To address how hair bundles are established across the LPR in the macular organs, we first live-imaged centriole movements as a proxy for hair bundle orientation establishment in medial utricular HCs (Md HCs) of Atoh1^Cre; Rosa^tdT/+; CAG:GFP-Centrin2 mice at embryonic day (E) 13.5, in which all centrioles are GFP-positive and nascent HCs are tdTomato-positive (Figures 2A,C–E and 3A–C). At this stage, most of the nascent HCs are located in the Emx2-negative, medial region of the utricle and few are in the Emx2-positive, lateral region (Figure 2A; Jiang et al., 2017; Yang et al., 2017). Some of the Md HCs are already polarized with the kinocilium asymmetrically located at the lateral periphery of the apical surface, whereas other immature HCs show the kinocilium at the center of the apical surface (Figure 2A, Figure 2—figure supplement 1). In the course of our experiments, we tracked centriole movements in a total of 32 nascent Md HCs for 40.8 hr. Figures 2 and 3 illustrate the locations of two of these HCs (Figure 2C, Md HC1, Figure 3A, Md HC2) and their centriole movements (Figures 2D–E and 3B–C). The trajectories of centriole movements (Figure 2D–D’ and Figure 3B–B’) and selected frames of the time-lapse recordings (Figures 2E and 3C) are shown. The identity of the MC (Figures 2D–E and 3B–C, Figure 2—figure supplement 1, yellow color) was determined based on its more apical location within the HC than the DC (Figures 2D–E and 3B–C, Figure 2—figure supplement 1, orange color; Sipe and Lu, 2011). The identity of the MC was further validated by its association with the kinocilium marker, Arl13b (Figure 2—figure supplement 1).

Figure 3 with 3 supplements see all

Download asset Open asset

Figure 3—source data 1

Coordinates of centriole positions relative to the center of the cell in Md HC2, Md HC3, and Md HC4.

https://cdn.elifesciences.org/articles/59282/elife-59282-fig3-data1-v2.xlsx

Download elife-59282-fig3-data1-v2.xlsx

Figure 3—source data 2

Quantification of daughter centriole trajectories in Atoh1^Cre; Rosa^Emx2/tdT; CAG:GFP-Centrin2 and Gfi1^Cre; Rosa^Emx2/tdT; CAG:GFP-Centrin2 utricles.

https://cdn.elifesciences.org/articles/59282/elife-59282-fig3-data2-v2.xlsx

Download elife-59282-fig3-data2-v2.xlsx

Based on tracking and analyses of trajectories and relationships between the MC and DC in Md HCs, two phases of centriole movements emerged (Figure 2C–E, Figure 2—figure supplement 2, Figure 2—video 1). In Phase I, the MC (yellow arrowhead) was positioned near the center of HC’s apical surface, whereas the DC (orange arrowhead) moved rapidly and sporadically around the MC (Figure 2D#1, 2E#1–3, 3B#1, 3C#1–3). The x-y and z distances between the two centrioles were variable during Phase I (Figure 2—figure supplement 2, A,C), in which the two centrioles could be far apart (Figure 3C#1) or aligned along the apical-basal axis (Figure 2E#3, 3C#3). The speed of the DC was also faster, up to 1.2 μm per a 10-min time frame (orange), whereas the speed of the MC (yellow) was more stable, not exceeding 0.5 μm per time frame after correcting for HC drift (Figure 2—figure supplement 2B, Md HC1: p=2.0×10⁻⁸, Md HC2: p=0.015, Figure 2—figure supplement 2—source data 1). By contrast, Phase II was characterized by the DC showing directional movements toward the lateral utricle (Figure 2D#2, 2D’, 2E#4–5, 3B#2, 3B’, 3C#4) where the kinocilium of Md HCs will subsequently reside in the lateral periphery (white arrow). Then, the MC migrated towards the direction of the DC (Figure 2D#3–4, 2E#6–7, 3B#3–4, 3C#5–6). The DC continued to move faster than the MC in Phase II (Figure 2—figure supplement 2B, Md HC1: p=1.8×10⁻⁶, Md HC2: p=4.7×10⁻⁶, Figure 2—figure supplement 2—source data 1) and the average x-y distance between the two centrioles in Phase II was significantly larger than Phase I but the z-distance was smaller in Phase II than Phase I (Figure 2—figure supplement 2A,C, Md HC1: x-y distance, p=1.9×10⁻¹⁰, Figure 2—figure supplement 2—source data 2, z-distance, p=7.0×10⁻⁶, Md HC2: x-y distance, p=2.0×10⁻⁵, z-distance, p=1.0×10⁻⁵, Figure 2—figure supplement 2—source data 3). Between 24 to 40.8 hr of recording, the two centrioles were observed to relocate again towards the center of HC as a pair and maintaining the relative positions between each other (Figure 2D#5–6, 2E#7–10, 3B#5-#6, 3C#6–7). This movement resembled what was previously described for the kinocilium being shifted centrally due to formation of the bare zone comprised of the LGN/Insc/Gαi complex (Tarchini et al., 2013).

