Abstract
In eukaryotic cell division, the Spindle Assembly Checkpoint (SAC) plays a key regulatory role by monitoring the status of chromosome-microtubule attachments and allowing chromosome segregation only after all chromosomes are properly attached to spindle microtubules. While the identities of SAC components have been known, in some cases, for over two decades, the molecular mechanisms of the SAC have remained mostly mysterious until very recently. In the past few years, advances in biochemical reconstitution, structural biology, and bioinformatics have fueled an explosion in the molecular understanding of the SAC. This chapter seeks to synthesize these recent advances and place them in a biological context, in order to explain the mechanisms of SAC activation and silencing at a molecular level.
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Keywords
- Spindle Assembly Checkpoint (SAC)
- Microtubule Attachment
- Anaphase-Promoting Complex/Cyclosome (APC/C)
- Comet 67P
- Mitotic Checkpoint Complex (MCC)
These keywords were added by machine and not by the authors. This process is experimental and the keywords may be updated as the learning algorithm improves.
1 Introduction
A critical decision point in the life of a eukaryotic cell is the mitotic metaphase-to-anaphase transition, when replicated chromosomes are segregated to opposite spindle poles prior to cell division. Before committing to anaphase, the cell must ensure that all chromosomes are attached to spindle microtubules, and that sister chromosomes (or homologs, in meiosis I) are bi-oriented; that is, attached to microtubules extending from opposite spindle poles. Failure to properly sense and respond to errors in microtubule attachment can lead to aneuploidy, a hallmark of cancer and (when it occurs in meiosis) a major cause of miscarriage and developmental disorders like Down Syndrome.
The metaphase-to-anaphase transition is controlled by the activity of a ubiquitin E3 ligase, the Anaphase-Promoting Complex/Cyclosome (APC/C) (Sudakin et al. 1995; King et al. 1995), which ubiquitinates and promotes the degradation of a number of substrates, most notably B-type cyclins and securin (Murray et al. 1989; Glotzer et al. 1991; Cohen-Fix et al. 1996; Morgan 1997; Shirayama et al. 1999). Securin is an inhibitor of a protease, separase, that when activated cleaves the Scc1 subunit of the cohesin complexes holding bi-oriented sister chromosomes together; this cleavage is the critical step initiating chromosome segregation in anaphase (Ciosk et al. 1998; Kamenz and Hauf 2016).
Prior to anaphase onset, the activity of the APC/C is inhibited by the spindle assembly checkpoint (SAC), which monitors the state of chromosome-microtubule attachment in the cell (reviewed in Musacchio and Salmon 2007; Lara-Gonzalez et al. 2012; Musacchio 2015; Zhang et al. 2016b; Etemad and Kops 2016). Microtubule attachment is mediated by kinetochores, complex protein assemblies with both DNA-binding and microtubule-binding subunits (reviewed in Pesenti et al. 2016; Nagpal and Fukagawa 2016). When kinetochores are not properly attached to microtubules, they mediate assembly of a soluble “wait anaphase” signal in the form of the four-protein Mitotic Checkpoint Complex (MCC), which directly binds and inhibits the APC/C. In this manner, a single unattached kinetochore is in most cases able to delay anaphase onset (Rieder et al. 1995).
Seminal work published in 1991 initiated study of the SAC by isolating the first mutants defective in this pathway, termed mad (mitotic arrest deficient) (Li and Murray 1991) and bub (budding uninhibited by benzimidazole) (Hoyt et al. 1991). Only now, however, are the detailed molecular mechanisms of SAC activation and silencing coming into sharp focus, thanks to a recent surge in structural and biochemical studies of the APC/C, its interactions with the MCC, and the mechanisms of MCC assembly and disassembly. This review covers several aspects of SAC function that have recently seen significant advances, beginning with the structure and function of the APC/C itself, and the mechanism of its inhibition by the MCC. I then move to the sites of MCC assembly—kinetochores—and outline the mechanisms of chromosome-microtubule attachment sensing and MCC assembly at unattached kinetochores. Finally, I address how the SAC is silenced after kinetochore-microtubule attachment, paying particular attention to a newly discovered pathway for direct MCC disassembly. Throughout, I attempt to place recent structural and biochemical work into the larger framework of SAC function that has been refined, through the work of many, over the 25 years since the discovery of this pathway.
