), and Ca3LC (587-1252 aa) were PCR amplified from the pLV-EGFP-Camsaps plasmids and constructed into pLV-EGFP-C1. The K257A mutant of Katanin p60 (900 AAG→GCG) were generated by PCR64. For expression of FLAG-fusion proteins, the cDNA fragments were subcloned into the pcDNA3.1-NFLAG vector. The full-length cDNAs of mouse Wdr47 or mouse Camsap1 (1073-1382 aa) were PCR amplified and constructed into pET28a to express His-tagged antigens for antibody production and into pGEX4T-1 to express GST-fusion proteins for antibody purification. All the primers were list in the Supplementary Table 1. All the constructs were verified by sequencing.
Mice experiments were performed in accordance with the ethical guidelines of Shanghai Institute of Biochemistry and Cell Biology, Chinese Academy of Sciences, and approved by the Institutional Animal Care and Use Committee.
Wdr47Kof/+ mice (Wdr47tm1a(EUCOMM)Wtsi) were purchased from Wellcome Trust Sanger Institute79. Wdr47+/− and Wdr47flox/+ mice were generated by crossing the Wdr47 Kof/+ mice with Ella-Cre or FLP mice (Model Animal Research Center of Nanjing University, China), respectively. To knockout Wdr47 in the GFAP-positive glial cells, Wdr47 flox/flox mice were crossed with GFAP-Cre mice (a gift from Dr. Leping Cheng, Institute of Neuroscience, Chinese Academy of Sciences). Primers used for genotyping are listed in Supplementary Table 1.
Cell culture, transfection, viral infection, and cilia purification
Cells were maintained at 37 °C in an atmosphere containing 5% CO2. Unless otherwise indicated, the culture medium was Dulbecco’s Modified Eagle’s medium (DMEM) supplemented with 10% fetal bovine serum (Ausbian, VS500T), 0.3 mg/ml glutamine (Sigma, G8540), 100 U/ml penicillin (Solarbio P8420), and 100 U/ml streptomycin (Solarbio S8290).
mTECs were isolated and cultured as described previously78,80. mTECs were isolated from 4-week C57BL/6J mice. After dissecting the adhered muscle tissue, tracheas were sliced lengthwise and digested in Ham’s F-12K medium with 0.15% Pronase E (Sigma, P6911) and 0.1 mg/ml DNase I (Sigma, D5025) overnight at 4 °C. Cells were collected by centrifugation for 5 min at 400 × g at room temperature (r.t.) and resuspended with mTEC basic medium [DMEM-Ham’s F-12 medium (Thermo Fisher, 11330-032) supplemented with 3.6 mM sodium bicarbonate, 4 mM l-glutamine, 1% penicillin/streptomycin, 0.25 μg/ml fungizone] with 10% FBS. Cells were plated and incubated at 37 °C for 4 h to allow fibroblasts to attach. mTECs were collected by centrifugation at 400 × g for 5 min, resuspended in mTEC plus medium [mTEC basic medium supplemented with 10 μg/ml insulin (Sigma, I6634), 5 μg/ml transferrin (Sigma, T8158), 0.1 μg/ml Cholera toxin (Sigma, C8052), 25 ng/ml epidermal growth factor (Sigma, E4127), 30 μg/ml bovine pituitary extract (Sigma, P1167), 5% FBS, and 0.05 μM retinoic acid (freshly added; Sigma, R2625)], and seeded into collagen (Sigma, C8897)-coated 6.5-mm Transwells with 0.4-μm-pore polyester membrane insert (Corning, 3470). When cells reached full confluency, air-liquid interface (ALI) was created by removing medium in the upper compartment and replacing medium in the bottom compartment with the mTEC differentiation medium [mTEC basic medium supplemented with 2% Nu Serum (BD, 355100) and 0.05 μM retinoic acid (freshly added)] to induce differentiation. DAPT (Sigma, D5942) was added to 10 μM at day 1 post ALI to increase multiciliated cell differentiation efficiency.