Hair bundles in the lateral utricle are in opposite orientation from the default hair bundles in the medial utricle (Figure 1A). We investigated whether centrioles in the Emx2-positive lateral HCs (Lat HCs) migrate directly to their destinated position in the medial periphery or they first migrate to the lateral position before relocating to the medial destinated position (Figure 2B). Since most of the HCs in the lateral utricle initiate terminal mitosis at E14.5 or later (Jiang et al., 2017), live-imaging of E13.5 utricular explants was analyzed for 41 hr (Figure 2F–H, Figure 2—figure supplement 3, A–E). At the beginning of recordings, tdTomato-positive HCs were only found in the medial utricle. Sixteen hr into imaging, several HCs emerged in the lateral region of the utricle and their centrioles were positioned in the medial periphery of the apical surface of the HCs by the end of the recording (Figure 2F, Lat HC1, Figure 2—figure supplement 3A, Lat HC2). Based on the positions of HCs at the end of the recordings, we re-traced and analyzed the centriole trajectories of 9 Lat HCs. Trajectories of centrioles in Lat HCs can also be grouped into two phases similar to Md HCs. In Phase I, the DC moved sporadically around the MC before or soon after the tdTomato signal was evident (Figure 2G#1–2, 2H#1–4, Figure 2—figure supplement 3, B#1–2, C#1–4, Figure 2—video 2). Then, in Phase II, the DC started to migrate towards the medial side, which was followed by the MC (Figure 2G#3–4, 2G’, 2H#5–7, Figure 2—figure supplement 3B#3–4, B’, C#5–7). Similar to Md HCs, the average x-y and z distances between the two centrioles were variable but the x-y distance was closer in Phase I than Phase II, but the z-distance was further apart in Phase I than Phase II (Figure 2—figure supplement 3, D,F, Lat HC1: x-y distance, p=2.7×10⁻¹¹, Figure 2—figure supplement 3—source data 2, z–distance, p=3.0×10⁻⁴, Figure 2—figure supplement 3—source data 3, Lat HC2: x-y distance, p=1.7×10⁻¹⁷, z-distance, p=3.8×10⁻³). Average moving speed of the DC was faster than that of the MC in each phase, although three out of nine Lat HCs failed to show a significant difference in speed between the two centrioles in Phase II (Figure 2—figure supplement 3E, Lat HC1: Phase I p=0.0078, Phase II p=0.028, Lat HC2: Phase I p=0.048, Phase II p=0.17, Figure 2—figure supplement 3—source data 4). These centriole trajectories in HCs were not observed in supporting cells in either the medial or lateral utricle (Figure 2—figure supplement 4, Figure 2—figure supplement 4—source data 1, Figure 2—figure supplement 4—source data 2). Centrioles in supporting cells behaved in a similar manner as centrioles in Phase I HCs, with the DC showing an inconsistent position in relationship to the MC.

Thus far, our analyses revealed that Md HCs and Lat HCs show similar centriole trajectories in reaching their destinations in opposite sides of the HC. The two centrioles in the Lat HC moved directly toward the medial periphery (Figure 2B#1) without first reaching the lateral periphery like in the Md HC and then relocated to the medial periphery (#2). These results indicate that Emx2 has already exerted its effects on the Lat HCs prior to hair bundle establishment. Notably, Emx2 transcripts are detected in the lateral region at E11.5, three days ahead of HC formation that begins at E14.5 (Figure 2—figure supplement 5; Jiang et al., 2017). Taken together, these results suggest that the mechanism of Emx2 in altering hair bundle orientation in the lateral utricle could be indirect via possible regional patterning and/or HC fate determination.

To gain further insight into the mechanism of Emx2 in altering hair bundle orientation, we investigated the time it takes for ectopic Emx2 to reverse hair bundle orientation in Md HCs (Jiang et al., 2017). Since Emx2 transcripts are detected in the lateral utricle three days earlier than Lat HC formation (Figure 2—figure supplement 5; Jiang et al., 2017), we reasoned that if endogenous Emx2 mediates hair bundle reversal via patterning or cell-fate change, effects of ectopic Emx2 may be similar and could take days to reverse hair bundle orientation. We crossed two different strains of cre mice, Atoh1^Cre or Gfi1^Cre to Rosa^Emx2 mice, which resulted in some offspring showing specific expression of Emx2 in all the HCs. Both Atoh1 and Gfi1 are transcription factors important for HC formation (Bermingham et al., 1999; Wallis et al., 2003), and lack of Atoh1 or Gfi1 results in loss of HCs. Atoh1 is the earliest known transcription factor that commits HC fate in the inner ear (Bermingham et al., 1999; Zheng and Gao, 2000). However, Atoh1 expression is not affected in Gfi1 knockout mice, suggesting that Gfi1 is required later than Atoh1 during HC differentiation (Wallis et al., 2003). Thus, the induction of Emx2 using Gfi1^Cre is expected to be later than that of Atoh1^Cre in the HC lineage.

We first live-imaged Atoh1^Cre; Rosa ^Emx2/tdT; CAG:GFP-Centrin2 utricles (Figure 3D–F), in which all Md HCs showed opposite hair bundle orientation from controls by E15.5 (Figure 3—figure supplement 1). Live-imaging results showed that the trajectory of centrioles in Md HCs ectopically expressing Emx2 showed the DC moving around the MC sporadically (Figure 3E#1, 3F#1–4), similar to normal Md HCs at Phase I (Figure 3B#1, 3C#1–3). Then, the DC migrated toward the medial periphery (Figure 3E#2, 3E’, 3F#5, yellow arrow, Figure 3—source data 1, Figure 3—video 1), opposite from the normal lateral direction (Figure 3F, white arrow) and controls (Figure 3B–C). This trajectory was followed by the MC (Figure 3E#3, 3F#6–7). This pattern of centriole migration from center of the HC to the medial edge occurred in 60% of the HCs analyzed (Figure 3J, Figure 3—source data 2). The remaining HCs exhibited a pattern that is similar to the Gfi1^Cre; Rosa^Emx2/tdT Md HCs described below, suggesting that there are two modes of centriole trajectory.

In Gfi1^Cre; Rosa^Emx2/tdT utricles (Figure 3G–I), in which all the hair bundle orientation in Md HCs are known to be reversed (Jiang et al., 2017), live imaging results showed that some of the centriole trajectories were different from those in Atoh1^Cre; Rosa^Emx2/tdT utricles (Figure 3G–J, Figure 3—figure supplement 2, A–C, Figure 3—source data 2, p=0.0010). At the beginning of the recording, Gfi1^Cre; Rosa^Emx2/tdT Md HCs analyzed already showed tdTomato expression and the DC was asymmetrically located towards the lateral side (Figure 3H#1, 3I#1, Md HC4, Figure 3—figure supplement 2C–C”#1, Md HC5-7, white arrow, Figure 3—video 1), resembling Md HCs at Phase II (Figure 3C). Within 3 hr (Figure 3—figure supplement 2, C’#1–3, Md HC6, Figure 3—figure supplement 2—source data 1) to 9 hr (Figure 3I#1–4, Md HC4, Figure 3—figure supplement 2, C” #1–4 Md HC7) of recordings, the DC remained lateral to the MC. Thereafter, the distance between the DC and MC was reduced and sometimes the two centrioles were transiently aligned along the apical-basal axis (Figure 3I#5 Md HC4, Figure 3—figure supplement 2, C#5–6 Md HC5, C’#5–6 Md HC7, Figure 3—figure supplement 2—source data 1). Then, the DC switched position to the medial side of MC (Figure 3H#3, 3H’, 3I#6–7, Figure 3—figure supplement 2, C–C”, yellow arrow). These results suggest that in Gfi1^Cre; Rosa^Emx2/tdT Md HCs, the centrioles are initially aligned in the normal lateral positions primed for hair bundle establishment but upon activation of Emx2 transcription mediated by Gfi1-driven Cre, the two centrioles reverse their positions to the medial side. This lateral to medial centriole reversal pattern was also observed in Atoh1^Cre; Rosa^Emx2/tdT utricles but at a lower frequency than Md HCs of Gfi1^Cre; Rosa^Emx2/tdT (Figure 3J, 40% vs 84.6%, p=0.0010, Figure 3—source data 2). These frequency differences in migration patterns between the two cre lines are consistent with the notion that Emx2 activation using Gfi1^Cre is later than Atoh1^Cre, thus a higher percentage of centrioles in Gfi1^Cre samples were observed to migrate from the destinated lateral periphery toward the medial rather than directly from the central toward the medial position (Figure 3J, 60% vs 15.4%). Furthermore, our results indicate that centriole trajectory during both Phase I and Phase II is plastic and can be altered by Emx2.

