During the prometaphase stage of mitosis, the cell builds a bipolar spindle of microtubules that mechanically segregates sister chromatids between two daughter cells in anaphase. The spindle assembly checkpoint (SAC) is a quality control mechanism that monitors proper attachment of microtubules to chromosome kinetochores during prometaphase. Segregation occurs only when each chromosome is bi-oriented with each kinetochore pair attached to microtubules emanating from opposite spindle poles. Overexpression of the protein kinase Aurora A is a feature of various cancers and is thought to enable tumour cells to bypass the SAC, leading to aneuploidy. Here, we took advantage of a chemical and chemical-genetic approach to specifically inhibit Aurora A kinase activity in late prometaphase. We observed that a loss of Aurora A activity directly affects SAC function, that Aurora A is essential for maintaining the checkpoint protein Mad2 on unattached kinetochores and that inhibition of Aurora A leads to loss of the SAC, even in the presence of nocodazole or Taxol. This is a new finding that should affect the way Aurora A inhibitors are used in cancer treatments.
Aurora kinases are key regulators of mitosis that fulfil complementary functions, as suggested by their localisation on mitotic structures; Aurora A localises at the centrosome and spindle poles, whereas Aurora B and Aurora C localise on chromosomes and at the midbody (Giet et al., 2005). Aurora B and Aurora C belong to the chromosome passenger complex (CPC) (Carmena et al., 2012b); their kinase activities are required for chromosome condensation through their phosphorylation of histones (Hsu et al., 2000; Wilkins et al., 2014), for the spindle assembly checkpoint (SAC) through their phosphorylation and regulation of Zwint-1 (Andrews et al., 2004; Kasuboski et al., 2011), for cytokinesis through their phosphorylation of the central spindlin component (Guse et al., 2005), and for the abscission checkpoint (Mathieu et al., 2013; Norden et al., 2006). Aurora A is involved in the G2/M transition (Dutertre et al., 2004; Seki et al., 2008), centrosome maturation (Hannak et al., 2001) and spindle assembly during prometaphase (Roghi et al., 1998). The SAC is a surveillance mechanism that monitors the attachment of kinetochores to microtubules during the process of bipolar spindle assembly (Rieder and Maiato, 2004). Every mitotic chromosome made of two sister chromatids possesses one kinetochore per chromatid. Once all of the chromosome kinetochores are attached to microtubules, the SAC is switched off, chromosome segregation occurs and the cell enters anaphase (Foley and Kapoor, 2013). The SAC components are localised at the kinetochores, a macromolecular structure organised through different layers of protein complexes. Starting at the level of the centromeric chromatin, the histone H3 variant centromere protein A (CENP-A) defines the localisation of the constitutive centromere-associated network (CCAN), which is composed of 16 CENPs. This complex provides a platform on which to build an interface between the kinetochore, the microtubules and the KMN network, which is made up of Knl1, Mis12 and Ndc80 (also known as Hec1).
At the molecular level, the SAC maintains the ubiquitin ligase anaphase-promoting complex/cyclosome (APC/C) in an inactive state through sequestration of its activator Cdc20 by the protein Mad2 (Nilsson et al., 2008). The mitotic checkpoint complex (MCC) responsible for the SAC signal in human cells is composed of the four proteins Mad2 (also known as MAD2L1 in mammals), BubR1, Bub3, Cdc20. Mad2 localises to unattached kinetochores and is released upon attachment by microtubules (Buffin et al., 2005; Chen et al., 1996). When all kinetochores are attached to microtubules, the inhibition of Cdc20 by Mad2 is relieved, allowing Cdc20 to bind to and activate the APC/C, which in turn ubiquitylates cyclin B and securin for their degradation by the proteasome. Without securin, the separase becomes active and cleaves the cohesin subunit Scc1 (also known as Rad21 and Mcd1), triggering sister chromatid separation (Uhlmann et al., 1999). APC/C also targets cyclin B1 for degradation, which induces the inhibition of CDK1 activity and allows the cell to exit mitosis (Thornton and Toczyski, 2003). BubR1 and Mad2 are present on unattached kinetochores and participate in SAC activity (Fang, 2002). Although the regulation of the SAC has been attributed to Aurora B rather than Aurora A, data suggest that Aurora A might also participate in SAC regulation. For example, phosphorylation of the centromere histone H3 variant CENP-A on serine 7 by Aurora A is required to localise Aurora B at the kinetochore (Kunitoku et al., 2003). CENP-A is considered as a platform on which to build the kinetochore where the mitotic checkpoint complex (MCC) is assembled. Unfortunately, inhibition of Aurora A kinase leads to defects in spindle assembly, which hinders any study of the role of the kinase in regulating the SAC (Hoar et al., 2007). To overcome this problem, we used two independent approaches that allow Aurora A inhibition in a timely and precise manner (analogue-sensitive inhibition and a specific inhibitor). By using the analogue-sensitive inhibition method, we have previously shown that the kinase activity of Aurora A is required for central spindle assembly through the phosphorylation of dynactin subunit p150Glued (also known as DCTN1) (Reboutier et al., 2013). Here, we report that, in the absence of Aurora A activity, cells exhibit defective chromosome congression, premature entry into anaphase and delocalisation of Mad2 from kinetochores to centrosomes, demonstrating for the first time that Aurora A activity is required to maintain an active SAC during prometaphase.