Multiciliated mEPCs were obtained and cultured as described36,53,81. P0 C57BL/6J mice telencephala were dissected after removing the cerebellum, olfactory bulbs, and hippocampus with sharp tweezers (Dumont, 1214Y84) in cold dissection solution (161 mM NaCl, 5 mM KCl, 1 mM MgSO4, 3.7 mM CaCl2, 5 mM Hepes, and 5.5 mM Glucose, pH 7.4) under a stereo microscope. The telencephala were digested with 1 ml of the dissection solution containing 10 U/ml papain (Worthington, LS003126), 0.2 mg/ml L-Cysteine, 0.5 mM EDTA, 1 mM CaCl2, 1.5 mM NaOH, and 0.15% DNase I (Sigma, D5025) for 30 min at 37 °C. Cells were dissociated mechanically by pipetting up and down 10 times with a 5-ml pipette and collected by centrifugation at 400 × g for 5 min at r.t. Cells were resuspended with DMEM medium supplemented with 10% fetal bovine serum (FBS) and 1% penicillin/streptomycin, and inoculated into the laminin-coated flask (Sigma, L2020). Neurons were shaken off and removed after culturing for 2 days after inoculation. The remaining cells were further cultured to ~80% confluency (usually 3–4 days) and then transferred into the wells of laminin-coated 29-mm glass-bottom dishes (Cellvis, D29-14-1.5-N) for motility assay or immunofluorescence staining or 75-cm2 laminin-coated flasks for cilia purification. After cells were confluent, FBS was removed from the medium to initiate differentiation.
To express exogenous proteins, HEK 293T were transfected with polyethlenimine (PEI, Polysciences, 23966-2), respectively, for 48 h. Lentiviral production and infection were performed as described previously78. Cultured mEPCs were infected at day one before serum starvation (day −1) unless otherwise stated. For rescue experiments and expressing GFP-tagged Camsaps, and their deletion constructs in Wdr47−/− ependymal cells, mEPCs derived from Wdr47−/− mice were infected with lentivirus at day −1, day 2, and day 5 and assayed at day 10.
Purification of ependymal cilia and LFQ mass spectrometric analyses were carried out as described53. To purify ependymal cilia, two 75-cm2 flasks of ependymal cells derived from 10 E18.5 Wdr47+/+ or Wdr47−/− embryos at the day 10 post serum starvation were harvested by centrifugation at 2000 rpm for 5 min at 4 °C. The cells were resuspended in 2.4 ml of deciliation buffer (20 mM PIPES, 250 mM sucrose, 20 mM CaCl2, 0.05% Triton X-100, pH 5.5) and agitated vigorously for 10 min on a vortex mixer (G560OE, Scientific Industries). After centrifugation at 600 × g for 5 min at 4 °C, the cilia-containing supernatant was collected by centrifugation at 20,000 × g for 30 min. The pelleted cilia were washed twice with 1 ml of PBS, followed by centrifugation at 20,000 × g for 15 min. The isolated cilia were lysed in 100 μl of lysis buffer [20 mM Tris-HCl (pH 7.5), 100 mM KCl, 0.1% NP-40, 1 mM EDTA, 10 mM Na4O7P2, and protease inhibitors] and boiled at 100 °C for 10 min. 50 μl of the samples was used for Mass spectrometry analysis and another 50 μl was used for immunoblotting (Fig. 2d). The full scan blots are provided in the Source Data file.
Label-free quantitative mass spectrometry
In all, 50 μL of lysed wild type and Wdr47−/− cilia samples were precipitated with acetone. The protein pellet was dried by using a Speedvac for 1−2 min. The pellet was subsequently dissolved in 8 M urea, 100 mM Tris-HCl, pH 8.5. TCEP (final concentration is 5 mM) (Thermo Scientific) and iodoacetamide (final concentration is 10 mM) (Sigma) for reduction and alkylation were added to the solution and incubated at room temperature for 30 min, respectively. The protein mixture was diluted four times and digested overnight with Trypsin at 1:50 (w/w) (Promega). The tryptic-digested peptide solution was desalted using a MonoSpinTM C18 column (GL Science, Tokyo, Japan) and dried with a SpeedVac.