2 The APC/C: Target of the Spindle Assembly Checkpoint
As the master regulator of anaphase onset, the mechanisms of the APC/C, particularly how it is regulated through the cell cycle and how it recognizes substrates, are of considerable interest. Because of its immense size and complexity, these questions were unanswerable until recent advances in cryo-electron microscopy (cryo-EM) began to provide high-resolution pictures of the APC/C in a variety of functional states (Chang et al. 2014, 2015; Brown et al. 2015, 2016; Zhang et al. 2016c; Yamaguchi et al. 2016; Alfieri et al. 2016). This structural work, coupled with in vitro and in vivo functional analysis, has significantly improved our understanding of APC/C substrate recognition, the role of “coactivator” proteins such as Cdc20 in that recognition, and how the APC/C is inhibited by the MCC. In particular, the previously enigmatic roles of Cdc20, a key APC/C coactivator that also acts as an inhibitor when incorporated into the MCC, have been significantly clarified.
2.1 Overall APC/C Architecture
The APC/C is a 19-subunit complex (20 when counting a bound coactivator; see below) with a total molecular weight of ~1.2 MDa (Fig. 1a) (Sudakin et al. 1995; King et al. 1995; Chang et al. 2014). It contains two E3 ubiquitin ligase subunits: Apc2 is related to the Cullin subunits of SCF ubiquitin ligases, while Apc11 contains a RING-type E3 ligase domain. These subunits bind several different E2 activating enzymes to mediate substrate ubiquitination, with different E2s responsible for ubiquitin chain initiation and elongation. The bulk of the APC/C forms two large structures, the so-called TPR lobe (or “arc lamp”) named for the tetratricopeptide (TPR) repeats found in this lobe’s subunits, and the platform. Together, the TPR lobe and platform define a large central cavity and serve to juxtapose functional modules responsible for substrate recognition with those responsible for ubiquitination (Fig. 1a). For a detailed discussion of APC/C architecture, the reader is referred to recent reviews on the subject (Primorac and Musacchio 2013; Chang and Barford 2014; Barford 2015).
2.2 APC/C Substrate Recognition Is Mediated by Coactivator Proteins
In order to recognize its substrates, the APC/C requires one of a family of “coactivator” proteins, which bind the APC/C in a cell cycle-regulated manner and dictate substrate specificity by binding directly to conserved “degron” motifs in those substrates. All APC/C coactivators are structurally related, with a central WD40 β-propeller domain responsible for degron recognition, and conserved motifs at the N- and C-terminus that mediate docking between the APC/C’s TPR lobe and platform (Figs. 1a and 2b) (Zhang and Lees 2001; Schwab et al. 2001; Vodermaier et al. 2003; Thornton et al. 2006; Matyskiela and Morgan 2009; Izawa and Pines 2012; Chang et al. 2015; Zhang et al. 2016c). While detailed discussion is outside the scope of this review, binding of the different coactivator proteins to the APC/C is regulated through phosphorylation of both the coactivators themselves (Zachariae et al. 1998; Jaspersen et al. 1999; Lukas et al. 1999; Kramer et al. 2000; Labit et al. 2012; Chang et al. 2015) and subunits of the APC/C (Lahav-Baratz et al. 1995; Shteinberg et al. 1999; Kramer et al. 2000; Golan et al. 2002; Kraft et al. 2003; Zhang et al. 2016c; Qiao et al. 2016). The end result of this regulation is that the bound coactivator, and therefore the APC/C’s substrate specificity, depends on cell-cycle stage: Cdh1 is bound during interphase, and Cdc20 is bound in mitosis. Here, I focus entirely on the APC/C-Cdc20 complex, which controls anaphase onset and constitutes the target of the SAC.