Our time-lapse recordings showed that the longest time observed for Gfi1^Cre; Rosa^Emx2/tdT Md HCs to reverse centriole positions from the lateral to medial periphery was approximately 12 hr (Figure 3, Md HC4, Figure 3—figure supplement 2, Md HC7) suggesting that Emx2 could exert its effects on hair bundle reversal within hours. However, the precise time frame between the onset of Emx2 expression driven by Gfi1-Cre and reversal of centriole positions remains unclear. To further investigate the time required by Emx2 to alter hair bundle orientation, we ectopically expressed Emx2 in utricular explants using AAV2.7m8 adeno-associated virus, which has been shown to infect cochlear HCs efficiently (Isgrig et al., 2019). We infected CAG:GFP-Centrin2 utricular explants at E13.5 with an AAV2.7m8 adeno-associated viral vector, AAV2.7m8-CAG-Emx2-P2A-tdTomato (AAV-Emx2-tdT), in which both Emx2 and tdTomato transcripts were driven under the universal CAG promoter. Forty-eight hr after infection, approximately 70% of total HCs were infected (Figure 4C, 71.1 ± 6.3% with AAV-Emx2-tdT, Figure 4—source data 1), which was similar to AAV-tdT controls (72.8 ± 5.6%). The void of anti-β2-spectrin staining indicates the kinocilium position in the apical HC surface and reveals the hair bundle orientation (Deans et al., 2007). In AAV-tdT controls, infected HCs showed normal hair bundle orientation (Figure 4A, white arrows, 4C). However, 13.9 ± 7.2% of HCs infected with AAV-Emx2-tdT showed opposite kinocilium position (Figure 4B yellow arrows, 4C) versus none in controls, indicating that AAV-Emx2-tdT is sufficient to reverse hair bundle orientation. The efficiency of changing kinocilium position was not correlated with the expression levels of ectopic Emx2 (Figure 4E, Figure 4—source data 2), as we found high Emx2 expressors with normal bundle orientation (Figure 4D and D’, white arrow with double arrowheads). At the same time, although high Emx2 expressors were found with opposite bundle orientation (yellow arrow with asterisk) from the normal orientation (white arrows), low Emx2 expressors could also change bundle orientation equally well (Figure 4D’, yellow arrow with arrowhead).

Figure 4

Download asset Open asset

Figure 4—source data 1

Efficiency of infections and hair bundle reversal phenotype mediated by control (AAV-tdT) and AAV-Emx2-tdT viruses.

https://cdn.elifesciences.org/articles/59282/elife-59282-fig4-data1-v2.xlsx

Download elife-59282-fig4-data1-v2.xlsx

Figure 4—source data 2

Correlation of Emx2 expression levels with hair bundle orientation.

https://cdn.elifesciences.org/articles/59282/elife-59282-fig4-data2-v2.xlsx

Download elife-59282-fig4-data2-v2.xlsx

Next, we live-imaged the centriole reversal process in AAV-Emx2-tdT infected CAG:GFP-Centrin2 utricular cultures (Figure 5A). At 24 hr after viral infection, the majority of the cells in the utricular explants were tdTomato-negative (Figure 5B) but many HCs turned on tdTomato by 36 hr after infection (Figure 5E and F). At the beginning of recordings, most of the infected Md HCs showed the DC lateral to the MC, even though the outline of the HCs was not evident yet due to the lack of tdTomato signal (Figure 5C#1, D#1, E, F, Figure 5—video 1). As tdTomato expression became apparent, the peripheral location of the two centrioles was confirmed, indicating that these cells were at late Phase II (Figure 5E–F, Md HC8, 21 hr, Md HC9, 13 hr). Then, the two centrioles moved to align longitudinally with each other transiently (Figure 5E–F, small panel insets, 22.3 hr for Md HC8 and 15 hr for Md HC9), followed by the DC moving medial to the MC (Figure 5C#3, 5C’, 5E 24–25.3 hr, Md HC8, 5D#3, 5D’, 5F 21–25.3 hr, Md HC9), suggesting a change in the course of DC trajectory from lateral to medial periphery. Quantification of tdTomato signal that was above background in infected cells showed that tdTomato signals were elevated by 9–12 hr of imaging (Figure 5A,G, 1.5 days after infection), although the signals may not be apparent in the single time frame images (Figure 5E,F). Then, DC positional reversal occurred within 10–12 hr after the detectable tdTomato signals. Using positive tdTomato signals as a proxy for Emx2 activation, these results suggest that Emx2 can reverse centriole trajectory within 10–12 hr. Thus, both the viral approach using AAV and genetic approach using Gfi1^Cre; Rosa^Emx2/tdT utricles suggest that Emx2 is able to mediate hair bundle reversal within a short period of time (Figure 5H) despite onset of endogenous Emx2 expression occurring 3 days prior to HC formation (Figure 2—figure supplement 5).