The peptide mixture was analyzed by a home-made 30-cm-long pulled-tip analytical column (75 μm ID packed with ReproSil-Pur C18-AQ 1.9 μm resin, Dr. Maisch GmbH), the column was then placed in-line with an Easy-nLC 1200 nano HPLC (Thermo Scientific, San Jose, CA) for mass spectrometry analysis. The analytical column temperature was set at 55 °C during the experiments. The mobile phase and elution gradient used for peptide separation were as follows: 0.1% formic acid in water as buffer A and 0.1% formic acid in 80% acetonitrile as buffer B, 0–1 min, 3–8% buffer B; 1–301 min, 8–25% buffer B; 301–339 min, 25–50% buffer B, 339–340 min, 50–100% buffer B, 340–360 min, 100% buffer B. The flow rate was set as 300 nl/min.
Data-dependent tandem mass spectrometry (MS/MS) analysis was performed with a Q Exactive Orbitrap mass spectrometer (Thermo Scientific, San Jose, CA). A cycle of one full-scan MS spectrum (m/z 300–1800) was acquired followed by top 20 MS/MS events, sequentially generated on the first to the twentieth most intense ions selected from the full MS spectrum at a 28% normalized collision energy. Full scan resolution was set to 70,000 with automated gain control (AGC) target of 3e6. MS/MS scan resolution was set to 17,500 with isolation window of 1.8 m/z and AGC target of 1e5. The number of microscans was one for both MS and MS/MS scans and the maximum ion injection time was 50 and 100 ms, respectively. The dynamic exclusion settings used were as follows: charge exclusion, 1 and >8; exclude isotopes, on; and exclusion duration, 15 s. MS scan functions and LC solvent gradients were controlled by the Xcalibur data system (Thermo Scientific).
MS/MS data were processed using Maxquant software version V188.8.131.52. MS/MS spectra were searched by the Andromeda search engine against the SwissProt Mouse database at a false discovery cutoff ≤1%. Data were searched at 20 ppm mass tolerances for precursor ions for mass calibration and six amino acids were required as the minimum peptide. LFQ intensity was used as relative quantification of protein.
mEPCs grown on fibronectin-coated 29-mm glass-bottom dishes (Cellvis, D29-14-1.5-N) were fixed with 4% paraformaldehyde in PBS for 10 min at room temperature and permeabilization with 0.5% Triton X-100 for 15 min. In Figs. 1e and 4c, mEPCs were pre-extracted with 0.5% Triton X-100 for 30 s before fixation. GFP signals in mEPCs were visualized by immunostaining using anti-GFP antibody. All the antibodies used are listed in Supplementary Table 2.
Confocal images were captured by using Leica TCS SP8 system with a ×63/1.40 oil immersion objective and Z-stack images were obtained with maximum intensity projections. 3D-SIM images were captured with Delta Vision OMX SR imaging system (GE Healthcare) equipped with a Plan Apo ×60/1.42 NA oil-immersion objective lens (Olympus). Serial Z-stack sectioning was performed at 125-nm intervals. Images were processed with SoftWoRx software.
Ciliary motilities were recorded at 140 fps (frames per second) by using an Andor Neo sCMOS camera on Olympus IX71 microscope with a ×63/1.40 oil immersion objective43. To track fluid flows driven by ciliary beat82, fluorescent beads (Fluoresbrite PolyFluor 570 microspheres, Polysciences, 24061-10) were added at 1:200 dilution to the culture medium and imaged at 20 fps for 30 s with a ×63/1.40 oil immersion objective on an Olympus IX81 equipped with Hamamatsu EMCCD camera. Images were processed with ImageJ and Adobe Photoshop CS6.