Aurora A inhibition causes premature exit from mitosis of cells arrested in prometaphase due to SAC activation
We previously developed an allele-sensitive Aurora A (as-Aurora A) where the activity can be inhibited by means of an ATP analogue (Reboutier et al., 2013), allowing specific inhibition of Aurora A in a very narrow window of time during cell cycle progression. We took advantage of this system to determine whether Aurora A activity plays a role in the SAC. We used a cell line expressing a GFP-tagged wild-type version of Aurora A (wt-Aurora A; cells denoted WT-U2OS) and another cell line expressing a GFP-tagged allele-sensitive Aurora A (AS-U2OS). Only as-Aurora A is sensitive to the ATP analogue 1-Na-PP1 (Reboutier et al., 2013). Importantly the ectopic kinase was expressed under the control of its own minimum promoter (Reboutier et al., 2013; Tanaka et al., 2002). We depleted the endogenous Aurora A via RNAi, controlled the efficiency of the depletion (Fig. 1A,B) and left the cells with ectopic Aurora A. The cells were then treated with the microtubule poison nocodazole at 100 nM for 13 h. This compound affects microtubule dynamics and arrests the cells in prometaphase of mitosis for several hours by maintaining an active SAC (Rieder and Maiato, 2004). To directly test whether Aurora A kinase activity was required in these cell cycle-arrested cells, the AS-U2OS and WT-U2OS cell lines were treated with 10 µM 1-Na-PP1 for 30 min in the presence of nocodazole and filmed for 3 h. In the presence of the inhibitor, only the WT-U2OS cells containing an active Aurora A kinase remain arrested in prometaphase, while the cells containing an inactive Aurora A kinase exited from mitosis as soon as we added the as-Aurora A inhibitor (Fig. 1A,C). To control that Aurora A inhibition did not stabilise kinetochore–microtubule attachments we repeated the experiment with 3.3 µM nocodazole, a concentration that not only maintains an active SAC but also depolymerises all mitotic microtubules (De Brabander et al., 1981; Jordan et al., 1992). We obtained the same result; namely, when treated with 3.3 µM nocodazole or with 3.3 µM nocodazole plus 10 µM 1-Na-PP1 the two cell lines AS-U2OS and WT-U2OS behave the same way, they arrest in prometaphase (Fig. 1D). When cells treated with nocodazole and 1-Na-PP1 were depleted of endogenous Aurora A, only cells expressing wt-Aurora A (insensitive to 1-Na-PP1) remained in mitosis, whereas cells expressing as-Aurora A (inhibited by 1-Na-PP1) exited mitosis in less than 1 h (Fig. 1C,D).
We also counted the number of mitotic cells for each cell line upon depletion of endogenous Aurora A and treatment with nocodazole and 1-Na-PP1. In the presence of nocodazole and 1-Na-PP1, the number of cells in mitosis was much higher (seven times higher) in cells expressing wt-Aurora A (78.29%, ±4.65, n=46) than in cells expressing as-Aurora A (9.41%, ±1.99, n=62) (Fig. 1E). 21.71% of the cells expressing active wt-Aurora A escape the nocodazole block and exit mitosis within 1 h, whereas the percentage of cells escaping the block reached 91.59% upon inhibition of Aurora A (Fig. 1E). Similar observations were made when cells were treated with taxol; 40% of cells escaped mitosis in the presence of active Aurora A, whereas 85% escaped mitosis in the absence of active Aurora A (data not shown).