Figure 5 with 1 supplement see all

Download asset Open asset

Figure 5—source data 1

Coordinates of centriole positions relative to the center of the hair cell (HC) or the mother centrioles (MCs) in Md HC8 and Md HC9.

https://cdn.elifesciences.org/articles/59282/elife-59282-fig5-data1-v2.xlsx

Download elife-59282-fig5-data1-v2.xlsx

Thus far, our live-imaging results indicate that the migration of the DC always preceded that of the MC under either control or treated conditions. To identify potential qualitative differences between the two centrioles that could account for the migration pattern, we investigated their association with microtubules and proteins related to microtubule nucleation and anchoring. Using SiR-tubulin, a cell permeable fluorogenic probe for microtubules, we labeled microtubules in live Atoh1^Cre; Rosa^tdT/+; CAG:GFP-Centrin2 utricular cultures. We showed that both centrioles were associated with microtubules in tdTomato-positive HCs determined to be Phase II, based on the position of the centrioles (Figure 6A). Immunostaining with anti-γ-tubulin antibodies indicated that both centrioles in Phase II HCs are associated with microtubule nucleation (Figure 6B). Ninein is a centrosomal protein that has both microtubule nucleation and anchoring functions (Delgehyr et al., 2005) and it is preferentially associated with the MC than the DC in somatic cells, serving its microtubule nucleation role (Betleja et al., 2018; Piel et al., 2000). In Phase I HCs, in which centrioles are centrally located, ninein staining was concentrated by the two centrioles (Figure 6C, Phase I, n = 6). As DC started to migrate towards the periphery and the two centrioles became further apart, ninein staining became broadly distributed surrounding both centrioles (Figure 6C, early Phase II, n = 17). However, ninein staining was concentrated at the centrioles again at late Phase II (Figure 6C, n = 21). Even though the association of ninein with specific centrioles or the location in between the two centrioles is inconsistent and does not distinguish between the two centrioles (Figure 6E, Figure 6—source data 2), the broad distribution of ninein staining beyond the centrioles during centriole migration is significantly different from other stages of the trajectory (Figure 6D, Phase I vs early Phase II, p=0.0005; early Phase II vs late Phase II, p=0.0025; Phase I vs late Phase II, p=0.21, Figure 6—source data 1). This broad distribution of ninein staining beyond the centrioles during centriole migration suggests that ninein may serve as microtubule anchoring during this period.

Figure 6

Download asset Open asset

Figure 6—source data 1

Quantification of ninein area in hair cells (HCs) during each phase of centriole migration.

https://cdn.elifesciences.org/articles/59282/elife-59282-fig6-data1-v2.xlsx

Download elife-59282-fig6-data1-v2.xlsx

Figure 6—source data 2

Anti-ninein staining intensity associated with the mother centriole (MC), daughter centriole (DC) and area in between the centrioles.

https://cdn.elifesciences.org/articles/59282/elife-59282-fig6-data2-v2.xlsx

Download elife-59282-fig6-data2-v2.xlsx

Previous reports in cochlear explants proposed that microtubule plus ends attached to the LGN/Insc/Gαi complex relocate the MC/kinocilium through microtubule shortening and/or dynein mediated mechanism to the periphery (Ezan et al., 2013). Blocking Gαi with pertussis toxin disrupted the microtubule plus-end binding protein, EB1 and the kinocilium positioning. We tested this hypothesis in our live utricular culture and asked whether the DC behaves in a similar manner as MC. We treated utricular explants with nocodazole, which disrupts the microtubules by binding to free tubulin dimers and inhibits microtubule polymerization (Hoebeke et al., 1976) and we analyzed nocodazole effects on all stages of centriole migration (Figure 7). Nocodazole was introduced for 1 hr at 1.5 hr into the live-imaging and recording continued for 5.5 hr after drug removal (Figure 7A). In Phase I HCs, in which centrioles were centrally located at the beginning of the recording (Figure 7B#1, 7C 0–1.3 hr), centrioles remained in the apical center of the HC even though the DC continued to move around the MC during nocodazole treatments (Figure 7B#2, 7C 1.5–2.3 hr). After drug removal, some of the HCs showed migration of DC towards the periphery (Figure 7B#3-#4, 7C 3.5–8 hr, n = 3 out of 6 HCs analyzed). The rest of the Phase I HCs remained in Phase I for 5.5 hr after nocodazole removal (not shown). In early Phase II HCs where there was a bigger distance between the centrioles and the DC was positioned closer to the periphery (Figure 7D#1, 7E 0–1.3 hr), nocodazole treatments caused the DC to move centrally (Figure 7E 1.5–2.3 hr, 7D#2, 7D’). The DC continued to move sporadically around the MC (Figure 7D#2, 7E 1.5–2.3 hr), resembling the behavior observed in Phase I of nascent HCs (Figure 2). After nocodazole removal, the DC started to migrate towards the periphery again ahead of the MC (Figure 7D#4, D’, 7E 3.5–8 hr, n = 11 out of 12 HC analyzed).

Figure 7 with 2 supplements see all

Download asset Open asset

Figure 7—source data 1

Coordinates of centriole positions relative to the center of the cell for Md HC10, MD HC11 and Md HC12.

https://cdn.elifesciences.org/articles/59282/elife-59282-fig7-data1-v2.xlsx

Download elife-59282-fig7-data1-v2.xlsx

HCs at the late Phase II show both centrioles located in the periphery (Figure 7F#1, 7G 0–1.3 hr). Similar to the phenomenon observed with HCs at the beginning of Phase II (Figure 7D–E), both centrioles returned to the center of the HC in the presence of nocodazole within 30 min (Figure 7F#2, 7F’, 7G 1.5–2 hr, Figure 7—source data 1, Figure 7—figure supplement 1, Figure 7—figure supplement 1—source data 1), and the DC continued to move sporadically around the relatively stable MC (Figure 7F#2, 7G 2–2.3 hr). Once nocodazole was washed out, two centrioles returned to the lateral periphery within a few hr with the DC moving ahead of the MC (Figure 7F#3-#4, 7F’, 7G, 3.5–8 hr, Figure 7—video 1, n = 17 out of 18 HCs analyzed). These results indicate that both the DC and MC respond to nocodazole treatments in a similar manner. Furthermore, acetylated-tubulin staining of HCs, which labels stable microtubules, showed a loss of tubulin arrays along with mislocalized DC and MC from the periphery during nocodazole treatment (Figure 7H). After nocodazole removal, tubulin arrays were re-established and both centrioles recovered their positions in the periphery (Figure 7I). Together, these results suggest that both the DC and MC are dependent on an active force that translocate them to the periphery via an intact microtubule network.