For transmission EM, mouse trachea or cultured mEPCs were fixed in 2.5% glutaraldehyde overnight at 4 °C, washed with PBS, and treated with 1% OsO4 for 30 min at room temperature. The samples were dehydrated with graded ethanol series and embedded in Epon 812 resin. In total, 70-nm ultrathin sections were stained with 1% lead citrate and 2% uranyl acetate. Images were captured at 80 KV using a Tecnai G2 Spirit transmission electron microscope (FEI, Hillsboro, OR).
For scanning EM, the cortex of P10 mouse brains was fixed in 2.5% glutaraldehyde and 2% paraformaldehyde overnight at 4 °C and dehydrated with a graded ethanol series. Critical point drying was carried out before metal shadowing. The images were taken with a FEI Quanta 250 scanning electron microscope.
Magnetic resonance imaging, tissue section and H&E staining
Mice were anesthetized with isoflurane. T2 weighted spin echo images of the head were acquired by using BioSpec 70/30 USR (Bruker). The imaging parameters were: slice thickness 0.5 mm; time of repetition (TR) 2777.2 ms; and time of echo (TE) 34 ms.
P10 mouse brains were dissected and sectioned into 250-μm-thick sagittal slices using a Leica VT 1000S vibratome. Images were captured with an Olympus SZX16 Stereo Microscope.
For H&E staining, P14 mouse brains and noses were paraffin-embedded and sectioned into 5-μm thick slices with an RM 2235 microtome (Leica). The sections were deparaffinized with xylene, rehydrated, and stained with hematoxylin for 5 min and eosin for 1 min. The tissue images were captured with an Olympus BX51 microscope.
Immunoprecipitation experiments were performed as described78. Cells were lysed with lysis buffer [20 mM Tris-HCl, pH 7.5, 100 mM KCl, 0.1% NP-40, 1 mM EDTA, 10 mM Na4O7P2, 10% Glycerol, and protease inhibitors (Sigma, 539134)] and was cleared by centrifugation at 14,000 × g for 10 min at 4 °C. The precleared cell lysates were incubated with 20 μl of anti-FLAG beads (Sigma, A2220) for 2 h. The beads were washed three times with lysis buffer and three times with wash buffer (20 mM Tris-HCl, pH 7.5, 150 mM KCl, 0.5% NP-40, 1 mM EDTA, 10 mM Na4P2O7,10% Glycerol). The proteins on the FLAG beads were eluted with 30 μl of 1 mg/ml FLAG peptide.
Quantification and statistics
Microscopic and biochemical results were repeated at least twice. Quantification results are presented as mean ± s.d. unless otherwise stated. Two-sided Student’s t test (GraphPad Prism software) was used to calculate P-values between unpaired samples. Differences were considered significant when P < 0.05. Only results from three or more independent experiments were applied to the t-tests.
Further information on research design is available in the Nature Research Reporting Summary linked to this article.
Raw data of label-free quantitative (LFQ) proteomic analysis results (Fig. 2c) have been deposited to the ProteomeXchange Consortium (http://proteomecentral.proteomexchange.org) via the iProX partner repository83 with the accession code (PXD028219). Source data are provided with this paper. Any remaining data that support the results of this study are available from the corresponding author upon reasonable request. Source data are provided with this paper.
Kapitein, L. C. & Hoogenraad, C. C. Building the neuronal microtubule cytoskeleton. Neuron 87, 492–506 (2015).
Oakley, B. R., Paolillo, V. & Zheng, Y. gamma-Tubulin complexes in microtubule nucleation and beyond. Mol. Biol. Cell 26, 2957–2962 (2015).
Stannard, W., Rutman, A., Wallis, C. & O’Callaghan, C. Central microtubular agenesis causing primary ciliary dyskinesia. Am. J. Respir. Crit. Care Med. 169, 634–637 (2004).