These findings demonstrate that inhibition of Aurora A induces cells to exit mitosis in conditions where the SAC should prevent it.
Premature exit and abortive cytokinesis
To confirm and further characterise the observations above, we simplified the approach and used the Aurora A inhibitor MLN8237 at a concentration (50 nM) that affects only Aurora A and not Aurora B and C (Asteriti et al., 2014). We also decided to use a low concentration of nocodazole to avoid a complete depolymerisation of microtubules, but a concentration that remains sufficient to keep the SAC active (Wang and Burke, 1995). HeLa cells expressing tubulin–GFP were treated with 100 nM nocodazole for 10 h, released in prometaphase for 15 min, then incubated with 50 nM MLN8237, 20 nM nocodazole or both, and filmed (Fig. 2A).
As previously reported, Aurora A inhibition affected spindle morphology, in particular the spindle length (Bird and Hyman, 2008; Fig. 2B, compare green rows 1 and 2) but did not affect mitotic timing (Fig. 2C,D). A low dose of nocodazole (20 nM), however, drastically affected spindle formation (Fig. 2B, yellow line) and it maintained an active SAC, inducing a mitotic arrest (Fig. 2C,D). By adding MLN8237 on these mitotic arrested cells (20 nM nocodazole and 50 nM MLN8237), we confirm our above observation (Fig. 1); almost 75% of mitotic cells exited from mitosis (Fig. 2D) without having been able to assemble a proper bipolar spindle structure. Nonetheless, these cells that prematurely exit mitosis do not divide (Fig. 2B, red line). Instead, we observed a deformation of the cell cortex that might reveal an attempt by the cell to complete mitosis and to divide. Cytokinesis eventually aborted and the tetraploid cell re-adhered to the coverslip (Fig. 2B, red line).
Because these phenotypes were reminiscent of that Aurora B inhibition, we decided to control whether Aurora B could be affected during Aurora A inhibition. Cells were synchronised in prophase and released in the presence on MG132 (50 min, a proteasome inhibitor) to inhibit anaphase execution. Then cells were treated with DMSO, MLN8237, nocodazole, or both MLN8237 and nocodazole (Fig. 3A,B). In control cells, the Aurora B signal was detected in between CREST (a marker of centromeres) signals indicating that the kinase is localised in between kinetochore pairs, as previously reported (Figs 2B and 3C, line scans; Tanaka et al., 2002). We did not detect any overlapping area between Aurora A and Aurora B. Nor did we detect any modification of Aurora-B localisation under MLN8237 treatment (Fig. 3C, line scans) or using the as-Aurora A/1-Na-PP1 approach (data not shown).
To control the specificity of MLN8732 towards Aurora A kinase activity, we compared the auto-phosphorylation state of each of the Aurora kinases (Aurora A, B and C) in the absence or in the presence of 50 nM MLN8237 by means of western blotting with anti-phosphoserine antibodies (Fig. 3D). Aurora A auto-phosphorylation was almost completely lost under MLN8237 treatment, demonstrating that Aurora A was inactivated. In the same condition, we did not observe any change in Aurora B or C auto-phosphorylation. Additionally, the phosphorylation level of serine 10 on histone H3, an in vivo substrate of Aurora B and C was not affected by MLN8732 (Fig. 3D).
These data indicate that the conditions we used to inhibit Aurora A kinase does not affect Aurora B localisation or activity.
Inactivation of Aurora A disrupts the localisation of Mad2
To obtain molecular insight into the role of Aurora A in mitotic exit in the presence of abnormal spindle we investigated the behaviour of Mad2, one major MCC component that localises on unattached kinetochores during prometaphase and that signals the presence of an active SAC.
