1. Structural Biology and Molecular Biophysics

The inner junction complex of the cilia is an interaction hub that involves tubulin post-translational modifications

  1. Ahmad Abdelzaher Zaki Khalifa
  2. Muneyoshi Ichikawa
  3. Daniel Dai
  4. Shintaroh Kubo
  5. Corbin Steven Black
  6. Katya Peri
  7. Thomas S McAlear
  8. Simon Veyron
  9. Shun Kai Yang
  10. Javier Vargas
  11. Susanne Bechstedt
  12. Jean-François Trempe
  13. Khanh Huy Bui  Is a corresponding author
  1. McGill University, Canada
  2. Kyoto University, Japan
https://doi.org/10.7554/eLife.52760
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Cite this article
  1. Ahmad Abdelzaher Zaki Khalifa
  2. Muneyoshi Ichikawa
  3. Daniel Dai
  4. Shintaroh Kubo
  5. Corbin Steven Black
  6. Katya Peri
  7. Thomas S McAlear
  8. Simon Veyron
  9. Shun Kai Yang
  10. Javier Vargas
  11. Susanne Bechstedt
  12. Jean-François Trempe
  13. Khanh Huy Bui
(2020)
The inner junction complex of the cilia is an interaction hub that involves tubulin post-translational modifications
eLife 9:e52760.
https://doi.org/10.7554/eLife.52760
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Abstract

Microtubules are cytoskeletal structures involved in stability, transport and organization in the cell. The building blocks, the α- and β-tubulin heterodimers, form protofilaments that associate laterally into the hollow microtubule. Microtubule also exists as highly stable doublet microtubules in the cilia where stability is needed for ciliary beating and function. The doublet microtubule maintains its stability through interactions at its inner and outer junctions where its A- and B-tubules meet. Here, using cryo-electron microscopy, bioinformatics and mass spectrometry of the doublets of Chlamydomonas reinhardtii and Tetrahymena thermophila, we identified two new inner junction proteins, FAP276 and FAP106, and an inner junction-associated protein, FAP126, thus presenting the complete answer to the inner junction identity and localization. Our structural study of the doublets shows that the inner junction serves as an interaction hub that involves tubulin post-translational modifications. These interactions contribute to the stability of the doublet and hence, normal ciliary motility.

Introduction

Cilia and flagella are highly conserved organelles present in protists all the way to humans. They are commonly classified into two forms: motile and non-motile cilia. Motile cilia are responsible for mucus clearance in the airway, cerebrospinal fluid circulation and sperm motility (Satir and Christensen, 2007). The non-motile cilia, namely primary cilia, function as the cellular antennas that sense chemical and mechanical changes. Cilia are essential for growth and development and therefore human health. Defects in cilia often result in abnormal motility or stability, which lead to cilia-related diseases such as primary ciliary dyskinesia, retinal degeneration, hydrocephalus and polydactyly (Hurd and Hildebrandt, 2011).

Both cilia types are comprised of a bundle of nine specialized microtubule structures termed doublet microtubules (doublets). Ciliary components, important for motility such as the outer and inner dynein arms, radial spokes and the dynein regulatory complex (DRC) are assembled onto the surface of the doublet (Bui et al., 2008; Bui et al., 2009; Bui et al., 2012; Heuser et al., 2009). Inside the doublets, is a weaving network of proteins, termed microtubule-inner-proteins (MIPs), that bind to the inner lumen surface of the doublet (Ichikawa et al., 2017; Ichikawa et al., 2019). These MIPs act to stabilize the doublet and possibly regulate the ciliary waveform through interactions with the tubulin lattice (Ichikawa et al., 2019).

Doublets consist of a complete 13-protofilament (PF) A-tubule, similar to a 13-PF cytoplasmic microtubule and a partial 10-PF B-tubule forming on top of the A-tubule (naming of the PF number is shown in Figure 1B). To this day there still exists a long-standing question of how the junctions between the two tubules are formed (Tilney et al., 1973; Linck and Stephens, 2007; Nicastro et al., 2011). The recent high-resolution cryo-EM structure of the doublet shows that the outer junction is formed by a non-canonical tubulin interaction among PF B1, A10 and A11 (Ichikawa et al., 2017). The inner junction (IJ), which bridges the inner gap between the B-tubule and A-tubule is formed by non-tubulin proteins. Both primary and motile cilia have been observed to contain the IJ (Nicastro et al., 2011; Sun et al., 2019).

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The IJ structures of Chlamydomonas and Tetrahymena doublet.

(A–D) Surface renderings and schematics of the 48 nm repeat cryo-EM maps of Chlamydomonas (A, B) and Tetrahymena (C, D) doublets viewed from the tip of the cilia. Black arrow indicates longitudinal view in (E), (F) and (G). (E–F) The longitudinal section of the Chlamydomonas doublet at the IJ complex from the inside (E) and outside (F). (G) The longitudinal section of Tetrahymena doublet viewed from the inside. Color scheme: FAP20: dark green; PACRG: gray; FAP52: light green, Y-shaped density: purple; FAP45: yellow green; fMIP-B8B9: orange; Tubulin: light gray; Unknown density: yellow; Rest of MIPs: white; Tether density 1 and 2: red; Tether density 3, pink. Plus and minus ends are indicated by + and - signs. (H) Cross sectional views of the different Tether densities from Chlamydomonas (left) and Tetrahymena (right). In Chlamydomonas, there is a Y-shaped density (purple) that cradles the FAP52 density. The Y-shaped density is absent in Tetrahymena. In Tetrahymena, we observed Tether density 3, which is absent in Chlamydomonas.

In vitro formation of a B-tubule-like hook (i.e. the outer junction like interaction) was assembled onto pre-existing axonemal and mitotic spindle microtubule with the addition of purified brain tubulin (Euteneuer and McIntosh, 1980). More recently, the B-tubule-like hook can be achieved by adding purified tubulins onto existing subtilisin-treated microtubules (Schmidt-Cernohorska et al., 2019). However, these hooks are not closed and appear to be flexible (Schmidt-Cernohorska et al., 2019). This supports the notion that the IJ is composed of non-tubulin proteins that are indispensable to the stability of the IJ.

The IJ is composed of FAP20 as shown through cryo-electron tomography (Yanagisawa et al., 2014). Dymek et al. (2019) reported that PArkin Co-Regulated Gene (PACRG) and FAP20 proteins form the IJ. PACRG and FAP20 are arranged in an alternating pattern to form the IJ linking the PF A1 of A-tubule and PF B10 of the B-tubule. In addition, both FAP20 and PACRG are important components for motility (Yanagisawa et al., 2014; Dymek et al., 2019). Both PACRG and FAP20 are conserved among organisms with cilia, suggesting a common IJ between species.

PACRG shares a bi-directional promoter with the Parkinson’s disease-related gene parkin (Kitada et al., 1998; West et al., 2003). Knockdowns of PACRG genes in Trypanosoma brucei and Xenopus, lead to defects in the doublet structure and, therefore, impaired flagellar motility. In vertebrates, defects in left-right body symmetry and neural tube closure were observed from knockdowns of PACRG (Thumberger et al., 2012). In mice, PACRG knockout results in male sterility (Lorenzetti et al., 2004) and hydrocephalus (Wilson et al., 2010). FAP20 knockout mutants in Chlamydomonas have motility defects and frequent splaying of the axoneme (Yanagisawa et al., 2014). Similarly, FAP20 knockdown in Paramecium has an altered waveform (Laligné et al., 2010). A recent report identified other MIPs near the IJ, namely FAP52 and FAP45 (Owa et al., 2019). Knockouts of FAP52 or FAP45 lead to an unstable B-tubule in Chlamydomonas. Double knockouts of FAP52 or FAP45 together with FAP20 lead to severe damage of the B-tubule. The gene deletion of the human homolog of FAP52 has been shown to cause heterotaxy and situs inversus totalis in patients (Ta-Shma et al., 2015).

Cryo-EM structures of isolated doublets from Tetrahymena show that there are different tethering densities that connect the B-tubule to the A-tubule aside from the IJ (Ichikawa et al., 2017; Ichikawa et al., 2019). However, the identity of such protein remains unknown to date. Taken together, these data suggest that there is a complex interaction at the IJ region involving multiple proteins in addition to PACRG, FAP20, FAP45 and FAP52. These interactions may play a role in regulating ciliary motility via stability.