Nakayama, K. & Katoh, Y. Ciliary protein trafficking mediated by IFT and BBSome complexes with the aid of kinesin-2 and dynein-2 motors. J. Biochem. 163, 155–164 (2018).
Wu, J. & Akhmanova, A. Microtubule-organizing centers. Annu. Rev. Cell Dev. Biol. 33, 51–75 (2017).
Sanchez, A. D. & Feldman, J. L. Microtubule-organizing centers: from the centrosome to non-centrosomal sites. Curr. Opin. Cell Biol. 44, 93–101 (2017).
Muroyama, A. & Lechler, T. Microtubule organization, dynamics and functions in differentiated cells. Development 144, 3012–3021 (2017).
Kreitzer, G. & Myat, M. M. Microtubule motors in establishment of epithelial cell polarity. Cold Spring Harb. Perspect. Biol. 10, a027896 (2018).
Musch, A. Microtubule organization and function in epithelial cells. Traffic 5, 1–9 (2004).
Atherton, J. et al. A structural model for microtubule minus-end recognition and protection by CAMSAP proteins. Nat. Struct. Mol. Biol. 24, 931–943 (2017).
Hendershott, M. C. & Vale, R. D. Regulation of microtubule minus-end dynamics by CAMSAPs and Patronin. Proc. Natl Acad. Sci. USA 111, 5860–5865 (2014).
Jiang, K. et al. Microtubule minus-end stabilization by polymerization-driven CAMSAP deposition. Dev. Cell 28, 295–309 (2014).
Akhmanova, A. & Hoogenraad, C. C. Microtubule minus-end-targeting proteins. Curr. Biol. 25, R162–R171 (2015).
Zhou, Z. et al. CAMSAP1 breaks the homeostatic microtubule network to instruct neuronal polarity. Proc. Natl Acad. Sci. USA 117, 22193–22203 (2020).
Chen, Y. et al. Wdr47 controls neuronal polarization through the camsap family microtubule minus-end-binding proteins. Cell Rep. 31, 107526 (2020).
Yau, K. W. et al. Microtubule minus-end binding protein CAMSAP2 controls axon specification and dendrite development. Neuron 82, 1058–1073 (2014).
Tanaka, N., Meng, W., Nagae, S. & Takeichi, M. Nezha/CAMSAP3 and CAMSAP2 cooperate in epithelial-specific organization of noncentrosomal microtubules. Proc. Natl Acad. Sci. USA 109, 20029–20034 (2012).
Pongrakhananon, V. et al. CAMSAP3 maintains neuronal polarity through regulation of microtubule stability. Proc. Natl Acad. Sci. USA 115, 9750–9755 (2018).
Toya, M. et al. CAMSAP3 orients the apical-to-basal polarity of microtubule arrays in epithelial cells. Proc. Natl Acad. Sci. USA 113, 332–337 (2016).
Brooks, E. R. & Wallingford, J. B. Multiciliated cells. Curr. Biol. 24, R973–R982 (2014).
Fliegauf, M., Benzing, T. & Omran, H. When cilia go bad: cilia defects and ciliopathies. Nat. Rev. Mol. Cell Biol. 8, 880–893 (2007).
Euteneuer, U. & McIntosh, J. R. Polarity of some motility-related microtubules. Proc. Natl Acad. Sci. USA 78, 372–376 (1981).
Teves, M. E., Nagarkatti-Gude, D. R., Zhang, Z. & Strauss, J. F. 3rd Mammalian axoneme central pair complex proteins: broader roles revealed by gene knockout phenotypes. Cytoskeleton 73, 3–22 (2016).
Carbajal-Gonzalez, B. I. et al. Conserved structural motifs in the central pair complex of eukaryotic flagella. Cytoskeleton 70, 101–120 (2013).
Oda, T., Yanagisawa, H., Yagi, T. & Kikkawa, M. Mechanosignaling between central apparatus and radial spokes controls axonemal dynein activity. J. Cell Biol. 204, 807–819 (2014).