Nocodazole treatments affected centriole migration at E13.5. However, we observed some HCs with peripherally located centrioles (late Phase II) that were unaffected by 1 hr of nocodazole treatments (n = 8 out of 30 HCs analyzed). It was not clear whether these HCs required longer than 1 hr of exposure to nocodazole in order to respond or they represented HCs that were more mature and thus insensitive to microtubule disruption. To distinguish these possibilities, we treated E13.5 and E14.5 utricle explants with nocodazole for 6 hr and followed centriole trajectories in HCs (Figure 8). We reasoned that if the non-responsive HCs at E13.5 represented more mature HCs, then this population of HCs should increase in older utricles at E14.5. We observed that 6 hr of nocodazole treatments at E13.5 resulted in rapid central migration of centrioles within an hr (Figure 8B#2, 8C 1.7–2 hr, 8G), similar to treatments for 1 hr (Figure 7), and the centrioles stayed in the center with the DC in variable positions relative to the MC (Figure 8B#2-#4, 8C 2–7.7 hr). However, a majority of the HCs at E14.5 did not respond to nocodazole treatments in a similar manner. Only 20% of the HCs analyzed showed their centrioles moved away from the periphery within the first hr, compared to 60.3% of the HCs at E13.5 (Figure 8G, p=0.000089, Figure 8—source data 2) and the relative positions between the two centrioles always maintained with the DC being more lateral than the MC (Figure 8E#2-#3, 8F 1.7–3.5 hr). By the end of the experiment, although the two centrioles seemed more centrally displaced, the apical surface of the HC was also reduced (Figure 8E#3, 8F 7.7 hr). It is not clear whether the central migration of the centrioles by the end of the experiment was secondary due to reduction of the apical HC surface. Although the apical surface of HCs at E13.5 also appeared smaller by 6 hr of nocodazole treatments (Figure 8C 7.7 hr), the response of centrioles to nocodazole was much more acute and profound at E13.5 than E14.5. Together, these results suggest that as HCs mature, they are less sensitive to microtubule disruption.

Figure 8

Download asset Open asset

Figure 8—source data 1

Coordinates of centriole positions relative to the center of the cell for Md HC14 and MD HC15.

https://cdn.elifesciences.org/articles/59282/elife-59282-fig8-data1-v2.xlsx

Download elife-59282-fig8-data1-v2.xlsx

Figure 8—source data 2

Timing of the daughter centriole (DC) to lose its peripheral position under nocodazole treatments.

https://cdn.elifesciences.org/articles/59282/elife-59282-fig8-data2-v2.xlsx

Download elife-59282-fig8-data2-v2.xlsx

Thus far, our results showed no difference between the DC and MC in their association with the microtubule network and nucleation center as well as their response and recovery from nocodazole treatments. Lastly, we investigated the association of the polarity complex, LGN/Insc/Gαi, with centriole migration. We correlated the timing of centriole trajectory with the formation of the LGN/Insc/Gαi complex using anti-Gαi antibody staining as well as formation of the cuticular plate using anti-spectrin antibody. Our results showed that during Phase I when both centrioles were at the center of the HC, Gαi staining was diffused on the apical HC surface whereas β2-spectrin staining was not detectable (Figure 9A and A’). By the beginning of Phase II, when the DC was moving towards the periphery whereas the MC remained relatively closer to the center of the HC, Gαi staining was concentrated at the lateral side of the HC where the future hair bundle will be established (Figure 9B and B’). The DC being more laterally positioned than the MC was better associated with the Gαi domain than the MC (Figure 9B’). By this stage, β2-spectrin staining was also apparent, located in the medial side of the HC (Figure 9B and B’). This complementary expression patterns between Gαi and β2-spectrin became more strengthened and evident by the time centrioles reached late Phase II (Figure 9C and C’). Although blocking Gαi activity using pertussis toxin primarily affects hair bundle orientation in the lateral and not the medial utricle (Figure 9—figure supplement 1; Jiang et al., 2017), our centriole tracking and immunostaining results suggest that the polarity complex LGN/Insc/Gαi is established at the same time that centrioles started to migrate and these processes precede cuticular plate formation.

Figure 9 with 1 supplement see all

Download asset Open asset

Figure 9—source data 1

Coordinates of centriole positions during the 2 hr of live imaging.

https://cdn.elifesciences.org/articles/59282/elife-59282-fig9-data1-v2.xlsx

Download elife-59282-fig9-data1-v2.xlsx

Our live-imaging study is the first extensive time-lapse imaging of hair bundle acquisition in mammalian HCs. Imaging results of centriole migration in utricular HCs are consistent with a previous model extrapolated from results of SEM that the kinocilium starts out in the center of a HC before reaching its peripheral destination for hair bundle establishment (Dabdoub et al., 2003; Lu and Sipe, 2016; Denman-Johnson and Forge, 1999). Based on results in the chicken basilar papilla, it was proposed that the kinocilium undergoes fairly extensive migration along the periphery of the HC before reaching its final destination (Figure 1A; Cotanche and Corwin, 1991; Tilney et al., 1992). However, more recent studies in the mouse cochlea suggest that the MC/kinocilium takes a more direct route from the center of the HC to its final destination in the periphery (Dabdoub et al., 2003; Lu and Sipe, 2016; Denman-Johnson and Forge, 1999; Montcouquiol et al., 2003). Additionally, a similar time-lapse recording of embryonic cochlear explants of approximately 3 hr demonstrated a confined Brownian motion of centrioles in HCs (Lepelletier et al., 2013). By calculating the mean square distance of centriole movements in the utricular HCs as described (Lepelletier et al., 2013), it is likely that centrioles undergo Brownian motion in the utricular HCs but it is not clear whether centriole movements are as confined as in cochlear HCs. Nevertheless, our results are consistent with findings in the mouse that the MC/kinocilium and DC take a direct path to their destination in the periphery (Figure 10). Additionally, we found an intriguing centriole migration pattern for hair bundle establishment as discussed below.

Figure 10

Download asset Open asset

It has been proposed that the migration of kinocilium to its destinated location is achieved through an active force on centrioles via the microtubule network. This active force is suggested to be exerted through LGN/Insc/Gαi complex on microtubules by recruiting Lis1/dynein and/or shortening of microtubule (Ezan et al., 2013; Lu and Sipe, 2016; Tarchini and Lu, 2019). Disruption of the microtubule network caused the centrioles to promptly return to their initial central location rather than to remain stationary at the periphery of HCs. These results supported this active force hypothesis regardless of the mechanism involved, whether it is generated by pulling or shortening of the microtubules or both. Furthermore, our nocodazole results (Figure 7) as well as the anti-Gαi staining (Figure 9) indicate that the DC is likely to be under similar control of the LGN/Insc/Gαi complex as the MC. However, once the centrioles acquire their final position and cuticular plate starts to form, centriole positioning becomes less sensitive to microtubule disruption (Figures 8 and 9).