Despite all the phenotypes known about these IJ proteins, there are not yet any high-resolution structures to explain the molecular mechanism of the B-tubule closure and the IJ stability. In this study, we present the high-resolution cryo-EM structure of the IJ region from the Chlamydomonas doublet. Using a combination of bioinformatics and mass spectrometry, we were able to identify two new IJ proteins, FAP276 and FAP106, and a new IJ-associated MIP, FAP126. Our results suggest that the IJ is made up of a complex of proteins involving PACRG, FAP20, FAP52, FAP276, FAP106 and FAP126. We also compare the Chlamydomonas structure with the Tetrahymena structure to understand the common and species-specific features of the IJ.

Results

Multiple tether proteins exist at the IJ

We obtained the 48 nm repeating unit of taxol stabilized and salt-treated Chlamydomonas doublet at 4.5 Å resolution (Figure 1A,B and Figure 1—figure supplement 1A–C). Due to the salt wash, some MIPs were lost when compared to the intact tomographic doublet structure (dashed parts in Figure 1B) (Bui et al., 2012). On the other hand, the IJ region bridging PF B10 and A1 of the Chlamydomonas doublet remained intact (Figure 1A,B). In the corresponding salt-treated Tetrahymena doublet map, most of the IJ region bridging PF B10 and A1 is missing (Ichikawa et al., 2017; Ichikawa et al., 2019) (Figure 1C,D, more details later). Based on previous studies (Yanagisawa et al., 2014; Dymek et al., 2019; Owa et al., 2019), we were able to localize FAP52, FAP45 in both Tetrahymena and Chlamydomonas (FAP52, light green and FAP45, yellow-green in Figure 1E,G), and PACRG and FAP20 (PACRG, light gray and FAP20, dark gray in Figure 1F) in Chlamydomonas.

In this study, we termed the structure formed by the repeating units of PACRG and FAP20, the IJ protofilament (IJ PF), and refer to the IJ complex as all the proteins involved in the attachment of the B-tubule to the A-tubule. Most of the proteins in this IJ complex are attached to PFs B8 to B10 and the IJ PF.

The presence of the complete IJ PF stabilizes the B-tubule of the Chlamydomonas doublet compared to that of Tetrahymena, as evidenced by local resolution measurements (Figure 1—figure supplement 1D). Despite having a good resolution in the A-tubule, the Tetrahymena doublet has a significantly lower resolution in the IJ area of the B-tubule.

Inside the B-tubule of both species, it is clear that the IJ region is held up by many tether densities along the doublet connecting the B-tubule to PF A13 (Figure 1E–G). First, the B-tubule is held up by Tether density 1 (red, Figure 1H), referred to as MIP3b previously (Ichikawa et al., 2017; Ichikawa et al., 2019). Tether density 1 connects the PF B9/B10 and A13. The second connection is named Tether density 2 (red, Figure 1E–G), projecting from the proximal lobe of the FAP52 density (referred to as MIP3a previously Ichikawa et al., 2017) and connecting to PF A13 (Figure 1H). In Chlamydomonas, there is another Y-shaped density (purple) cradling the FAP52 proximal lobe and projecting into the gap between the IJ PF and PF B10 (Figure 1H).

FAP45 is referred to as MIP3c previously (Owa et al., 2019). Cryo-electron tomography of Chlamydomonas FAP45 mutant indicate it is a L-shaped filamentous MIP binding at the inner ridge between PF B7 and B8 (Figure 1E) (Owa et al., 2019). In both species, the L-shaped FAP45 contacts FAP52 once every 48 nm. This explains the pull-down of FAP45 using FAP52 antibody and vice versa after chemically crosslinking the Chlamydomonas axonemes by a zero-length cross-linker (Owa et al., 2019). In Tetrahymena, there exists a Tether density 3 (pink, Figure 1G,H), projecting from the distal lobe of the FAP52 density and connecting to PF A13. This Tether density 3 is not present in the Chlamydomonas doublet, suggesting that this density is specific to Tetrahymena. All the tether densities described above repeat with 16 nm.

The IJ PF is formed by a pair of PACRG and FAP20 repeating every 8 nm with the same repeating unit as tubulin dimers (Figure 1F). This is to be expected as the purpose of the IJ PF is to bridge the tubulin dimers from PFs B10 and A1. In the 48 nm Chlamydomonas doublet map, there is one PACRG unit with a less defined density compared to the others (dashed box, Figure 1F). It has been shown that there is one PACRG density missing in every 96 nm repeat (Heuser et al., 2009; Dymek et al., 2019). Since our doublet map is a 48 nm repeat unit, the less defined density of PACRG corresponds to the average from one unit of PACRG and one missing unit, that is half the signal. This missing unit of PACRG in the 96 nm repeat allows the basal region of the DRC to anchor onto the doublet (Heuser et al., 2009) (Figure 1—figure supplement 1F,G).

The entire IJ filament of PACRG and FAP20 is previously reported missing in the Tetrahymena structure, probably due to salt wash and dialysis treatment (Ichikawa et al., 2019). However, upon adjusting the threshold value of the surface rendering, we observed one pair of PACRG and FAP20 remaining in the structure (Figure 1—figure supplement 1E) (Ichikawa et al., 2017). This can be a result of a specific region in the 96 nm repeat of the Tetrahymena doublet that has extra interactions to prevent this pair of PACRG and FAP20 to detach during sample preparation.

PACRG, FAP20, FAP52 and FAP276 form an IJ complex

Since the majority of IJ proteins repeat with 8 nm and 16 nm, we first obtained the 16 nm repeating unit from Chlamydomonas and Tetrahymena at 3.9 Å resolution (Figure 1—figure supplement 1C). Using focused refinement, the IJ complex of Chlamydomonas was improved to 3.6 Å resolution (Figure 2A,B). Since the B-tubule is flexible in Tetrahymena, the resolution in the IJ area was significantly lower than that of Chlamydomonas (Figure 1—figure supplement 1D). In contrast, the IJ region of Chlamydomonas has good resolution with the intact IJ PF. It is worth mentioning that PFs A3-A6 in Chlamydomonas have lower resolution due to the loss of MIPs in this region. At 3.6 Å resolution, we were able to segment, trace and de novo model PACRG, FAP20 and FAP52 in Chlamydomonas (Figure 2A,B and Figure 2—figure supplement 1A–F). We could not model FAP45 since FAP45 repeats with 48 nm, and therefore was averaged out in the 16 nm averaged map.

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16 nm structure of Chlamydomonas doublet.

(A, B) 16 nm repeat structure of Chlamydomonas doublet and model at the IJ region. Tubulin densities are depicted as transparent gray, except in A in which tubulins are shown in dark blue. (C) Atomic model of the IJ complex, consisting of PACRG, FAP20, FAP52 and FAP276. Color scheme: FAP20: dark green; PACRG: gray; FAP52: light green, FAP276: purple; tubulin: transparent gray density. (D, E) Maps and models of PF A1 and B10, and IJ PF illustrating how the IJ PF interacts with tubulins. The views are indicated in the schematics. Dashed boxes indicate the views in (F), (G) and (H). Color scheme: α-tubulin: green; β-tubulin: blue; PACRG: gray; FAP20: dark green; FAP276: purple. (F) Electrostatic surface charge of PACRG, FAP20 and α- and β-tubulins of PF A1. Tubulin surface is negatively charged while the interacting interface of PACRG and FAP20 are positively charged. (G) The interaction of the PACRG with the inter-dimer interface of tubulins from PF B10 is shown. H136 from PACRG is conserved and is likely to take part in the interaction with D127 and C129 from α-tubulin of PF B10. (H) The C-terminus of β-tubulin of PF A1 interacts with PACRG and FAP20. Potential residues involved in the interaction of C-tail of β-tubulin and PACRG and FAP20 are shown. (I) Chlamydomonas PACRG has a long N-terminus 1–117. The N-terminus of Chlamydomonas PACRG (red) forms a stable triple helix arrangement with the core of the protein. This is not observed in the human PACRG (PDB: 6NDU) shown in yellow. In addition, the N-terminus of PACRG going into the wedge between PF A13 and A1.

The Y-shaped density is repeating with 16 nm and has a large binding interface with FAP52, we hypothesized that this protein would be missing in FAP52 knockout cells. Therefore, we did mass spectrometry of split doublets isolated from Chlamydomonas FAP52 knockout cells and performed relative quantification of axonemal proteins compared to the wild type (Dai et al., 2019). We observed 12 proteins completely missing (no peptide detected) and 26 proteins reduced by at least twofold (Table 1 and Supplementary Table 1). PACRG, FAP20 and FAP45 levels are unchanged in FAP52 mutants since their binding interfaces with FAP52 are not as large as supported by our structure. The level of tektin, another suggested IJ protein, did not change as well. Using the predicted molecular weight and fold of the density of the Y-shaped density, we identified FAP276 as the Y-shaped density (details in Materials and methods).