Praveen, K., Davis, E. E. & Katsanis, N. Unique among ciliopathies: primary ciliary dyskinesia, a motile cilia disorder. F1000prime Rep. 7, 36 (2015).
Chilvers, M. A., Rutman, A. & O’Callaghan, C. Ciliary beat pattern is associated with specific ultrastructural defects in primary ciliary dyskinesia. J. Allergy Clin. Immunol. 112, 518–524 (2003).
Lechtreck, K. F., Delmotte, P., Robinson, M. L., Sanderson, M. J. & Witman, G. B. Mutations in Hydin impair ciliary motility in mice. J. Cell Biol. 180, 633–643 (2008).
Lechtreck, K. F. & Witman, G. B. Chlamydomonas reinhardtii hydin is a central pair protein required for flagellar motility. J. Cell Biol. 176, 473–482 (2007).
Zhang, Z. et al. Accelerated mortality from hydrocephalus and pneumonia in mice with a combined deficiency of SPAG6 and SPAG16L reveals a functional interrelationship between the two central apparatus proteins. Cell Motil. Cytoskeleton 64, 360–376 (2007).
Tovey, C. A. & Conduit, P. T. Microtubule nucleation by gamma-tubulin complexes and beyond. Essays Biochem. 62, 765–780 (2018).
Nachury, M. V., Seeley, E. S. & Jin, H. Trafficking to the ciliary membrane: how to get across the periciliary diffusion barrier? Annu. Rev. Cell Dev. Biol. 26, 59–87 (2010).
Garcia-Gonzalo, F. R. & Reiter, J. F. Open sesame: how transition fibers and the transition zone control ciliary composition. Cold Spring Harb. Perspect. Biol. 9, a028134 (2017).
Taschner, M. et al. Intraflagellar transport proteins 172, 80, 57, 54, 38, and 20 form a stable tubulin-binding IFT-B2 complex. EMBO J. 35, 773–790 (2016).
Bhogaraju, S. et al. Molecular basis of tubulin transport within the cilium by IFT74 and IFT81. Science 341, 1009–1012 (2013).
Zheng, J. et al. Microtubule-bundling protein Spef1 enables mammalian ciliary central apparatus formation. J. Mol. Cell Biol. 11, 67–77 (2019).
Wang, W. et al. Nemitin, a novel Map8/Map1s interacting protein with Wd40 repeats. PLoS ONE 7, e33094 (2012).
Ghosh, D. K., Dasgupta, D. & Guha, A. Models, regulations, and functions of microtubule severing by katanin. ISRN Mol. Biol. 2012, 596289 (2012).
Hartman, J. J. & Vale, R. D. Microtubule disassembly by ATP-dependent oligomerization of the AAA enzyme katanin. Science 286, 782–785 (1999).
Jiang, K. et al. Structural basis of formation of the microtubule minus-end-regulating CAMSAP-katanin complex. Structure 26, 375–382 (2018).
Shin, S. C. et al. Structural and molecular basis for katanin-mediated severing of glutamylated microtubules. Cell Rep. 26, 1357–1367 (2019).
Karabay, A., Yu, W., Solowska, J. M., Baird, D. H. & Baas, P. W. Axonal growth is sensitive to the levels of katanin, a protein that severs microtubules. J. Neurosci. 24, 5778–5788 (2004).
Xu, Y. et al. Characterization of tetratricopeptide repeat-containing proteins critical for cilia formation and function. PLoS ONE 10, e0124378 (2015).
Wang, W. J. et al. CEP162 is an axoneme-recognition protein promoting ciliary transition zone assembly at the cilia base. Nat. Cell Biol. 15, 591–601 (2013).
Zhao, H. et al. Fibrogranular materials function as organizers to ensure the fidelity of multiciliary assembly. Nat. Commun. 12, 1273 (2021).
Lechtreck, K. F., Gould, T. J. & Witman, G. B. Flagellar central pair assembly in Chlamydomonas reinhardtii. Cilia 2, 15 (2013).