Using the as-Aurora A approach, we observed that without any treatment, 90% of the control cells had Mad2 at the kinetochores in prometaphase. In the presence of the as-Aurora A inhibitor 1-Na-PP1, 87% of cells expressing wt-Aurora A had Mad2 at the kinetochores, whereas only 10% of cells expressing as-Aurora A did (Fig. S1A,B). Western blot analysis revealed that Mad2 protein levels were not affected by Aurora A inhibition, indicating that the absence of the protein at the kinetochores was not due to a reduced amount of protein (Fig. 1B). Interestingly, in these last cells Mad2 was accumulating at the centrosomes (Fig. S1A) as revealed by a quantification of Mad2 signal at the kinetochore and centrosome (Fig. S1B).
We then used MLN8237 treatment to confirm these data by following the previously described experimental approaches (Fig. 3A). In the presence of MG132, the cells were treated with either 50 nM MLN8237 or 20 nM nocodazole or both, and images were acquired by super resolution microscopy (Zeiss Airyscan) to evaluate the localisation of Mad2 in late prometaphase (Fig. 4A). As previously reported by others (Bird and Hyman, 2008), inhibition of Aurora A led to shorter spindles, indicative of a good efficiency of MLN8237. By using super resolution images and quantitative analysis, the mean Mad2 intensity per kinetochore (stained with CREST) was calculated, pooled and compared. As expected, we observed a recruitment of Mad2 at kinetochores under nocodazole treatment (Fig. 4B). Interestingly, MLN8237 treatment reduces the Mad2 signal levels at the kinetochore in nocodazole-treated cells as well as in untreated cells (Fig. 4B). As observed in the as-Aurora A approach, this decrease of Mad2 at kinetochores is concomitant with a massive recruitment of Mad2 at centrosomes (Fig. 4A, red arrows, B,C).
This data indicates that Aurora A activity is required to maintain Mad2 on unattached kinetochores, thereby possibly contributing to maintain an active SAC.
Kinetochore localisation of Aurora A
Because we observed that Mad2 localisation at kinetochores is disrupted upon Aurora A inhibition, we investigated whether the Aurora A itself could be detected at or near the kinetochores. Although it is thought that Aurora A localises at the centrosome while Aurora B localises at the kinetochores during prometaphase, the presence of the Aurora A at kinetochores has been previously reported (Katayama et al., 2008). By using a super resolution approach, we investigated Aurora A localisation around kinetochores during the kinetochore–microtubule attachment process. As above, we used cells synchronised with nocodazole and blocked in metaphase by treatment with 50 nM of the proteasome inhibitor MG132 (Fig. 3A). We investigated the localisation of Mad2 and Aurora A along the axis of microtubules attached to kinetochores (Fig. 5A, c panels, red dotted lines). Microtubules were visualised by tubulin staining and kinetochores by CREST staining.
In control cells, we observed Aurora A signal following that of microtubules with a regularly decreasing intensity (reflecting protein levels) until reaching the kinetochore. Two kinetochores are shown in Fig. 5A in the first row. Mad2 is absent on the first kinetochore on the left but present in the one on the right signalling the presence of an active SAC (Fig. 5A, panel 1b). The drawing scheme representing the area occupied by the CREST signal (kinetochore) in purple and by Aurora A signal in red reveals an area occupied by both signals at the external surface of the kinetochore where the microtubules attach (Fig. 5A, panel 1e).
After MLN8237 treatment, as observed above, Mad2 was no longer found at kinetochores (Fig. 5A, panel 2b). Interestingly, MLN8237 treatment also affects Aurora A localisation, the kinase signal accumulated at kinetochores (Fig. 5A, panel 2d and 2e; Fig. 5B, second row). Nocodazole treatment at a low dose, on the other hand, induced a massive recruitment of Mad2 at kinetochores (Fig. 4A, panel 3b and 3e) but also a recruitment of Aurora A (Fig. 5A, panel 3d and 3e; Fig. 5B, third row).
In the presence of both nocodazole and MLN8237, only kinetochores still linked to microtubules showed Aurora A accumulation (Fig. 5A, panel 4c and 4d; Fig. 5B, fourth row), suggesting Aurora A accumulation at kinetochores relies on the presence of microtubules.