Table 1
Proteins completely missing (no peptide detected) in FAP52 knockout mutant
NamesMol. weight
(kDa)		p-values
(WT vs FAP52)		Exclusive unique peptide
counts in WT (quantitative values
after normalization)
ARL3200.00132, 2, 1 (2, 1, 2)
CHLREDRAFT_171815570.0352, 6, 1 (2, 5, 2)
CHLREDRAFT_156073110.0241, 1, 1 (2, 1, 2)
FAP276100.0153, 3, 2 (8, 7, 14)
FAP52660.004627, 21, 15 (59, 73, 105)
FAP36410.00233, 3, 1 (3, 3, 2)
CrCDPK154<0.00013, 5, 2 (3, 4, 4)
CHLREDRAFT_1768301100.0242, 1, 2 (2, 1, 1)
FAP173330.0123, 3, 1 (5, 3, 2)
FAP291120.000452, 3, 2 (3, 3, 4)
CHLREDRAFT_181390410.0281, 1, 1 (1, 1, 2)
ANK2600,00411, 2, 1 (1, 1, 2)

FAP276 supports and mediates the interaction between FAP52 and tubulin (Figure 2C). FAP276 itself forms different contacts with tubulin with both of its N- and C-termini, thus it provides strong anchorage for FAP52 to the tubulin lattice (Figure 2C). Thus, the IJ complex is made up of two copies of PACRG and FAP20, one copy of FAP52 and FAP276 and one copy of Tether density 1 and 2 per 16 nm (Figure 2C). This represents a high stoichiometry compared to other proteins in the axoneme such as CCDC39 and CCDC40, which have only one copy per 96 nm (Oda et al., 2014).

PACRG has an alpha solenoid architecture coupled with a long unstructured N-terminal region (Figure 2—figure supplement 1A). The alpha solenoid architecture is also contained in the microtubule binding TOG domain, which is present in many microtubule polymerases (Brouhard et al., 2008; Leano and Slep, 2019). However, the binding orientation of PACRG to the surface of tubulin is completely different from that of the TOG domain (Leano and Slep, 2019). FAP20 has a beta jelly roll architecture, which consists of mainly β-sheets with a small α-helix. The C-terminus of FAP20 is located at the outside of the doublet, in agreement with a tomographic study of FAP20 Chlamydomonas mutant with a Biotin Carboxyl Carrier Protein tag at the C-terminus (Yanagisawa et al., 2014).

PACRG and FAP20 have two potential microtubule-binding sites, one on the surface of the A-tubule and the other on the lateral side of the B-tubule (Figure 2D,E). The lateral binding site is unique and has never been observed in previously known microtubule-associated proteins. PACRG binds to the inter-dimer interface of PF B10 in the region of MEIG1 binding loop (Khan et al., 2019). In this loop, H136 from PACRG is conserved (Khan et al., 2019) and likely interacts with D127 and C129 of α-tubulin from PF B10 (Figure 2G). FAP20 is sandwiched by the tubulin dimer from PF B10 and the α-tubulin from PF A1 (Figure 2D,E).

The interactions of PACRG and FAP20 with tubulin from PF A1 appear to be electrostatic. The outside surfaces of α- and β-tubulins are highly negatively charged while the corresponding interacting surfaces of PACRG and FAP20 are positively charged (Figure 2F).

In addition to the interactions highlighted above, we also observed the possible interaction of the β-tubulin C-terminus from PF A1 with PACRG (Figure 2E,H). The C-termini of α- and β-tubulins are a hot spot for post-translational modifications such as polyglutamylation and polyglycylation (Wloga et al., 2017). However, due to its flexibility, densities for the α- and β-tubulin C-termini are usually not visible in cryo-EM reconstructions of the microtubules. This is also the case for the outside of the A- and B-tubules in our ex vivo structure. However, in the lumen of the B-tubule, the β-tubulin C-terminus from PF A1 appears to be stabilized by contacts with PACRG and FAP20 (Figure 2H). These contacts stabilize the β-tubulin C-terminus forming a helical turn in segment E432-F436, which otherwise would not be present due to its flexibility (Figure 2H).

The structure of the β-tubulin C-terminus in PF A1 appears to be the result of the steric proximity with the N-terminus of PACRG. This interaction is important in maintaining the stability of the IJ by preventing steric clashing between the two. It could also be an indication of further post-translational modifications that occur in this region, which could have a potential role in IJ formation and stability.

In our structure, we also observe that the distance between FAP20 and the proximal PACRG is closer compared to the distal PACRG, thus PACRG and FAP20 likely form a heterodimer in the axoneme instead of a continuous filament (Figure 3A), except for one missing PACRG unit (Figure 1—figure supplement 1F,G). The PACRG and FAP20 binding interface involves complementary surface charges, suggesting a specific and strong interaction (Figure 3B–D). The loop N225-I260 of PACRG forms β-sheet-like interactions with strand H33-R36 of FAP20 (Figure 3B). In addition, residues Q264 and D258 of PACRG form hydrogen bonds with residue T38 and K20 of FAP20, respectively. This FAP20 binding loop of PACRG is well-conserved among species (Figure 3E), but is not present in the PACRG-like protein, a homolog of PACRG that exists in the basal body (Khan et al., 2019). FAP20, on the other hand, has a high degree of sequence conservation (Figure 3—figure supplement 1).

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Interaction between PACRG and FAP20.

(A) Consecutive molecules of PACRG and FAP20 in the IJ PF. PACRG and FAP20 form a heterodimer as indicated by brackets. (B) Magnified view of the interacting region of PACRG and FAP20. Residues Q264 and D258 of PACRG form hydrogen bonds with residue T38 and K20 of FAP20, respectively. (C, D) Electrostatic interactions between PACRG and FAP20 illustrated by their surface charge. The dashed boxes in (A, C, D) highlight the interacting loops between PACRG and FAP20 (B). (E) Multiple sequence alignment of PACRG in the regions of FAP20-binding loop. Asterisks indicate residues that are involved in FAP20 binding.

The cryo-EM structure of the Chlamydomonas PACRG is highly similar to the crystal structure of the human PACRG binding to MEIG1 (PDB: 6NDU) (Khan et al., 2019), suggesting a conserved role of PACRG. Chlamydomonas PACRG has a long N-terminus that binds on top of PF A13 and into the wedge between PF A1 and A13 (Figure 2I, Figure 2—figure supplement 1A). This N-terminal region is not conserved in humans or Tetrahymena (Khan et al., 2019). This could indicate organism-specific adaptations to achieve finely tuned degrees of ciliary stability.

FAP52 forms an interaction hub and stabilizes α-tubulin’s acetylated K40 loop

Next, we investigated the structure of FAP52 (Figure 2—figure supplement 1E). FAP52 consists of eight WD40 repeats forming two seven-bladed beta-propellers. The two beta-propellers form a V-shape that docks onto PF B9 and B10. The proximal beta-propeller docks onto the inside of the α- and β-tubulin intra-dimer interface, while the distal beta-propeller is aligned with the next inter-dimer interface toward the plus end (Figure 4A).

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Structure of FAP52 and its interaction with tubulins and PACRG.

(A) Structure of FAP52 in a top view from the outside of the B-tubule looking down on the A-tubule. Black arrow indicates the direction of view in (B). (B) Three-point contacts of FAP52 with α-tubulins from PF B9 and B10 and PACRG, indicated by the black dashed boxes. The α-K40 loops are colored red. (C, D) The structure of the α-K40 loop from PF B10. Red dashed boxes indicate the α-K40 loop. (E) Interaction of α-K40 loop of PF B10 with FAP52. FAP52’s K229 is within favorable distance to form hydrogen bonds with the backbone of D39 and T41. Hydrophobic interactions between L226 and I42 and interactions involving R225 are also possible.