When bound to the APC/C as a coactivator, Cdc20 recognizes several different degron motifs via distinct surfaces on its central WD40 β-propeller domain (Figs. 1b, 2b and 3a) (reviewed in Davey and Morgan 2016). Recognition of one such motif, the destruction box (D-box) (Glotzer et al. 1991), is bipartite: this motif becomes sandwiched between Cdc20 and an adjacent APC/C subunit, Apc10 (Fig. 1b) (Buschhorn et al. 2011; da Fonseca et al. 2011; Chang et al. 2014). Recognition of the two other known degron motifs—the KEN box (named for its sequence: lysine-glutamate-asparagine) (Pfleger and Kirschner 2000) and ABBA motif (also termed A-motif, Phe-box, or IC20BD) (Burton et al. 2011; He et al. 2013; Lischetti et al. 2014; Diaz-Martinez et al. 2015; Di Fiore et al. 2015)—is mediated solely by Cdc20 (Fig. 3a). Together, binding of one or more degrons by the APC/C-Cdc20 complex positions a substrate for ubiquitination by the catalytic module (Chang et al. 2014; Brown et al. 2015).
3 The Mitotic Checkpoint Complex Inhibits APC/C-Cdc20
The key element of SAC signaling is the four-protein MCC, which is generated at unattached kinetochores and directly binds and inhibits the APC/C-Cdc20 complex. The conserved “core” MCC comprises Mad2, Cdc20, and BubR1 (Mad3 in fungi), with BubR1 forming a constitutive dimer with Bub3 in a subset of organisms including humans. Cdc20’s role as an APC/C coactivator is outlined above; for many years, how Cdc20 also functions as an APC/C inhibitor was unknown. Recent structural work on both the isolated MCC and its complex with the APC/C have clarified this question, resulting in a simple, yet elegant, model for APC/C inhibition by the MCC and for the dual roles of Cdc20.
3.1 Mitotic Checkpoint Complex Architecture
Mad2 was the first protein demonstrated to bind and inhibit the APC/C (Li et al. 1997). Mad2 contains a HORMA domain (Aravind and Koonin 1998) that can adopt two different conformations: an inactive “open” conformation (O-Mad2), and a “closed” conformation (C-Mad2) that binds short peptide motifs called Mad2-interacting motifs (MIMs) or, more generally, closure motifs (Fig. 2a) (reviewed in Mapelli and Musacchio 2007; Luo and Yu 2008). These two conformations differ in the structure of the C-terminal region of the protein, termed the “safety belt”: in C-Mad2, this segment wraps entirely around a bound closure motif to form a topologically linked complex (Luo et al. 2002). In O-Mad2, the safety belt is docked against the closure motif binding site (Luo et al. 2000), and the protein is therefore unable to bind a closure motif. The bulk of soluble Mad2 in the cell is in the O-Mad2 state (Luo et al. 2004); the rate-limiting step of MCC assembly is the recruitment of O-Mad2 to unattached kinetochores, where it is converted to C-Mad2 and associates with a closure motif in Cdc20, termed the KILR motif (Fig. 2b) (Hwang et al. 1998; Kim et al. 1998; Fang et al. 1998; Kallio et al. 1998; Luo et al. 2002).
BubR1 is the third member of the so-called “core” MCC (Hardwick et al. 2000; Tang et al. 2001; Sudakin et al. 2001; Fang 2002), and directly interacts with both Mad2 and Cdc20, significantly stabilizing the overall complex (Figs. 2c and 3a) (Sczaniecka et al. 2008; Tipton et al. 2011; Chao et al. 2012; Faesen et al. 2017). BubR1, which arose along with its paralog Bub1 from a gene duplication event (Suijkerbuijk et al. 2012a; Vleugel et al. 2012; Di Fiore et al. 2016), has a complex domain structure featuring at least seven degron-like motifs: the N-terminal TPR-repeat domain contains a KEN box, and this domain is followed by a second KEN box, two D-boxes, and three ABBA motifs (Fig. 2c). In the core MCC, BubR1 binds Cdc20 through its N-terminal KEN box (KEN1) and the adjacent TPR-repeat domain (Sczaniecka et al. 2008; Chao et al. 2012), and also through one of its ABBA motifs (most likely ABBA2; Di Fiore et al. 2016). The TPR domain also binds MAD2, completing the cooperative assembly of the highly stable core MCC (Fig. 3a).