We tested this hypothesis by investigating the level of Aurora A signal at kinetochores by using the same methodology we used to quantify Mad2 (Fig. 3C). We observed an increase of Aurora A signal at kinetochores when cells were treated with either MLN8237 or nocodazole. This indicates that inhibiting Aurora A or maintaining an active checkpoint triggers Aurora A localisation at kinetochores. In cells treated with MLN8237 and nocodazole together, the level of Aurora A at the kinetochore further increased again (Fig. 5A, panel 4d and 4e; Fig. 5B, fourth row; Fig. 5C). These data strongly suggest that Aurora A uses microtubules to localise at kinetochores.
Until very recently, all of the studies describing the function of Aurora A have used loss of function by RNA interference, mutations in animal models, expression of a dominant-negative version of the kinase, or gain of function by overexpressing either a wild-type Aurora A or a mutated version that is hyperactive or non-degradable (Glover et al., 1995; Littlepage et al., 2002; Sasai et al., 2008; Schumacher et al., 1998; Zhou et al., 1998). Because Aurora A is essential for centrosome maturation, the phenotype observed in all of these cases corresponds to a defect in spindle assembly and the cell never reaches metaphase (Berdnik and Knoblich, 2002; Hannak et al., 2001). We investigated whether Aurora A is involved in the SAC by specifically inhibiting Aurora A activity after the centrosomes have matured and the cell reaches metaphase. We succeeded in this goal by taking advantage of the as-Aurora A isoform already described (Reboutier et al., 2013). In addition, we confirmed our results with the Aurora A-specific inhibitor MLN8237. Although Aurora A has never been directly involved in kinetochore functions, it phosphorylates CENP-A in prophase to allow Aurora B localisation at kinetochores (Kunitoku et al., 2003). Aurora A also phosphorylates Haspin in late G2, participating indirectly to the phosphorylation of threonine 3 of histone H3 and to the recruitment of Aurora B to kinetochores, and more directly to the localisation of CPC and SAC proteins at kinetochores (Yu et al., 2017). Aurora A was also recently reported to phosphorylate Ndc80 and to associate with the inner centromere Aurora B partner INCENP, when overexpressed, to localise at the mitotic chromosome kinetochore (DeLuca et al., 2018).
Eventually, Aurora A and Aurora B share substrates with phosphorylation events occurring where the kinases are located. Aurora A phosphorylates MCAK and PLK1 at the centrosome (Macůrek et al., 2008; Seki et al., 2008; Zhang et al., 2008), whereas Aurora B phosphorylates the same two proteins on the same residues but at the kinetochore (Andrews et al., 2004; Carmena et al., 2012a; Lan et al., 2004). Therefore, both Aurora A and Aurora B act in concert on the same substrates but at different locations to coordinate mitotic progression. This coordination was demonstrated further in DT40 cells in which Aurora A was depleted (knockout) and Aurora B inhibited. The authors found cooperation between both proteins in the coordination of chromosome segregation in metaphase and microtubule depolymerisation in anaphase (Hégarat et al., 2011).
In the present study and in contrast to what is seen upon Aurora A knockout, Aurora A was present and active until very late prometaphase. Its inhibition in that precise window of time led to a premature exit from mitosis with reduced Mad2 at kinetochores. In the presence of nocodazole or paclitaxel, which maintains an active SAC due to Mad2 recruitment at the kinetochores (Rieder and Maiato, 2004), inhibition of Aurora A led to the removal of Mad2 from the kinetochores, illustrating the loss of the checkpoint, and a relocalisation of Mad2 to the centrosomes. This indicates that Aurora A activity is required to maintain Mad2 at non-attached kinetochores during prometaphase, ensuring that the SAC remains active. Whether this is a direct or indirect effect of Aurora A remains unknown.
Consistent with such role of Aurora A, we also observed the inhibition of the kinase (MLN8237) led to its retention at kinetochores. Consistent with a recent report by DeLuca and collaborators (DeLuca et al., 2018) who identified Ndc80 as an Aurora A kinase substrate, we detected Aurora A at the outer kinetochores. This localisation of Aurora A seems to be very dynamic and the kinase might in fact shuttle at this localisation to phosphorylate substrates. Indeed, we observed that an inhibition of Aurora A increases its localisation to kinetochores as if the inactive kinase remained blocked on its substrate (Widmann et al., 2012). This localisation of Aurora A under MLN8237 sheds light on a possible cooperation between both Aurora A and B in regulating kinetochores bi-orientation leading to SAC silencing. Aurora A localises at the outer kinetochore while Aurora-B at the inner kinetochore (Fig. 6).