The distal beta-propeller of FAP52 has a three-point contact with the inner surface of the B-tubule (Figure 4B). Two of the FAP52 contacts involve the K40 loop of α-tubulin from PF B9 and B10. The α-K40 acetylation was first discovered in Chlamydomonas flagella, which is almost fully acetylated (LeDizet and Piperno, 1987). This α-K40 loop has not been fully visualized in reconstituted studies of acetylated tubulins (Eshun-Wilson et al., 2019; Howes et al., 2014). In our structure, the α-K40 loop is fully structured in this position (Figure 4C,D and Figure 4—figure supplement 1D–G). The density of the α-K40 loop of PF B10 has a higher SNR than the one from B9. Residue K229 of FAP52 is within favorable distance to form hydrogen bonds with the backbone of D39 and T41 of α-tubulin from PF B10. It is also possible that there is a hydrophobic interaction between L226 and I42 (Figure 4E). Residue R225 of FAP52 and D39 of α-tubulin are in an environment where they could interact; however, the side chain densities for both residues are not well-resolved. At the second tubulin contact point, FAP52 segment G142-P144 is in the close proximity of the α-K40 loop from PF B9 (Figure 4B). In the lower region of FAP52, the loop V268-L279 is in close proximity with the N-terminus of PACRG (Figure 4B). The density of the aforementioned loop is not present in the FAP52 structure in Tetrahymena doublet (Figure 4—figure supplement 1A,B). This long loop (V268 to L279) of Chlamydomonas FAP52 is, in fact, deleted in other species (Figure 4—figure supplement 1C). The interaction of this loop with Chlamydomonas PACRG suggests that it is a Chlamydomonas-specific feature that contributes to additional stabilization of PACRG and, hence the IJ PF.

We then investigated the α-K40 loops from Chlamydomonas and Tetrahymena doublets (Figure 4—figure supplement 1D–G). When there is no interacting protein, this loop is flexible consistent with previous literature (Eshun-Wilson et al., 2019). Despite having low resolution in the B-tubule in Tetrahymena, we still observed the α-K40 loop of PF B9 and B10 interacts with FAP52 (Figure 4—figure supplement 1B). We were also able to visualize the α-K40 loop in several locations in both Chlamydomonas and Tetrahymena doublets where there are other proteins interacting with it (Figure 4—figure supplement 1F,G). The conformation of the α-K40 loop appeared to be different depending on its corresponding partner. This suggests that the α-K40 loop might have a role in MIP recognition and binding. Given the numerous interactions of FAP52 with all the proteins in the IJ, FAP52 is likely to function as an interaction hub, which could play an important role during IJ assembly.

FAP106 is the Tether loop, consisting of Tether densities 1 and 2

We were able to trace the Tether density in the 16 nm averaged map. Tether density 1 is connected to Tether density 2 (Figure 5A–D), forming a Tether loop, through which the A- and B-tubules are connected. The loop connecting the Tether density 1 binds on top of PF A12 and then into the outside wedge between A12 and A13 before connecting with Tether density 2. The entire Tether loop is a single polypeptide, conserved between Tetrahymena and Chlamydomonas (Figure 5A–B). Part of this Tether loop resembles Tau binding to the microtubule (Kellogg et al., 2018). There is a small helical region in this loop that binds to α-tubulin of PF A12 (Figure 5—figure supplement 1C,D).

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Structure of the Tether densities.

(A–B) At higher resolution, Tether densities 1 and 2 appear to be a single polypeptide chain in both Chlamydomonas (A) and Tetrahymena (B). Color scheme: tubulin: transparency gray; Tether densities 1 and 2 (Tether loop/FAP106): red; FAP276: purple; PACRG: light gray; Densities between PF A13 and A12 (turquoise). The dashed regions indicate the location of FAP52, which has been digitally removed to show the Tether densities underneath. (C) Model of FAP106 fitted inside the segmented Tether loop from Chlamydomonas. (D) Model of FAP106 tethering the B-tubule and A-tubule. Dashed box indicates view in (E). (E) Helix H3 and H4 of FAP106 insert into the gap formed by four tubulin dimers of PF B9 and B10. (F) Structure of Tether density 3 from Tetrahymena, which binds on top of the wedge between PF A13 and A1. (G) Overlay of the PACRG from Chlamydomonas onto the structure of Tetrahymena shows a hypothetical steric clash of a long Tetrahymena PACRG N-terminus with Tether density 3.

To identify the protein that makes up the Tether loop, we utilized mass spectrometry, bioinformatics and modeling (details in Materials and methods, Figure 5—figure supplement 1A). This allowed us to identify the Tether loop as FAP106. We were able to model segments Q2-P13, P20-A148 and W189-I226 where the density had sufficient signal (Figure 5C,D and Figure 5—figure supplement 1B). Helix H3 and H4 of FAP106 insert into the interdimer interfaces between PF B9 and B10 forming the anchor point to the B-tubule (Figure 5E) while helix H1 and H2 bind to β-tubulin of PF A13 and α-tubulin of PF A12 (Figure 5D). FAP106 is a homolog of ENKURIN (ENKUR), a conserved protein in sperms of many species (Sutton et al., 2004; Jungnickel et al., 2018). Enkur knockout mice have abnormal sperm motility with asymmetric flagellar waveform and therefore low fertility rate (Jungnickel et al., 2018). In addition, mutations in ENKUR is linked to situs inversus in human and mouse (Sigg et al., 2017; Stauber et al., 2017). However, the IQ motif of Enkurin that binds Calmodulin is not conserved in Chlamydomonas (Figure 5—figure supplement 1E).

In Tetrahymena, Tether density 3 connects the distal lobe of FAP52 and binds across the wedge between PF A13 and A1. (Figure 5F). Upon superimposing the Chlamydomonas PACRG structure onto the Tetrahymena IJ area, the N-terminus of PACRG will have a steric clash with Tether density 3 (Figure 5G). This explains the shorter N-terminus of Tetrahymena PACRG relative to the Chlamydomonas PACRG. Tether density 3 might interact with and perform the same function as the N-terminus of PACRG in Chlamydomonas.

FAP126, a FLTOP homolog, interacts with the tether loop, FAP106

Using the same approach as FAP106, we were also able to identify a density that lies on top of PF A13 and goes into the wedge between PF A12 and A13 (Figure 6A, turquoise and Figure 6—figure supplement 1B) as FAP126. FAP126 does not have a homolog in Tetrahymena and is not present in the Tetrahymena map.

Figure 6 with 1 supplement see all
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Structure of FAP126 and its interaction.

(A) View from the top of the PF A12 and A13 showing the density of FAP126 (dark turquoise). Dashed box indicates view in (B). (B) Closeup view of the interactions of FAP126 with the Tether loop, FAP106. T76 and Q77 of FAP126 form hydrogen bonds with Q126 and Q129 of FAP106, respectively. (C) Complimentary electrostatic surface charges of tubulins and FAP126. (D) Electrostatic charge of FAP126 on the tubulin interacting surface. (E) The N-terminus of PACRG and the hook density go into the wedges between PF A12 and A13, and PF A13 and A1, respectively. This likely contributes to the curvature of this region. (F) Inter-PF angles of the A- and B-tubules from Chlamydomonas and Tetrahymena (Ichikawa et al., 2019) showing very similar angle distributions. (G and H) Correlation graphs of consensus normalized expression levels for two selected pairs of genes (ENKURIN(FAP106)/FAP126 and FAP52/FAP126). Tissues showing high levels of expression of one or both genes are labeled. Correlation coefficients (r) are indicated. By excluding testis, corpus callosum, pons and medulla and fallopian tube, the correlation coefficients between ENKUR and FAP126 and between FAP52 and FAP126 are 0.66 and 0.84, respectively.

FAP126 is a homolog of the human FLTOP protein, which is shown to be important for basal body docking and positioning in mono- and multi-ciliated cells (Gegg et al., 2014). Multiple alignment sequence alignment of FAP126 shows that the Chlamydomonas FAP126 lacks the proline-rich regions of other species (Figure 6—figure supplement 1A).

FAP126 appears to interact with FAP106 (Figure 6B). Segment F75-Q77 of FAP126 is in proximity to segment Q126-Q129 of FAP106. T76 and Q77 of FAP126 form hydrogen bonds with Q126 and Q129 of FAP106, respectively (Figure 6B). Therefore, FAP126 might play a role in recruiting FAP106 or vice versa. Almost half of FAP126 density runs along the wedge between PF A12 and A13, close to the tubulin lateral interface with complementary surface charge (Figure 6C,D). FAP126 might act as a low curvature inducer or sensor from the outside similar to Rib43a from the inside since the curvature of A12 and A13 is significantly lower compared to 13-PF singlet (Figure 6E,F) (Ichikawa et al., 2019).

To support whether FAP126 interacts with FAP106, we analyzed the normalized RNA expression of FAP126 with FAP106 (ENKUR) and FAP52 from different human tissues (Figure 6G,H and Figure 6—figure supplement 1D–F). FAP126 showed high correlation with both FAP106 (ENKUR) and FAP52(r = 0.89, p-value=<0.0001, r = 0.94, p-value=<0.0001, respectively) (Figure 6G,H). This indicates that FAP126 might be functionally related to other members of the IJ complex such as FAP106 and FAP52, which further supports the identity of these proteins.