3.2 APC/C-Cdc20 Binding and Inhibition by MCC
The fully assembled MCC contains a copy of BubR1 with a series of degron motifs—D1, ABBA1, and KEN2—unoccupied (Fig. 3c). The presence of these degrons, and their importance for APC/C-Cdc20 inhibition by the MCC, led to a proposal that BubR1 could bind two copies of Cdc20, one as part of the MCC (termed Cdc20MCC) and a second bound to the APC/C as a coactivator (termed Cdc20APC/C) (Primorac and Musacchio 2013). An important biochemical and cryo-EM analysis of APC/C-Cdc20 and APC/C-MCC complexes purified from HeLa cells provided early evidence that this might be the case, as the stoichiometry of Cdc20 was doubled in APC/C-MCC versus APC/C-Cdc20 (Herzog et al. 2009). The relatively low resolution (by today’s standards) of that study’s EM analysis, however, prevented a clear visualization of the two copies of Cdc20 in APC/C-MCC. More recently, it was shown biochemically that the fully assembled MCC could bind a second copy of Cdc20 that was already bound to the APC/C, and that this binding was disrupted by mutating BubR1’s D1 degron motif (Izawa and Pines 2014). More recent high-resolution structures of the APC/C-MCC complex have clearly shown the positions of two copies of Cdc20 in this complex, confirming the above findings (Fig. 3b) (Yamaguchi et al. 2016; Alfieri et al. 2016). These structures, plus detailed biochemical and genetic analysis with BubR1 mutants, also finally reveal the roles of BubR1’s many degron-like motifs: in the APC/C-MCC complex, BubR1 winds between Cdc20MCC and Cdc20APC/C, occupying all degron-binding sites of both copies (Fig. 3c) (Alfieri et al. 2016; Di Fiore et al. 2016). BubR1 binds Cdc20MCC through its KEN1 motif and TPR domain as described above, and also through its ABBA2 motif (Figs. 2c and 3c) (Diaz-Martinez et al. 2015; Alfieri et al. 2016; Di Fiore et al. 2016). Between these motifs, BubR1 wraps around the WD40 domain of Cdc20APC/C, binding through its D1, ABBA1, and KEN2 motifs (Fig. 3c) and also causing a significant rotation of Cdc20APC/C that disrupts the bipartite D-box recognition site (Alfieri et al. 2016). APC/C-bound MCC also sterically occludes the binding of E2 enzymes to the APC/C catalytic module, further inhibiting activity (Yamaguchi et al. 2016; Alfieri et al. 2016). Thus, MCC targets already-assembled APC/C-Cdc20 for inhibition, binding through a series of degron motifs in BubR1. Because Cdc20APC/C remains bound to the APC/C in this complex, reactivation of the APC/C upon SAC silencing requires only removal or disassembly of the bound MCC (see Sect. 5 and Fig. 4).
4 Assembly of the Mitotic Checkpoint Complex at Unattached Kinetochores
The key molecular event monitored by the SAC is kinetochore-microtubule attachment. Kinetochores are complex multi-megadalton structures that assemble on each chromosome’s centromere, where they both mediate chromosome-microtubule attachment and serve as signaling hubs for the checkpoints monitoring attachment status. The architecture and function of kinetochores are covered in recent excellent reviews (Pesenti et al. 2016; Nagpal and Fukagawa 2016); here I focus mainly on a conserved outer kinetochore complex, the KMN network, that serves as the major sensor of microtubule attachment and a scaffold for MCC assembly.
4.1 The KMN Network: A Scaffold for SAC Signaling and MCC Assembly
The KMN network is a highly conserved outer kinetochore complex that serves as both the main microtubule-binding component of the kinetochore, and a platform for MCC assembly when microtubules are not bound (Fig. 5a) (Cheeseman et al. 2006; Varma and Salmon 2012). The KMN network contains three subcomplexes with distinct roles: the Mis12 complex anchors the network to the inner kinetochore, the Ndc80 complex binds microtubules, and the Knl1 complex is responsible for recruiting SAC proteins.