The directed migration of the centrioles depends on oriented microtubule arrangement of the minus ends at the centrioles and the plus ends at the periphery. This arrangement raises the possibility that proper anchoring of microtubules within HCs is an important factor. Among the anchoring proteins, we focused on ninein, which has both microtubule nucleation and anchoring functions (Delgehyr et al., 2005). It functions as a microtubule nucleation by docking γ-tubulin to the centrosomes and it also anchors microtubules in non-centrosomal site. For example, in pillar cells (supporting cells) of the cochlea, ninein has a non-centrosomal location in adherens junctions, which serve as microtubule anchors (Mogensen et al., 2000; Moss et al., 2007). Although ninein expression is dynamic and variable during the two phases of centriole migration, the broaden distribution of ninein when centrioles migrate towards periphery of the HC is clear and raises the possibility that ninein may function as microtubule anchors in addition to microtubule nucleation during this stage of centriole migration (Figures 6 and 10).

Many well described morphological and functional features distinguish between the MC and DC (Pelletier and Yamashita, 2012; Fujita et al., 2016). In addition to the function of DC maturing into an MC during the cell cycle, the function of the DC in differentiating cells is only beginning to be understood (Loukil et al., 2017; Betleja et al., 2018; Gottardo et al., 2015). Other than the DC being actively inhibited to form the cilium, recent results indicate that the proximity of the DC to the MC is also important for primary cilium formation (Loukil et al., 2017). Here, in nascent HCs, we show that when the MC was located at the center during Phase I, the DC was observed to move sporadically around the relatively stationary MC (Figures 2 and 10). This phenomenon has been described in several vertebrate somatic cell lines (Piel et al., 2000). In these cell lines, the MC, which is associated with a microtubule network is stationary, whereas the DC, although associated with the microtubule nucleation marker, γ-tubulin, is more mobile. The functional significance of the mobile DC, however, remains unclear except that this behavior is regulated by the cell cycle and attenuates as cells transition from G1 to S phase.

During Phase II of the centriole migration, the DC invariably moved ahead of the MC to reach the peripheral destination. This pattern of the DC preceding the MC in migration was observed repeatedly in HCs under all conditions investigated such as during normal centriole migration, recovery from nocodazole treatments, and ectopic Emx2 activation, suggesting that the migration of the DC is related to the MC. Although little is known about the relationships between the DC and MC in HCs, an inner ear conditional knockout of Kif3a, which encodes an intraflagellar transport protein, shows misplaced location and relationship between the MC and DC in cochlear HCs (Sipe and Lu, 2011).

Several scenarios could account for the observed behavior of the DC moving ahead of the MC in HCs. One possibility is that the two centrioles move independently of each other. Since the DC is similar to the MC in all parameters examined (association with the microtubule nucleation protein γ-tubulin and responses to microtubule disruption), each centriole can be independently transported by the microtubule-dynein system to their destinations in the peripheral cortex. The faster and higher mobility of the DC may simply be due to the MC being restricted by the attached cilium (Paintrand et al., 1992). An alternative scenario is that the MC is being dragged to the periphery by the DC via the intercentrosomal linkers between MC and DC, which are made of rootletin filaments (Yang et al., 2006). The sporadic movements of the DC around the MC in Phase I could also be regulated by the intercentrosomal linkers. In other systems, the length of these linkers can change and disintegrate based on maturation of the centrioles during the cell cycle (Bahmanyar et al., 2008; Mardin et al., 2010). However, little is known about the regulation and possible functions of these linkers in post-mitotic cells including HCs. Based on our findings, we speculate that the DC has an active role in guiding the MC/kinocilium to its proper location in differentiating HCs, in addition to its known role in regulating ciliogenesis.

In zebrafish lateral line, Emx2 regulates neuronal selectivity as well as hair bundle orientation (Ji et al., 2018). In the mouse utricle, onset of Emx2 expression is well ahead of the emergence of HCs (Figure 2—figure supplement 5). Therefore, Emx2 may have a role in regional patterning and/or HC fate specification that indirectly lead to hair bundle reversal. This notion is supported by our live-imaging results demonstrating that HCs are already pre-patterned by Emx2 prior to centriole movements (Figure 2). Nevertheless, our ectopic Emx2 experiments using AAV indicate that tdTomato signal was detectable within 36 hr of AAV-Emx2 infection (Figure 5). This time frame of sequential transcriptional and translational events to yield detectable tdTomato signal is comparable to other mammalian systems. Under the assumption that Emx2 is synthesized in a comparable time frame as tdTomato, hair bundle orientation reversal occurred relatively quickly within approximately 12 hr of detectable tdTomato (Figure 5). These results suggest that while Emx2 may have other functions in the utricle, its bundle reversal effect is likely to be direct and does not require multiple cascades of transcriptional and translational events. Additionally, both the genetic and AAV viral approaches indicate that during these early phases of centriole migration in hair bundle establishment, the system is plastic and responsive to Emx2 (Figures 3 and 5). However, the time-window of centrioles’ responsiveness to Emx2 is limited in vivo as ectopic activation of Emx2 after E15.5 only has a moderate effect on hair bundle reversal in naive HCs (Jiang et al., 2017). Taken together these in vivo results and the in vitro results here showing a lack of correlation between the level of Emx2 expression and change in hair bundle orientation of AAV-Emx2-tdT infected HCs (Figure 4), suggest that there is a critical time-window when HCs are responsive to Emx2 (Figure 10). Our results suggest that ectopic Emx2 is able to alter the course of centriole trajectory during centriole migration (Figures 3 and 5, Figure 3—figure supplement 2) but perhaps as cuticular plate starts to form with the accumulation of β2-spectrin, centrioles are hindered from relocation (Figure 9).

Furthermore, our results showed that the DC may have an active role in guiding the MC to its designated location in the HC periphery and a positive force is required to actively maintain this peripheral centriole positioning. These findings provided insights into the regulation of centriole dynamics during hair bundle establishment.