Adams, G. M., Huang, B., Piperno, G. & Luck, D. J. Central-pair microtubular complex of Chlamydomonas flagella: polypeptide composition as revealed by analysis of mutants. J. Cell Biol. 91, 69–76 (1981).
Witman, G. B., Plummer, J. & Sander, G. Chlamydomonas flagellar mutants lacking radial spokes and central tubules. Structure, composition, and function of specific axonemal components. J. Cell Biol. 76, 729–747 (1978).
Zhu, L., Liu, H., Chen, Y., Yan, X. & Zhu, X. Rsph9 is critical for ciliary radial spoke assembly and central pair microtubule stability. Biol. Cell 111, 29–38 (2019).
Zietkiewicz, E. et al. Mutations in radial spoke head genes and ultrastructural cilia defects in East-European cohort of primary ciliary dyskinesia patients. PLoS ONE 7, e33667 (2012).
Zhao, L., Hou, Y., Picariello, T., Craige, B. & Witman, G. B. Proteome of the central apparatus of a ciliary axoneme. J. Cell Biol. 218, 2051–2070 (2019).
Zhu, X., Liu, Y. & Yang, P. Radial spokes-a snapshot of the motility regulation, assembly, and evolution of cilia and flagella. Cold Spring Harb. Perspect. Biol. 9, a028126 (2017).
Zhang, Y. et al. Vertebrate Dynein-f depends on Wdr78 for axonemal localization and is essential for ciliary beat. J. Mol. Cell Biol. 11, 383–394 (2019).
Kannan, M. et al. WD40-repeat 47, a microtubule-associated protein, is essential for brain development and autophagy. Proc. Natl Acad. Sci. USA 114, E9308–E9317 (2017).
Sironen, A. et al. Loss of SPEF2 function in mice results in spermatogenesis defects and primary ciliary dyskinesia. Biol. Reprod. 85, 690–701 (2011).
Horani, A., Ferkol, T. W., Dutcher, S. K. & Brody, S. L. Genetics and biology of primary ciliary dyskinesia. Paediatr. Respir. Rev. 18, 18–24 (2016).
Bajenaru, M. L. et al. Astrocyte-specific inactivation of the neurofibromatosis 1 gene (NF1) is insufficient for astrocytoma formation. Mol. Cell. Biol. 22, 5100–5113 (2002).
Spassky, N. et al. Adult ependymal cells are postmitotic and are derived from radial glial cells during embryogenesis. J. Neurosci. 25, 10–18 (2005).
Rowitch, D. H. & Kriegstein, A. R. Developmental genetics of vertebrate glial-cell specification. Nature 468, 214–222 (2010).
Yang, T. T. et al. Superresolution pattern recognition reveals the architectural map of the ciliary transition zone. Sci. Rep. 5, 14096 (2015).
Dymek, E. E., Lefebvre, P. A. & Smith, E. F. PF15p is the chlamydomonas homologue of the Katanin p80 subunit and is required for assembly of flagellar central microtubules. Eukaryot. Cell 3, 870–879 (2004).
Dymek, E. E. & Smith, E. F. PF19 encodes the p60 catalytic subunit of katanin and is required for assembly of the flagellar central apparatus in Chlamydomonas. J. Cell Sci. 125, 3357–3366 (2012).
Sharma, N. et al. Katanin regulates dynamics of microtubules and biogenesis of motile cilia. J. Cell Biol. 178, 1065–1079 (2007).
Buster, D., McNally, K. & McNally, F. J. Katanin inhibition prevents the redistribution of gamma-tubulin at mitosis. J. Cell Sci. 115, 1083–1092 (2002).
Teves, M. E. et al. Sperm-associated antigen-17 gene is essential for motile cilia function and neonatal survival. Am. J. Respir. Cell Mol. Biol. 48, 765–772 (2013).
Robinson, A. M. et al. CAMSAP3 facilitates basal body polarity and the formation of the central pair of microtubules in motile cilia. Proc. Natl Acad. Sci. USA 117, 13571–13579 (2020).