Discussion

In this study, we describe the molecular details of the IJ complex using a combination of mass spectrometry and cryo-EM. The IJ complex in Chlamydomonas is made up of PACRG, FAP20, FAP52, FAP276, FAP106 (Tether loop) and associated proteins such as FAP126 and FAP45 (Figure 7A) and Video 1). We identified two new members of the IJ, FAP106 and FAP276. FAP276, a Chlamydomonas-specific protein, anchors and mediates FAP52’s binding onto tubulins from PF B9 and B10. FAP106 tethers the B-tubule to the A-tubule, through its interactions with the PF A12 and A13, FAP52 and FAP276, while the IJ PF, composed of PACRG and FAP20, closes the IJ gap. For the doublet to withstand the mechanical strain during ciliary beating, it needs proper structural supports. Tektin, a coiled-coil protein, was also proposed to be another component of the IJ complex in Chlamydomonas by biochemical experiments (Yanagisawa et al., 2014). However, no filamentous density corresponding to tektin was found at the IJ PF in our Chlamydomonas map. It suggests that tektin in Chlamydomonas might not be located inside the doublet and is washed out from the salt treatment.

Figure 7
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Inner junction structure and proposed model of IJ formation.

(A) Model of the IJ complex including PACRG, FAP20, FAP52, FAP126, FAP276 and FAP106. FAP45 is not depicted here. Tubulin is depicted as transparent. (B) The B-tubule starts growing laterally from the outer junction side as shown in Schmidt-Cernohorska et al. (2019). PACRG and FAP20 form a heterodimer, which binds onto the outside surface of PF A1. Following this, multiple alternative hypotheses are possible. One hypothesis is that FAP52, FAP276 and FAP106 would bind onto PF A12 and A13. FAP45 and other fMIP proteins would then be incorporated inside the B-tubule, which fixes the proper curvature so that PF B9 and B10 can interact with other IJ proteins. FAP52 binds both PF B9 and B10 through their K40 loops and finally, PACRG and FAP20 interact with the lateral side of PF B10 allowing for B-tubule closure.

Video 1
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The IJ complex of the Chlamydomonas reinhardtii flagella.

Reconstituted doublet microtubules (Schmidt-Cernohorska et al., 2019) indicate that the B-tubule cannot be closed and is extremely flexible without the IJ PF. Therefore, the IJ PF is necessary to dock the B-tubule onto the A-tubule. In our Tetrahymena doublet, in which most of the IJ PF was washed away, even with the presence of FAP52 and FAP106, the doublet is still flexible which can be seen by the lower resolution of the B-tubule compared to the A-tubule (Figure 1—figure supplement 1D). In addition, the B-tubule can be subjected to depolymerization when the IJ PF is not fully formed (Owa et al., 2019). Therefore, the IJ PF serves as an anchor, which might protect the B-tubule from depolymerization by shielding the lateral side of PF B10 (Figure 7B). Because of the complexity of interactions and the diverse protein composition of the IJ complex, it is reasonable to assume that the IJ is assembled after the outer junction nucleates and expands toward the IJ. The IJ complex might be assembled or co-assembled at the same time as PF B10 for the closure of the B-tubule (Figure 7B).

During doublet assembly, the unorderly binding of PACRG and FAP20 to any of the PFs in the B-tubule lateral interfaces would lead to an incomplete B-tubule (Khan et al., 2019). To ensure a successful IJ assembly, chaperones might be needed for the transport of PACRG and FAP20. PACRG forms a complex with MEIG1 (Khan et al., 2019). Even though MEIG1 is not present in lower eukaryotes and the MEIG1 binding loop is not conserved between Chlamydomonas and humans, a chaperone similar to MEIG1 can function to target PACRG to the lateral interface of the PF B10. There is a possibility that PACRG and FAP20 form a heterodimer before their transport and assembly into the cilia. FAP20 shows a similar fold and mode of binding to a class of proteins called carbohydrate-binding modules. Carbohydrate-binding modules form a complex with carbohydrate-active enzymes and are known to have a substrate targeting and enzyme-concentrating function (Hervé et al., 2010). This supports the role of FAP20 as an assembly chaperone in a FAP20-PACRG complex. Furthermore, both studies from Yanagisawa et al. (2014) and Dymek et al. (2019) show reduced endogenous PACRG in Chlamydomonas FAP20 knockout mutant. In the latter study, it was shown that the assembly of exogenous PACRG was less efficient in the FAP20 knockout compared to conditions where FAP20 was intact. This implies that PACRG assembly might indeed depend on FAP20 (Yanagisawa et al., 2014). However, since the expression patterns of PACRG and FAP20 have surprisingly low correlation compared to the rest of the IJ proteins (Figure 6—figure supplement 1F) and homolog of FAP20 exists in non-ciliated organisms such as Arabidopsis, FAP20 might have an additional function outside the cilia.

Furthermore, our atomic models could explain the severe motility phenotypes observed in PACRG and FAP20 mutants compared to FAP52 mutant. Mutants in either PACRG or FAP20 might affect the stability of the DRC, which can severely affect the regulation of ciliary beating. This is supported by the fact that FAP20 mutant is prone to splaying of the cilia (Yanagisawa et al., 2014). Our results could also explain how the double knockout of FAP20 along with FAP45 or FAP52 can affect B-tubule stability at the IJ (Owa et al., 2019). In such conditions, both the IJ PF and the FAP52 or FAP52-mediated anchorage between the A- and B-tubules will be completely lost.

By comparing Chlamydomonas and Tetrahymena, we show that the conserved IJ components are PACRG, FAP20, FAP45, FAP52 and FAP106. There are also species-specific proteins such as FAP276 and FAP126 in Chlamydomonas and Tether density 3 in Tetrahymena. Tether density 3 clashes with a superimposed Chlamydomonas FAP276 structure, suggesting that it takes over its role in mediating the interactions between FAP52 and tubulin in Tetrahymena. This suggests that there is a common framework for the IJ complex in all species. Species-specific proteins may then fine-tune this framework according to the survival needs of the organisms.

In this study, we revealed that FAP106/ENKUR, an important protein for sperm motility, is a MIP and an IJ protein. Knockout of ENKUR leads to the asymmetric waveform of sperm flagella while mutations in ENKUR disturb the left-right symmetry axes in vertebrates. It is shown that ENKUR knockout shows a loss of Ca++ responsiveness while wild-type sperm shows highly curved flagella (Jungnickel et al., 2018). The IQ domain responsible for Ca++ binding of ENKUR is not conserved in the Chlamydomonas sequence, although an alternative means of Ca++ binding or inducing a Ca++-mediated response is still possible.

We also identified FAP126, an IJ-associated MIP. The homolog of FAP126 in human and mouse, the FLTOP protein, exists in the cilia and basal bodies and is thought to function in the positioning of the basal body (Gegg et al., 2014). In Flattop knockout mice, cilia formation in the lung is significantly affected. In the inner ear, Flattop interacts with a protein called Dlg3 in the process of basal body positioning to the actin skeleton in the inner ear. Therefore, it is possible that FAP126 might perform both functions (i) as a MIP that stabilizes the basal body in the same fashion as shown here in the cilia and (ii) in basal body positioning and planar cell polarity (Gegg et al., 2014). The high correlation of FAP126 and FAP106 co-expression, and also with FAP52 in different human tissue suggests they might function similarly or co-operatively in cilia assembly. Tetrahymena, which lacks FAP126, probably implements an alternative mechanism to substitute for FAP126 functions.

Our study demonstrates that all the protein components associated with the IJ complex such as PACRG, FAP20, FAP52, FAP126 and FAP106 in the IJ complex is of high importance for the assembly and proper motility of the cilia. Multiple studies have indeed showed the implication of such proteins in human disease (Lorenzetti et al., 2004; Ta-Shma et al., 2015; Stauber et al., 2017). Remarkably, these proteins are MIPs existing inside the doublet except for PACRG and FAP20. In addition, the structures of the IJ components such as PACRG and FAP126 also highlight the unique roles of the MIPs in curvature induction or sensing as shown previously with Rib43a (Ichikawa et al., 2019). FAP126 binds tightly to the wedge PF A12 and A13 while the N-terminus of Chlamydomonas PACRG penetrates the wedge between PF A13 and A1 and forces the PF pairs into a high-curvature conformation (Figure 6E). From our curvature analysis of the doublet (Figure 6F), this region of PF A12-A1 contains extreme high and low curvatures compared to the 13-PF singlet. Alternatively, the curvature might be enforced by MIPs inside the A-tubule. This inter-PF curvature could help to facilitate the specific binding and anchoring of FAP126 and PACRG to the correct position. It has been shown that doublecortin can sense the curvature of the 13-PF microtubule (Bechstedt and Brouhard, 2012). The Tetrahymena-specific Tether density 3 might act as a high curvature inducer/sensor or an IJ complex stabilizer.