Aurora A has been observed at kinetochores where it participates in kinetochore or chromatin microtubule nucleation (Katayama et al., 2001). Consistent with a potential function in the SAC, overexpression of Aurora A has been shown to be sufficient to override the SAC in the presence of Taxol (Anand et al., 2003; Dutertre et al., 2004). Increased Taxol sensitivity was also observed in pancreatic cancer cell lines upon Aurora A depletion (Hata et al., 2005). More recently, it has been reported that the phosphorylation of p73 by Aurora A contributes to the breakdown of the Mad2–Cdc20 complex releasing Cdc20 to degrade cyclin B and securin, providing a molecular explanation for the SAC override (Katayama et al., 2012). Although resistance to Taxol treatment has been observed in breast cancer cells overexpressing Aurora A, this is only true in estrogen receptor (ER)-positive tumours and not in ER-negative tumours (Noguchi, 2006). The reason for this difference remains to be elucidated, but the phosphorylation by Aurora A of serine 167 and serine 305 in ERα might be involved (Zheng et al., 2014).
Reports have also indicated a bypass of the SAC upon Aurora inhibition, but the inhibitors used were not specific to one Aurora kinase and the bypass was eventually attributed to Aurora B inhibition. For example, the use of MLN8054, a more specific inhibitor of Aurora A than Aurora B, revealed that inhibition of Aurora A accelerates mitosis exit in the presence of nocodazole or taxol (Wysong et al., 2009). The concentration of MLN8054 used in the study was optimised for Aurora A inhibition, but the observed phenotype mimicked Aurora B inhibition (Tyler et al., 2007).
Here, we used two strategies to specifically inhibit Aurora A to clearly demonstrate for the first time that inhibition of Aurora A is sufficient to inhibit SAC activity and exit from mitosis. We demonstrated that the mechanism involved is not SAC override, but SAC inactivation. The molecular mechanism underlying the involvement of Aurora A in maintaining an active SAC during prometaphase remains to be elucidated, and a search for Aurora A substrates has begun. This report is the first to demonstrate a role of Aurora A kinase activity at the kinetochore to promote maintenance of the SAC. Aurora A is a major target in cancer therapy with several inhibitors currently in clinical trials (Kollareddy et al., 2012). A precise understanding of the multiple functions of Aurora A during mitosis will undoubtedly help in designing drug combinations and increase the efficiency of chemotherapeutic strategies to eliminate cancer cells (Bush et al., 2013; Schmidt et al., 2010).
MATERIALS AND METHODS
For analog-sensitive inhibition, three U20S cell lines were used: a normal U2OS cell line as control and two stable cell lines expressing a wild-type version of Aurora A tagged with GFP (wt-Aurora A) and an allele-sensitive version of Aurora A tagged with GFP (as-Aurora A). Both versions of Aurora A were expressed under the control of the Aurora A endogenous promoter (Reboutier et al., 2013). These cell lines were maintained in McCoy's 5A medium containing GluthaMAX (Gibco, Invitrogen) supplemented with 10% FBS (PAA) and 1% penicillin-streptomycin (Gibco, Invitrogen). In addition, the wt-Aurora A and as-Aurora A cells were grown in the presence of 1.25 mg/ml geneticin (G418 sulphate, PAA).
Hela tubulin–GFP and U2OS cells expressing Aurora A–GFP from its endogenous promotor were grown in a humidified incubator at 37°C and 5% CO2 in Dulbecco's modified Eagle medium (Gibco, Invitrogen) supplemented with 10% fetal calf serum (PAA Laboratories) and 1% penicillin-streptomycin (Gibco).
Small interfering RNA and transient transfections
The oligonucleotide sequence of the siRNA targeting Aurora A (Qiagen) was 5′-AAATGCCCTGTCTTACTGTCA-3′ (Reboutier et al., 2013). Transfection was performed using JetPRIME (Polyplus transfection). Depletion of endogenous Aurora A kinase was assessed by western blotting in every experiment, as described by Reboutier et al. (2013).