All animal experiments were conducted according to NIH guidelines and under the Animal Care Protocol of NIDCD/NIH (#1212–17). CAG:GFP-Centrin2 mice were obtained from Xiaowei Lu at University of Virginia (RRID:MGI:3793421), Atoh1-Cre mice from Bernd Fritzsch at University of Iowa (RRID:MGI:3775845), and Gfi1-Cre mice from Lin Gan at Augusta University (RRID:MGI:4430258; Yang et al., 2010). The Rosa26R^Emx2 mouse was generated by knocking in the cassette attb-pCA promoter-lox-stop-lox-Emx2-T2A-Gfp-WPRE-polyA-attb to the Rosa locus as described previously (Jiang et al., 2017). Rosa26R^tdTomato were purchased from Jackson laboratory (RRID:IMSR_JAX:007914, Madisen et al., 2010). Atoh1^Cre; Rosa^tdT/+ control specimens for live imaging was generated by crossing Atoh1^Cre; Rosa^tdT/tdT males with CAG:GFP-Centrin2^+/- females. Emx2 gain-of-function specimens was generated by crossing Atoh1^Cre; Rosa^tdT/tdT or Gfi1^Cre; Rosa^tdT/tdT males with CAG:GFP-Centrin2^+/-; Rosa^Emx2/Emx2 females. In addition to tdTomato signals, HC identity in the live-images was confirmed based on the round or oval shape of the apical cell surface and its more apical position of the nucleus within the epithelium relative to nuclei of the supporting cells.

The mouse utricle together with anterior and lateral cristae for orientation were dissected from E13.5 or E14.5 mouse inner ears. The harvested tissue was mounted on a Cell-Tak (Corning, NY, NY)-coated coverslip (Belyantseva, 2016) in culture medium containing DMEM/F12 (Thermo Fisher Scientific, Waltham, MA), 10% of fetal bovine serum (FBS, Thermo Fisher Scientific, Waltham, MA) and 50 U/ml penicillin G (Sigma-Aldrich, St Louis, MO), unless indicated otherwise. Live imaging was started after the explant had been incubated for 4 hr in a tissue culture incubator to ensure full attachment of the explant to the coverslip. The imaging was conducted in a chamber maintained at 37°C and 5% CO₂ on either an inverted PerkinElmer UltraVIEW Time Lapse Image Analysis System with a CMOS camera or a Nikon A1R HD confocal system on a Ni-E upright microscope with a GaAsP detector. For the UltraVIEW, a 10x objective was used for the lower magnification images and a 63x objective was used for time-lapse imaging (pixel size is 0.216 × 0.216 μm). For the Nikon A1R, a 25x objective was used for both the low- (pixel sizes are 0.48 × 0.48 μm) and high-magnification (pixel sizes 0.16 × 0.16 μm) time lapse recordings. In both microscopes, Z-stacks of 30–60 µm thickness with a 0.5 µm step were taken at each time frame per 10 min intervals. Live imaging was conducted up to 41 hr.

For microtubule inhibition experiments, we first determined the dose of nocodazole (Catalog# M1404, Sigma-Aldrich, St Louis, MO) to apply. Two doses of nocodazole, 5 μM and 33 μM, which were used in other cochlear explant studies (Szarama et al., 2012; Shi et al., 2005), were tested on E13.5 utricular explants for 24 hr. While explants treated with 5 μM nocodazole showed largely intact HCs with reduced tubulin signals in the cytoplasm, the utricular explants treated with 33 μM nocodazole showed reduced number of HCs, which looked unhealthy or apoptotic. Therefore, 5 μM of nocodazole was chosen for our live imaging studies. Nocodazole in DMEM/F12 with 10% FBS or culture media used for washing out the nocodazole was added to the utricular explant directly without disturbing the position of the explant under the microscope.

For the pertussis toxin experiments, we tested two dosages of pertussis toxin (Catalog# 516560–50 UG, Millipore Sigma, St Louis, MO), 2.1 and 8.4 nM, that were used for an in vivo inner ear study (Kakigi et al., 2019) and an in vitro outer HC study (Kakehata et al., 1993), respectively. Figure 9—figure supplement 1a shows the results of 8.4 nM pertussis toxin treatments, but the phenotypes observed were consistent between both dosages.

The AAV2.7m8-CAG-Emx2-P2A-tdTomato (2.2 × 10¹² genome copies/ml (GC/ml)) and AAV2.7m8-CAG-tdTomato (5.4 × 10¹² GC/ml) were synthesized by Vector Biolabs, Inc. The expression of Emx2 and tdTomato were driven by the CAG promoter. Four hr after an E13.5 utricular explant was established on a Cell-Tak coated coverslip in culture medium, the coverslip was transferred to a 24-well tissue culture plate filled with 100 µl of DMEM/F12 containing 2% of FBS and AAV in a final concentration of 4.0 × 10¹⁰ GC. One hour later, another 100 µl of medium without AAV was added to the culture. After an overnight incubation, the culture was washed several times before changing to regular medium that contained 10% FBS.

Dissected or live-imaged utricles attached on Cell-Tak coated coverslips were fixed with 4% paraformaldehyde in PBS at room temperature for 15 min. After fixation, the tissue attached to the coverslip was washed three times in PBS before blocking with PBS containing 5% donkey serum and 0.3% Triton-X for 45 min. For primary antibody, mouse anti-βII spectrin (1:500; BD Biosciences, San Jose, CA, Catalog# 612562, RRID:AB_399853), rabbit anti-Arl13b (1:500; Proteintech, Rosemont, IL, Catalog# 17711–1-AP, RRID:AB_2060867), mouse anti-acetylated tubulin (1:500; Sigma-Aldrich, St Louis, MO, Catalog# T7451, RRID:AB_609894), rabbit anti-ninein, (1:500; Abcam, Cambridge,UK, Catalog# Ab231181), rabbit anti-γ-tubulin (1:500; Sigma-Aldrich, St Louis, MO, Catalog# ab4447, RRID:AB_304460), rabbit anti-Emx2 (1:250; KO609, Trans Genic, Fukuoka, Japan), and rabbit anti-Gαi (1:1000; provided by B. Nurnberg) was used for overnight incubation at 4°C. Secondary antibodies of either Alexa Fluor 488/647 donkey anti-mouse IgG (Thermo Fisher Scientific, Waltham, MA, Catalog# A-21202 RRID:AB_2535788/Catalog# A-31571 RRID:AB_162542), Alexa Fluor 405 Donkey anti rabbit IgG (ab175651, Abcam, Cambridge, MA), or Alexa Fluor donkey anti-rabbit 647 (Thermo Fisher Scientific, Waltham, MA, Catalog# A-31573 RRID:AB_2536183) was used at 1:500 dilution for 15 min at room temperature. After extensive washing with PBS, samples were mounted in ProLong Gold Antifade (Thermo Fisher Scientific, Waltham, MA).