Post-translational modifications in tubulin are known to be important for the activity of the cilia. There have been many studies about the effect of acetylation on the properties of microtubule such as stability (Portran et al., 2017; Xu et al., 2017). In 3T3 cells, the K40 acetyltransferase, αTAT1 promotes rapid ciliogenesis (Friedmann et al., 2012). The absence of acetylating enzymes has indeed been shown to affect sperm motility in mice (Kalebic et al., 2013) while SIRT2 deacetylation decreases axonemal motility in vitro (Alper et al., 2014). A recent cryo-EM study of reconstituted acetylated microtubules showed, using molecular dynamics, that the acetylated α-K40 loop has less conformational flexibility, but a full α-K40 loop in the cryo-EM map has not been visualized due to its flexibility. In this work, we show that the acetylated K40 loop binds to FAP52 and forms a fully structured loop. This loop remains flexible and unstructured when there is no protein interacting with it. This suggests that the α-K40 loop has a role in protein recruitment and interactions, especially, MIPs. We hypothesize that the acetylation disrupts the formation of an intra-molecular salt bridge between K40 and D39, which affects the loop’s sampling conformations and allows D39 to take part in atomic interactions with other proteins. This, in turn, improves the stability of the doublet and therefore, correlates with axonemal motility. In neurons, microtubules are also highly acetylated and are known to be stable. Our hypothesis suggests that in neuron microtubules, there might exist MIPs with a similar stabilizing effect as in the doublet. Previous studies on olfactory neurons demonstrate that there are densities of proteins inside the microtubule, suggesting the existence of MIPs inside cytoplasmic microtubules (Burton, 1984).

Another interesting insight from our study is the structured C-terminus of β-tubulin. The C-termini of tubulin in the doublet normally have polyglycylation and polyglutamylation, in particular, the B-tubule (Lechtreck and Geimer, 2000). In reconstituted microtubules and other places in the doublet, the C-termini are highly flexible and cannot be visualized. However, we observed the C-terminus of β-tubulin in PF A1 which appears to interact with PACRG and FAP20. In addition, the position of FAP126 and FAP106 binding on top of tubulin molecules also suggest they are interacting with the C-termini of tubulins. In vitro study shows that the C-tails of tubulins must be suppressed for the outer junction to be formed (Schmidt-Cernohorska et al., 2019). This suggests that the C-terminus might have a role in the assembly and or stability of the doublet. Defects in tubulin polyglutamylase enzyme have indeed led to partially formed B-tubules (Pathak et al., 2007). This could indicate a role for polyglutamylation in the interaction and recruitment at the IJ PF, specifically PACRG and FAP20. Lack of polyglutamylation can lead to an easily detachable PACRG and FAP20 and hence the partial assembly of the B-tubule. Finally, it is possible that MIPs can act as readers of tubulin post-translational modifications for their orderly recruitment and assembly.

Materials and methods

Preparation of doublet samples

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WT Chlamydomonas cells (cc124) were obtained from Chlamydomonas source center and cultured either on Tris-acetatephosphate (TAP) media with shaking or stirring with 12 hr light-12 hr dark cycle. For flagella purification, Chlamydomonas cells were cultured in 1.5 L of liquid TAP media with stirring until OD600 reached around 0.5–0.6 and harvested by low-speed centrifugation (700 g for 7 min at 4°C). Chlamydomonas flagella were purified by dibucaine method (Witman, 1986), resuspended in HMDEKP buffer (30 mM HEPES, pH 7.4, 5 mM MgSO4, 1 mM DTT, 0.5 mMc, 25 mM Potassium Acetate, 0.5% polyethylene glycol, MW 20,000) containing 10 μM paclitaxel, 1 mM PMSF, 10 μg/ml aprotinin and 5 μg/ml leupeptin. Paclitaxel was added to the buffer since Chlamydomonas doublets were more vulnerable to high-salt extraction compared with Tetrahymena doublets (data not shown). Isolated flagella were demembraned by incubating with HMDEKP buffer containing final 1.5% NP40 for 30 min on ice. After NP40 treatment, Chlamydomonas doublets were incubated with final 1 mM ADP for 10 min at room temperature to activate dynein and then incubated with 0.1 mM ATP for 10 min at room temperature to induce doublet sliding. Since the Chlamydomonas doublets were harder to split compared to Tetrahymena doublet, sonication was done before ADP/ATP treatment. After this, Chlamydomonas doublets were incubated twice with HMDEKP buffer containing 0.6 M NaCl for 30 min on ice, spinned down (16,000 g and 10 min), and resuspended. Chlamydomonas doublets were not dialyzed against low-salt buffer since it was difficult to remove radial spokes.

Tetrahymena doublets were isolated according to our previous work (Ichikawa et al., 2017; Ichikawa et al., 2019).

Cryo-electron microscopy

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3.5 µl of sample of sonicated doublets (~4 mg/ml) was applied to a glow-discharged holey carbon grid (Quantifoil R2/2), blotted and plunged into liquid ethane using Vitrobot Mark IV (Thermo Fisher Scientific) at 25°C and 100% humidity with a blot force 3 or four and a blot time of 5 s.

9528 movies were obtained on a Titan Krios (Thermo Fisher Scientific) equipped with Falcon II camera at 59,000 nominal magnification. The pixel size was 1.375 Å/pixel. Dataset for Tetrahymena was described in Ichikawa et al. (2019). Chlamydomonas dataset was collected with a dose of 28–45 electron/Å2 with seven frames. The defocus range was set to between −1.2 and −3.8 µm.

The Chlamydomonas doublet structures were performed according to Ichikawa et al. (2019). In short, movies were motion corrected using MotionCor2 (Zheng et al., 2017). The contrast transfer function were estimated Gctf (Zhang, 2016). The doublets were picked using e2helixboxer (Tang et al., 2007).

270,713 and 122,997 particles were used for the reconstruction of 16 nm and 48 nm repeating unit of Chlamydomonas. 279,850 particles were used for the 16 nm reconstruction of Tetrahymena. The final Gold Standard FSC resolutions of the 16 nm and 48 nm reconstruction for Chlamydomonas after contrast transfer function refinement and polishing using 0.143 FSC criterion in Relion3 (Zivanov et al., 2018) are 4.5 and 3.8 Å, respectively. Using focus refinement of the IJ of the 16 nm reconstruction for Chlamydomonas, the resolution reaches 3.6 Å. The resolution for the 16 nm reconstruction of Tetrahymena was 3.6 Å. Focus refinement of the IJ of Tetrahymena did not improve the resolution of the IJ due to the flexibility of this region. The maps were local sharpened (Ichikawa et al., 2019). Local resolution estimation was performed using MonoRes (Vilas et al., 2018).

Modeling

Chlamydomonas reinhardtii α-β-tubulin

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A homology model of C. reinhardtii α-β-tubulin (Uniprot sequence α: P09204, β: P04690) was constructed in Modeller v9.19 (Webb and Sali, 2014) using the Taxol structure (PDB ID: 5SYF) as template. The model was refined using real-space refinement (Afonine et al., 2018) and validated using comprehensive validation for cryo-EM in Phenix v1.16 (Adams et al., 2010).

PACRG and FAP20

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A partial homology model of C. reinhardtii PACRG (B1B601) was constructed using the crystal structure of the human homolog (Q96M98-1) as template (Khan et al., 2019). The model was completed by building segments N2-D148 and Y249-L270 de novo in density using Coot v0.8.9.1 (Emsley et al., 2010). The density for segment M89-K101 is missing, likely due to flexibility and or the 16 nm averaging of the cryo-EM data. The missing segment was worked out based on the fact that i) all the surrounding densities have been assigned to the α-β-tubulin heterodimers, ii) there is a 101 long segment of the PACRG N-terminus that is still unassigned to density and iii) the density signature downstream and upstream of the gap matches the sequence identity of the PACRG N-terminus as shown in Figure 2—figure supplement 1B (right side). C. reinhardtii FAP20 (A8IU92) was completely built de novo in density. Both models were refined and validated as described for α-β-tubulin.