Cells were harvested by treatment with trypsin-EDTA (Gibco, Invitrogen) and resuspended in McCoy's 5A medium containing GluthaMAX, centrifuged at 161 g at 4°C for 3 min, and washed three times in PBS. The cell pellet was resuspended in Laemmli buffer, sonicated and incubated for 5 min at 95°C. Proteins in the cell extracts were separated on 12.5% SDS-PAGE gels and transferred onto a nitrocellulose membrane. After transfer, the membrane was blocked with 3% non-fat milk in TBST (Tris-buffered saline with Tween-20; 20 mM Tris-HCl, 150 mM NaCl, 0.05% Tween-20, pH 7.5) for 1 h at room temperature followed by an overnight incubation in TBST containing 3% non-fat milk and primary antibodies. The primary antibodies were mouse anti-Aurora A 5C3 (1:100; Cremet et al., 2003); rabbit anti-Mad2 (1:1000, cat. no. PRB-452C, Covance); rabbit anti-HCAP-D2 (1:10,000; Collas et al., 1999); mouse anti-Cyclin B1 (1:1000, cat. no. SC-245, Santa Cruz Biotechnology); mouse anti-HA (1/1000, cat. no. MMS -101R, Covance); mouse anti-β-tubulin (1:2000, cat. no. T8328, Sigma-Aldrich); rabbit anti phospho-Aurora A/B/C (1/1000, cat. no. 2914, Cell Signaling); rabbit antiphospho-histone H3 (H3S10) (1:1000, cat. no. PA5-17869, Thermo Fisher). The secondary antibodies were anti-mouse- or anti-rabbit-IgG coupled to peroxidase (1:5000 and 1:10,000, Jackson Laboratories). Finally, the membranes were processed for chemiluminescent enhancement with Dura or Pico (Thermo Fisher Scientific) before film exposure.
The cells were grown on coverslips in 12-well plates. Cells were then synchronised in late G2 (G2/M transition) by treatment with 100 nM nocodazole for 12 h at 37°C.
The cells were grown on coverslips in 12-well plates. They were depleted of endogenous Aurora A using siRNA as described by Reboutier et al. (2012). Cells were then synchronised in late G2 (G2/M transition) by treatment with 2 µM of the CDK1 inhibitor RO3306 (Calbiochem) at 37°C for 5 h. Next, they were released in late prometaphase by washing out RO3306 three times for 4 min. Finally, the cells were treated with 10 µM 1-Na-PP1 to inhibit as-Aurora A, fixed for 10 min at either −20°C in 100% cold methanol or at room temperature in 4% paraformaldehyde, and processed for immunofluorescence microscopy.
Cells were fixed in −20°C methanol for 5 min and then treated as described in Courthéoux et al. (2016). For the stable GFP cell line, GFP nano-booster (chromotek) was used at the secondary antibody incubation step. Images were taken with the new LSM800 Airyscan (Zeiss Inc.) and processed with FIJI (ImageJ). For Figs 3, 4 and 5, the Fast-Airyscan mode was used with optimum parameter settings. Lasers power and acquisition settings are the same for all conditions within an experiment. Enlarged pictures in Figs 3C and 5A are z-projections of five z-stacks.
Cells fixed in methanol or paraformaldehyde as described above were washed with PBST buffer (PBS containing 0.1% Triton X-100) and permeabilised by incubation in MBS buffer (100 mM PIPES pH 6.8, 1 mM MgCl2, 0.1 mM CaCl2 and 0.1% Triton X-100). The cells were then incubated in PBST containing 1% BSA for 1 h at room temperature, followed by 1 h incubation at room temperature in PBST containing 1% BSA and primary antibodies. After several washes in PBST containing 1% BSA, the cells were incubated with secondary antibodies. Images were taken using a Coolsnap ES (Photometrics) equipped Leica DMRXA2 microscope and image acquisition software MetaVue (Molecular Devices, Inc.). The images were deconvolved by use of the Metamorph software (Molecular Devices, Inc.) and edited using Adobe Photoshop CS3.