Kimura, T., Saito, H., Kawasaki, M. & Takeichi, M. CAMSAP3 is required for mTORC1-dependent ependymal cell growth and lateral ventricle shaping in mouse brains. Development 148, dev195073 (2021).
Usami, F. M. et al. Intercellular and intracellular cilia orientation is coordinated by CELSR1 and CAMSAP3 in oviduct multi-ciliated cells. J. Cell Sci. 134, jcs257006 (2021).
Vladar, E. K. & Stearns, T. Molecular characterization of centriole assembly in ciliated epithelial cells. J. Cell Biol. 178, 31–42 (2007).
Hagiwara, H., Kano, A., Aoki, T., Ohwada, N. & Takata, K. Localization of gamma-tubulin to the basal foot associated with the basal body extending a cilium. Histochem. J. 32, 669–671 (2000).
Clare, D. K. et al. Basal foot MTOC organizes pillar MTs required for coordination of beating cilia. Nat. Commun. 5, 4888 (2014).
Banks, G. et al. A missense mutation in Katnal1 underlies behavioural, neurological and ciliary anomalies. Mol. Psychiatry 23, 713–722 (2018).
Willsey, H. R. et al. Katanin-like protein Katnal2 is required for ciliogenesis and brain development in Xenopus embryos. Dev. Biol. 442, 276–287 (2018).
Sun, L. et al. Katanin p60-like 1 sculpts the cytoskeleton in mechanosensory cilia. J. Cell Biol. 220, e202004184 (2021).
Yu, W. et al. The microtubule-severing proteins spastin and katanin participate differently in the formation of axonal branches. Mol. Biol. Cell 19, 1485–1498 (2008).
Dong, C. et al. CAMSAP3 accumulates in the pericentrosomal area and accompanies microtubule release from the centrosome via katanin. J. Cell Sci. 130, 1709–1715 (2017).
Meng, W., Mushika, Y., Ichii, T. & Takeichi, M. Anchorage of microtubule minus ends to adherens junctions regulates epithelial cell-cell contacts. Cell 135, 948–959 (2008).
Zhao, H. et al. The Cep63 paralogue Deup1 enables massive de novo centriole biogenesis for vertebrate multiciliogenesis. Nat. Cell Biol. 15, 1434–1444 (2013).
Skarnes, W. C. et al. A conditional knockout resource for the genome-wide study of mouse gene function. Nature 474, 337–342 (2011).
You, Y., Richer, E. J., Huang, T. & Brody, S. L. Growth and differentiation of mouse tracheal epithelial cells: selection of a proliferative population. Am. J. Physiol. Lung Cell Mol. Physiol. 283, L1315–L1321 (2002).
Delgehyr, N. et al. Ependymal cell differentiation, from monociliated to multiciliated cells. Methods Cell Biol. 127, 19–35 (2015).
Kunimoto, K. et al. Coordinated ciliary beating requires Odf2-mediated polarization of basal bodies via basal feet. Cell 148, 189–200 (2012).
Ma, J. et al. iProX: an integrated proteome resource. Nucleic Acids Res. 47, D1211–D1217 (2019).
The authors thank institutional core facilities for cell biology and molecular biology for technical supports. We also thank Dr. Kai Jiang (Wuhan University) and Dr. Wenxiang Meng (Institute of Genetics and Developmental Biology, Chinese Academy of Sciences) for plasmids and antibodies. This work was supported by National Key R&D Program of China (2017YFA0503500), National Natural Science Foundation of China (31991192, 31771495, and 31900503), and Chinese Academy of Sciences (XDB19000000).
The authors declare no competing interests.
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Liu, H., Zheng, J., Zhu, L. et al. Wdr47, Camsaps, and Katanin cooperate to generate ciliary central microtubules. Nat Commun 12, 5796 (2021). https://doi.org/10.1038/s41467-021-26058-5