FAP52

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The density was traced in Coot v0.8.9.1 (Emsley et al., 2010) based on the topology of a seven-bladed beta propeller (PDB ID: 2YMU), which agrees with the I-TASSER (Yang et al., 2015) tertiary structure prediction of FAP52. The Uniprot sequence for C. reinhardtii FAP52 (A8ILK1, 615 amino acids long) is missing loop V264-K277. This was worked out based on the sequence-density disagreement following Q263. Upon further investigation, a longer sequence in the Uniprot database (633 long) was identified by a blast search (Uniprot ID: A0A2K3D260), which agrees with our electron density and both the Phytozome transcript (Cre12.g489750.t1.2) and the C. reinhardtii FAP52 sequence reported in Owa et al. (2019). Overall, the electron density for FAP52 had less resolution and lower SNR than surrounding proteins. This is likely due to the 16 nm averaging of the cryo-EM data and the heterogeneity of FAP52 due to the 48 nm periodic association with FAP45. The bulky residues of FAP52 were used as anchors to maintain the correct registry in lower resolution areas. The model could be overfit in segment D341-P627 where the density signal is significantly lower. Tracing the backbone of this segment was possible due to the predictability of the seven-bladed beta propeller topology. Furthermore, 7 out of 10 Tryptophan residues of the FAP52 sequence are located within this segment, which served as anchors and allowed us to maintain registry and overfit some side chains where the density was missing. The final model was refined and validated as described above.

FAP276

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After resolving all the proteins in the its environment, the density for the Y-shaped protein was segmented and traced to around 80 amino acids of ~9 kDa in mass. Candidates of approximately this size from the wild-type mass spectrometry data were compared to the FAP52 knockout data and reduced to only FAP276, which was completely missing in the latter (Table 1). The secondary structure prediction (Drozdetskiy et al., 2015) as well as the sequence of FAP276 (Phytozome transcript: Cre04.g216250) agree with the density signature of the Y-shaped region (Figure 2—figure supplement 1G,H). The model was traced, refined and validated as described above.

FAP106

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The trace of the Tether loop was estimated to be ~220–240 amino acids due to missing and likely flexible segments of this protein. To identify the protein that makes up the Tether loop, this protein needs to satisfy the following criteria: (i) has a high stoichiometry (1 per 16 nm of the doublet), (ii) has a minimum molecular weight of ~25 kDa (based on the sequence trace) and (iii) conserved in both Chlamydomonas and Tetrahymena.

We calculated the stoichiometry of proteins in the doublet after salt extraction by normalizing the averaged quantitative spectral count of each protein by their molecular weight. The triplicate mass spectrometry data comes from Dai et al. (2019). The top 35 proteins by copy numbers are shown in Table 2. In our calculation, some radial spoke and central pair proteins displayed high stoichiometry such as RSP9 and PF16. Remarkably, all the IJ proteins are in the top 35 (PACRG, FAP52, FAP20, FAP45 ranked 4, 9, 10 and 35, respectively) as supported by our structure. This validates the quality of the stoichiometry calculation. Although FAP276 should have the same stoichiometry as FAP52, it does not appear in high stochiometric numbers. This can be explained that by the small size of FAP276, which is not well detected in mass spectrometry.

Table 2
Normalized spectral count of proteins detected by mass spectrometry.
NameMolecular
Weight in kDa (MW)		Average quantitative
Value
(AQV)		Rough
Stoichiometric
Peptide
Abundance (RSPA)*		T. thermophila
Homologs**		Human homologs***Localization in
C. reinhardtii
TUA1501077.97215.59TBA_TETTHTUBA1CDoublet
TUB150625.46125.09TBB_TETTHTUBB4BDoublet
RIB7272116.7216.21TTHERM_00143690EFHC1MIP
PACRG2538.3915.35TTHERM_00446290PACRGIJ
PF165074.0914.82TTHERM_000157929SPAG6Central Pair
RSP93041.7913.93TTHERM_00430020RSPH9Radial Spoke
FAP863036.1112.04--Doublet
FAP12226.4612.03--Doublet
FAP526679.1211.99TTHERM_01094880CFAP52MIP
FAP202226.0811.86TTHERM_00418580CFAP20IJ
FAP1261516.8911.26-CFAP126MIP
RSP18898.7311.22TTHERM_00047490RSPH1Radial Spoke
FAP1152729.9811.10TTHERM_00193760-Doublet
FAP1062729.8111.04TTHERM_00137550ENKURIJ?
Tektin5357.6110.87-TEKT5IJ?
RSP35760.5510.62TTHERM_00566810RSPH3Radial Spoke
FAP2523939.9710.25TTHERM_00899430CETN3Axonemal
RSP27777.9510.12-CALM2Radial Spoke
FAP1614343.5010.12TTHERM_00155380CFAP161Axonemal
IDA42927.299.41TTHERM_00841210DNALI1Dynein
FAP1072623.669.10-FLG2Axonemal
DHC2457414.129.06TTHERM_01027670DNAH1Dynein
FAP125448.859.05-DAGLBCytoplasmic
RSP73430.629.01TTHERM_00194419CALML5Radial Spoke
RSP55649.328.81--Radial Spoke
FAP2304539.598.80--Axonemal
FAP772923.888.24TTHERM_00974270CFAP77Axonemal
FAP5511190.478.15-MYH14Axonemal
FAP902822.357.98-WBP11Axonemal
RSP102419.107.96TTHERM_00378600RSPH1Radial Spoke
FAP713224.867.77TTHERM_00077710EWSR1Axonemal
EEF15139.047.66TTHERM_00655820MultipleAxonemal
FAP1824936.697.49TTHERM_01049330C9orf116Axonemal
Rib43a4332.067.46TTHERM_00624660
TTHERM_00641119		RIBC2MIP
FAP455943.207.32TTHERM_001164064CFAP45MIP

  1. *RSPA was calculated by (AQV)/(MW)*10.

    ** T. thermophila homologs were BLAST searched using the Uniprot database.

  2. ***Human homologs were taken from the ChlamyFP project (Pazour et al., 2005).

Among the proteins that have high stoichiometry, the following proteins satisfy the three criteria above: FAP115, FAP106, FAP252, FAP161, FAP77 and FAP71. However, the homologs of FAP115 and FAP161 in Tetrahymena are too big. Our analysis of the secondary structure prediction places FAP106 at the top of the list of candidates for the Tether loop (Figure 5C).

The identity of FAP106 was further confirmed by a blast search against the complete C. reinhardtii proteome using a regular expression pattern that matches the density signature around residue W127 ([FHY]xWxxKxx[FHY]) (Figure 5—figure supplement 1A). The search was restricted for sequences of lengths between 220 and 280 based on the sequence trace. This returned two matches: FAP106 (uniport ID: A8IVJ1) and a transcription factor (uniport ID: A8I9A1). Furthermore, the sequence secondary structure prediction of FAP106 had high confidence in four α-helices and a long-disordered segment, which agrees with the density topology of this protein. As before, the sequence of FAP106 had side chain agreement with the density throughout the entire sequence. Segments Q14-R19, K149-K188 and R227-D240 could not be modeled due to poor density in these areas. Similar to what was described above for PACRG, the disconnected fragments of FAP106 were worked out to be part of the same protein based on resolving all the proteins in its environment, the presence of unassigned segments of FAP106 that need to be assigned to density and the density signature agreement with the sequence (Figure 5—figure supplement 1B). The model was built and refined as mentioned above.

FAP126

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The density for FAP126, which is mostly disordered, was traced as before to 133 amino acids and ~15 kDa in mass. The density had clear side chains signature, particularly in an area where it appeared to have a Tryptophan residue followed by a Proline, five more amino acids and another Tryptophan residues (Figure 6—figure supplement 1C). Doing a blast search against the entire C. reinhardtii proteome, in both C- and N-termini directions, using a regular expression matching the pattern above (WPxxxxxW) gives a single hit: FAP126 (Uniprot ID: A8IVJ1). The search was restricted for sequences of lengths between 128 and 147 residues based on the sequence trace. We also applied the same search strategy as FAP106 to identify this protein. The search criteria were: (i) a high stoichiometry number; (ii) a size of ~15 kDa and (iii) no homolog in Tetrahymena. In this case, the only protein that satisfied these criteria among high stoichiometry proteins (Table 2) was also FAP126. As before, the sequence has matching secondary structure prediction and density signature agreement throughout the entire sequence. The model was modeled and refined as mentioned above.

Inter-PF angle (lateral curvature) measurement

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The inter-PF angle between each PF pair are measured according to Ichikawa et al. (2017).

Visualization

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The maps and models were segmented, coloured and visualized using Chimera (Pettersen et al., 2004) and ChimeraX (Goddard et al., 2018).

Mass spectrometry

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Sample preparation and mass spectrometry of FAP52 mutant and relative quantification compared to wild type Chlamydomonas was done according to Dai et al. (2019). The ratio between the averaged quantitative values from the mass spectrometry (n = 3) and a proteins molecular weight was used to calculate their stoichiometry in the axoneme.