For experiments correlating live-imaged HCs followed by anti-β2-spectrin and anti-Gαi immunostaining, explants were fixed immediately after 2 hr of live imaging and processed for immunostaining. Then, the final frame of live imaging at low power was compared to the confocal image of the immunostained specimen. Based on the comparable distribution pattern of tdTomato-positive HCs between the two images, individual HCs tracked in the live imaging recording was identified and correlated with their immunostaining in the confocal images.

SiR-tubulin (Catalog# SC002, Spirochrome, Switzerland) was added to the live utricular samples attached on the coverslip to achieve a final concentration of 1 μM in the culture medium containing 10% FBS in DMEM/F12 and incubated for 10 hr before imaging. For imaging of γ-tubulin, acetylated-tubulin, and ninein staining as well as SiR-tubulin labeling, Airyscan imaging was conducted on a Zeiss LSM 780 with an Airyscan attachment (Carl Zeiss AG, Oberkochen, Germany) using a 63 × 1.4 NA oil objective lens. The acquired images were processed by Zeiss Zen Black software v2.1 for deconvolution.

In situ hybridization was conducted as described previously (Morsli et al., 1998). Digoxigenin-labeled RNA probes were synthesized for Sox2 (Evsen et al., 2013) and Emx2 (Simeone et al., 1992) as described.

To correct for sample drifting during imaging over time, the 3-D time-lapse image was processed using ImageJ (RRID:SCR_003070 Schneider et al., 2012) and the plugin of PoorMan3DReg (http://sybil.ece.ucsb.edu/pages/software.html) was used to re-align HCs to a stabilized x-y positions after semi-automatic adjustment of the z-positions using ImageJ macro, manual z-stack regulator (provided by Dr. Sho Ota). In some utricular images, GFP signals that overlapped with tdTomato signals in HCs were segmented and GFP signals without overlapping tdTomato signals were eliminated by using the ImageJ macro, Centrin-detector (provided by Dr. Sho Ota). The processed images were used for subsequent analyses. For tracking of centrioles and determination of the apical center of HCs, we performed spot and cell tracking algorithm using Imaris 9.5.0 (RRID:SCR_007370, Bitplane, Zurich, Switzerland) and these tracking data were used to generate the 3D reconstructed videos.

Three-dimensional reconstruction of the HC shape, total centriole trajectory relative to the center of the HC as well as temporal trajectory of selected time-frames of the recordings were generated by tracking data using Imaris. HC shape was determined based on tdTomato expression. For most summaries of selected time frames where the ending positions of the centrioles were drawn as circles such as Figure 2D#2, the HC contour of the last time frame was used. In selected time frames where the initial positions of the centrioles were shown as triangles such as Figure 2D#1, the HC contour at the beginning of the recording was used. In cases where the cell center was undefinable due to absence of tdTomato signal as in progenitors and supporting cells, or in young Lat HCs and AAV-infected Md HCs before clear detectable tdTomato expression, DC positions were plotted relative to the MC, which was used as a proxy for the center of the cell and thus no cell shape was drawn (Figure 2G#1, Figure 2—figure supplement 3B#1, Figure 2—figure supplement 4C–E, Figure 5C–D).

The entry of centriole movements into Phase II was determined retroactively when the DC is consistently moving toward the peripheral direction where hair bundles should be established. The x-y and z distance between centrioles were measured based on the coordinate of the tracking data. For the calculation of average x-y and z distances of centrioles in Lat HCs, only last 30 time-points before entering Phase II was used for computing the averages of Phase I Lat HCs, and earlier time-points possibly as progenitors were eliminated. The x-y migration speed was measured from the difference of coordinates of each centriole compared to the center of the HC per each 10 min time-frame, and the average speed of each centriole was calculated from all the time points after HC center could be determined based on tdTomato signals.

The tdTomato expression level of AAV-Emx2-tdTomato infected HCs was measured using ImageJ based on the relative fluorescent intensities of the tdTomato in HCs subtracted by signals from the surrounding background. To measure ninein fluorescence intensity associated with the centrioles, a line was drawn connecting the two centrioles and ninein signals associated with the centrioles (based on centrin-gfp signals) and in between the centrioles were measured along this line using ImageJ. For measuring the distribution of ninein during centriole migration, the ninein-positive region above threshold was outline and measured using Image J, and differences in ninein areas between Phases were analyzed by one-way ANOVA. Direction of DC trajectories in HCs ectopically expressing Emx2 using either Atoh1^cre or Gfi^cre was analyzed by Chi-square test and for other statistics, students t-test was used. P-values of less than 0.05, 0.01 and 0.001 are indicated by *, ** and ***, respectively.

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

We thank Dr. Sho Ota for writing the Fiji macro and providing helpful advice on live imaging data analyses, Kevin Isgrig and Dr. Wade Chen at NIDCD for advice on AAV2.7m8 virus and Dr. Elizabeth Driver at NIDCD for help with live imaging. We are also grateful to Drs. Brian Galletta, Matt Hannaford and Nasser Rusan at National Heart Lung and Blood Institute and Drs. Elizabeth Driver, Inna Belyantseva and Ronald Petralia at NIDCD, and members of the Wu Lab for their critical review of the manuscript. We also want to thank Michael Mulheisen for technical support in conducting the in situ hybridization experiments and Erina He at the NIH Medical Arts for drawing the illustrations.

Animal experimentation: All animal experiments were conducted according to NIH guidelines and under the approved Animal Care Protocol of NIDCD/NIH (#1212-17).

1. Received: May 28, 2020
2. Accepted: September 17, 2020
3. Accepted Manuscript published: September 23, 2020 (version 1)
4. Version of Record published: October 5, 2020 (version 2)

This is an open-access article, free of all copyright, and may be freely reproduced, distributed, transmitted, modified, built upon, or otherwise used by anyone for any lawful purpose. The work is made available under the Creative Commons CC0 public domain dedication.