Antibodies used were as follows: mouse anti-α-tubulin B-5-1-2 (1:2000, cat. no. T5168, Sigma); rat anti-β-tubulin (YL1/2 PRB-452C, 1:500, cat. no. MAB1864, Millipore), rabbit anti-Mad2 (1:500, cat. no. 15-234-0001, Covance), human anti-CREST centromere protein (1:3000, cat. no. 611083, Antibodies Incorporated); mouse anti-Aurora B (1:1000, cat. no. CF405s, BD) antibodies. Secondary antibodies were: rabbit and mouse CF™ (1:1000, cat. no. 20082 and 20380, Biotium). Alexa Fluor 488-conjugated donkey anti-rat IgG (1:1000), Alexa Fluor 555-conjugated donkey anti-mouse IgG (1:1000), or Alexa Fluor 555-conjugated goat anti-rabbit IgG (1:1000) (Invitrogen). Finally, samples were mounted with Vectashield or Vectashield-DAPI (1:1000, Vector Laboratories) for DNA staining.
Quantification of fluorescence signals
For the quantitative analysis in Figs 3C and 4C of Aurora A and Mad2 intensities at kinetochore, kinetochore volume was isolated by using the ‘3D object counter’ from FIJI on thresholded CREST z-stack images. Kinetochore volumes were imported by means of the ‘3D ROI manager’. The average intensities per kinetochore were collected and normalised to the maximum mean from the nocodazole (for Mad2) or MLN8237 condition (respectively showing the highest Mad2 or Aurora A mean intensity per kinetochore). Aurora A and Mad2 kinetochore values were pooled per condition and shown as box plots.
The integrated densities of Mad2 (equatorial plates and bipolar spindle poles) were determined from deconvolved images taken with the Leica DMRXA2 (63× objective) using the FIJI (ImageJ) 1.46i software (NIH).
HeLa cell lines expressing tubulin–GFP (Reboutier et al., 2013) was grown on Zeiss High resolution coverslips for 24 h then synchronised as described in Fig. 1A. Video microscopy was performed with a Spinning disk CSU-X1 set up on a Nikon Ti-E system. Seven z-stack (3 µm step) were collected every 3 min using the 63× magnification objective. Z-stacks were z-projected and movies were analysed using FIJI software. Anaphase was detected manually (Hours:minutes at 00:30 in control condition Fig. 2B). Timing was collected for experiments, pooled and presented as box plot (Fig. 2C).
Endogenous Aurora A was depleted from both stable U2OS cell lines expressing wt-Aurora A and as-Aurora A by using siRNA as described in Reboutier et al. (2013). The cells were then incubated in 100 ng/ml (0.2 µM) nocodazole or 5 µM Taxol until the end of the time lapse (16 h). After 13 h incubation in nocodazole, the cells were treated with 10 µM 1-Na-PP1 and filmed for 3 h. The addition of 1-Na-PP1 marks T0 for each movie. Video microscopy was performed on a Leica DM IRB microscope equipped with a 63×/1.4 NA oil-objective and a Coolsnap HQ camera (Photometrics) driven by Metamorph software (Molecular Devices, Inc.). Images were acquired every 5 min and analysed using the same software.
All experiments have been performed at least three independent times, and t-tests on the mean were performed using Igor (Wavemetrics). Where used, a Tukey's honestly significant difference (HSD) test was conducted in R 2.13.0 software (R Core Group). Values are represented as histograms or box plots.
Thibault Courtheoux was a fellow of the Region Bretagne and FHU CAMIn. Alghassimou Diallo was a fellow of the Guinée government; some data in the paper forms part of his PhD thesis prepared in the Institute of Genetics and Development of Rennes and defended at the University of Rennes 1 in December 18th, 2013. We thank the MRic facility (Microscopy Rennes Imaging Center, Biosit, IBISA), Stéphanie Dutertre (Biosit), and Jacques Pécreaux for helpful advice on integrated density.
Conceptualization: T.C., A.D., C.P.; Methodology: T.C., A.D., A.P.D., D.R., E.W., C.P.; Investigation: T.C., A.D., A.P.D., E.W., C.P.; Writing - original draft: T.C., C.P.; Writing - review & editing: T.C., E.W., C.P.; Supervision: E.W., C.P.; Project administration: C.P.; Funding acquisition: C.P.
This work was supported by the Centre National de la Recherche Scientifique, Université de Rennes 1, Institut National du Cancer, Ligue Contre le Cancer (Equipe Labelisée 2014), and Agence Nationale de la Recherche (Aurora).
The authors declare no competing or financial interests.