Transcriptomics analysis

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Transcriptomics analysis of PACRG, FAP20, FAP52, FAP126, FAP106, FAP45 and DCX using consensus normalized expression levels for 55 tissue types and seven blood cell types was done according to Khan et al. (2019).

Data availability

Cryo-EM maps have been deposited in EM data bank (EMDB) with accession numbers of EMD-20855 (48-nm averaged Chlamydomonas doublet), EMD-20858 (16-nm averaged Chlamydomonas IJ region) and EMD-20856 (16-nm averaged Tetrahymena IJ region). The model of IJ of Chlamydomonas is available in Protein Data Bank (PDB) with an accession number of PDB: 6VE7. The mass spectrometry is deposited in Dryad (http://doi.org/10.5061/dryad.d51c59zxt).

The following data sets were generated
    1. Bui KH
    (2020) Electron Microscopy Data Bank
    ID EMD-20855. 48-nm repeat unit of the doublet microtubule from Chlamydomonas reinhardtii.
    http://www.ebi.ac.uk/pdbe/entry/emdb/EMD-20855
    1. Bui KH
    (2020) Electron Microscopy Data Bank
    ID EMD-20858. 16-nm averaged Chlamydomonas IJ region.
    http://www.ebi.ac.uk/pdbe/entry/emdb/EMD-20858
    1. Bui KH
    (2020) Electron Microscopy Data Bank
    ID EMD-20856. 16-nm repeat of the doublet microtubule from Tetrahymena thermophila.
    http://www.ebi.ac.uk/pdbe/entry/emdb/EMD-20856
    1. Bui KH
    (2020) RCSB Protein Data Bank
    ID 6VE7. model of IJ of Chlamydomonas.
    http://www.rcsb.org/structure/6VE7

References

    1. Emsley P
    2. Lohkamp B
    3. Scott WG
    4. Cowtan K
    (2010) Features and development of coot
    Acta Crystallographica. Section D, Biological Crystallography 66:486–501.
    https://doi.org/10.1107/S0907444910007493

Article and author information

Author details

  1. Ahmad Abdelzaher Zaki Khalifa

    1. Department of Anatomy and Cell Biology, McGill University, Québec, Canada
    2. Centre de Recherche en Biologie Structurale - FRQS, McGill University, Québec, Canada
    Contribution
    Data curation, Formal analysis, Investigation
    Contributed equally with
    Muneyoshi Ichikawa
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0001-5569-2014

  2. Muneyoshi Ichikawa

    Department of Anatomy and Cell Biology, McGill University, Québec, Canada
    Present address
    Department of Systems Biology, Graduate School of Biological Sciences, Nara Institute of Science and Technology, Nara, Japan
    Contribution
    Data curation, Formal analysis, Investigation
    Contributed equally with
    Ahmad Abdelzaher Zaki Khalifa
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0002-5921-7699

  3. Daniel Dai

    1. Department of Anatomy and Cell Biology, McGill University, Québec, Canada
    2. Centre de Recherche en Biologie Structurale - FRQS, McGill University, Québec, Canada
    Contribution
    Formal analysis, Investigation
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0002-9973-0446

  4. Shintaroh Kubo

    1. Centre de Recherche en Biologie Structurale - FRQS, McGill University, Québec, Canada
    2. Department of Biophysics, Graduate School of Science, Kyoto University, Kyoto, Japan
    Contribution
    Formal analysis, Investigation
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0002-0946-8879

  5. Corbin Steven Black

    1. Department of Anatomy and Cell Biology, McGill University, Québec, Canada
    2. Centre de Recherche en Biologie Structurale - FRQS, McGill University, Québec, Canada
    Contribution
    Formal analysis, Investigation
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0003-2777-6434

  6. Katya Peri

    Department of Anatomy and Cell Biology, McGill University, Québec, Canada
    Contribution
    Formal analysis, Investigation
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0002-7367-7501

  7. Thomas S McAlear

    1. Department of Anatomy and Cell Biology, McGill University, Québec, Canada
    2. Centre de Recherche en Biologie Structurale - FRQS, McGill University, Québec, Canada
    Contribution
    Formal analysis, Investigation
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0001-6097-0103

  8. Simon Veyron

    1. Centre de Recherche en Biologie Structurale - FRQS, McGill University, Québec, Canada
    2. Department of Pharmacology & Therapeutics, McGill University, Montréal, Canada
    Contribution
    Formal analysis
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0002-5533-5268

  9. Shun Kai Yang

    1. Department of Anatomy and Cell Biology, McGill University, Québec, Canada
    2. Centre de Recherche en Biologie Structurale - FRQS, McGill University, Québec, Canada
    Contribution
    Formal analysis
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0002-2363-1441

  10. Javier Vargas

    1. Department of Anatomy and Cell Biology, McGill University, Québec, Canada
    2. Centre de Recherche en Biologie Structurale - FRQS, McGill University, Québec, Canada
    Contribution
    Software, Formal analysis
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0001-7519-6106

  11. Susanne Bechstedt

    1. Department of Anatomy and Cell Biology, McGill University, Québec, Canada
    2. Centre de Recherche en Biologie Structurale - FRQS, McGill University, Québec, Canada
    Contribution
    Formal analysis, Supervision, Funding acquisition
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0002-4706-9975

  12. Jean-François Trempe

    1. Centre de Recherche en Biologie Structurale - FRQS, McGill University, Québec, Canada
    2. Department of Pharmacology & Therapeutics, McGill University, Montréal, Canada
    Contribution
    Formal analysis, Supervision, Funding acquisition, Project administration
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0002-6543-3371

  13. Khanh Huy Bui

    1. Department of Anatomy and Cell Biology, McGill University, Québec, Canada
    2. Centre de Recherche en Biologie Structurale - FRQS, McGill University, Québec, Canada
    Contribution
    Conceptualization, Supervision, Investigation, Project administration
    For correspondence
    huy.bui@mcgill.ca
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0003-2814-9889

Funding

Canadian Institutes of Health Research (PJT-156354)

  • Khanh Huy Bui

Natural Sciences and Engineering Research Council of Canada (RGPIN-2016-04954)

  • Khanh Huy Bui

Natural Sciences and Engineering Research Council of Canada (RGPIN-2018-04813)

  • Javier Vargas

Canadian Institute for Advanced Research (Arzieli Global Scholar Program)

  • Khanh Huy Bui

Japan Society for the Promotion of Science

  • Muneyoshi Ichikawa
  • Shintaroh Kubo

Abdulla Al Ghurair Foundation for Education (Al Ghurair STEM program scholarship)

  • Ahmad Abdelzaher Zaki Khalifa

Canada Research Chairs (950-229792)

  • Jean-François Trempe

Natural Sciences and Engineering Research Council of Canada (RGPIN-2017-04649)

  • Susanne Bechstedt

The funders had no role in study design, data collection and interpretation, or the decision to submit the work for publication.

Acknowledgements

We acknowledge the Facility for Electron Microscopy Research of McGill University where our cryo-EM experiments were conducted, particularly, Drs. Kaustuv Basu and Kelly Sears. We are indebted to Dr. Masahide Kikkawa for sharing the FAP52 knockout Chlamydomonas strain. This research was financially supported by Natural Sciences and Engineering Research Council of Canada (RGPIN-2016–04954), Canada Institute of Health Research (CIHR PJT-156354) and the Canada Institute for Advanced Research Arzieli Global Scholars Program to KHB, MI and SK were supported by Japan Society for the Promotion of Science (JSPS) for JSPS Overseas Research Fellowships and JSPS Overseas Challenge Program for Young Researchers, respectively. AAZK is supported by CIHR and the Al Ghurair Foundation for Education. We declare no competing financial interests.

Version history

  1. Received: October 15, 2019
  2. Accepted: January 16, 2020
  3. Accepted Manuscript published: January 17, 2020 (version 1)
  4. Version of Record published: January 31, 2020 (version 2)

Copyright

© 2020, Khalifa et al.

This article is distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use and redistribution provided that the original author and source are credited.

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  1. Ahmad Abdelzaher Zaki Khalifa
  2. Muneyoshi Ichikawa
  3. Daniel Dai
  4. Shintaroh Kubo
  5. Corbin Steven Black
  6. Katya Peri
  7. Thomas S McAlear
  8. Simon Veyron
  9. Shun Kai Yang
  10. Javier Vargas
  11. Susanne Bechstedt
  12. Jean-François Trempe
  13. Khanh Huy Bui
(2020)
The inner junction complex of the cilia is an interaction hub that involves tubulin post-translational modifications
eLife 9:e52760.
https://doi.org/10.7554/eLife.52760

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