Knl1 (Spc105 in Saccharomyces cerevisiae, Spc7 in Schizosaccharomyces pombe, Knl1/CASC5/Blinkin in humans) contains a large disordered N-terminal region with multiple conserved motifs. Nearest the N-terminus is a phosphatase-binding site, termed SILK/RVSF (Hendrickx et al. 2009; Liu et al. 2010). When kinetochores are not attached to microtubules, phosphatase binding is inhibited through phosphorylation of this site by the Aurora B kinase (Liu et al. 2010). Following the SILK/RVSF motif in Knl1 are multiple short motifs, termed MELT repeats (Desai et al. 2003; Nekrasov et al. 2003; Cheeseman et al. 2004; Vleugel et al. 2015b), that are phosphorylated by the Mps1 kinase when kinetochores are not attached to microtubules (London et al. 2012; Shepperd et al. 2012; Yamagishi et al. 2012). Phosphorylated MELT repeats (P-MELT) recruit the SAC protein Bub3 along with its binding partners, Bub1 and BubR1 (Yamagishi et al. 2012; Primorac et al. 2013; Vleugel et al. 2013, 2015b; Krenn et al. 2014; Zhang et al. 2014; Overlack et al. 2015). As mentioned above, Bub1 and BubR1 are paralogs with similar overall structures, but each has evolved to fulfill distinct roles in the checkpoint: Bub1 serves as the major hub for MCC assembly by recruiting SAC proteins, and BubR1 is a subunit of the MCC (Bub1 and BubR1’s evolution from a bifunctional ancestor is discussed more fully in Suijkerbuijk et al. 2012a; Di Fiore et al. 2016). Both Bub1 and BubR1 bind Bub3 through their so-called GLEBS motifs (Taylor et al. 1998; Wang et al. 2001; Larsen et al. 2007), and the resulting complex is competent to bind Knl1 P-MELT repeats (Fig. 5b). Interestingly, Bub1:Bub3 binds much more strongly to P-MELT repeats than does BubR1:Bub3 (Primorac et al. 2013; Overlack et al. 2015), and the bulk of BubR1:Bub3 is recruited to kinetochores indirectly, through a pseudo-symmetric Bub1-BubR1 dimer interaction (Overlack et al. 2015; Zhang et al. 2015). Some BubR1:Bub3 is recruited directly to Knl1 P-MELT repeats, however, and preliminary evidence suggests that this pool may be the major source of BubR1:Bub3 that is incorporated into the MCC (see Sect. 4.3) (Zhang et al. 2016a). The requirement for BubR1 localization to kinetochores varies between organisms, however, as some BubR1 orthologs—such as S. pombe Mad3—lack both Bub3 and Bub1 binding motifs (Fig. 2c).
Once recruited to Knl1 P-MELT motifs, Bub1 and BubR1 recruit the remaining SAC components necessary for MCC assembly: Cdc20 and a complex of Mad1 bound to C-Mad2. Cdc20 is recruited by both Bub1 and BubR1, through homologous degron-like motifs C-terminal to these proteins’ GLEBS motifs (BubR1 ABBA3 (Lischetti et al. 2014; Di Fiore et al. 2015), Bub1 KEN-ABBA (Vleugel et al. 2015a)). Mad1:Mad2 is also probably recruited by Bub1, with direct interactions between Mad1 and Bub1 having been reported in multiple organisms including fungi, nematodes, and humans (London and Biggins 2014; Moyle et al. 2014; Ji et al. 2017). Humans and other complex eukaryotes also possess a separate complex, known as RZZ (Rod-Zwilch-ZW10) that binds Bub1 and recruits Mad1:Mad2 (Wang et al. 2004; Kops et al. 2005; Buffin et al. 2005; Karess 2005; Barisic and Geley 2011; Zhang et al. 2015; Caldas et al. 2015; Silió et al. 2015). Regardless of its recruitment pathway, kinetochore-localized Mad1:Mad2 is necessary to recruit soluble O-Mad2 and mediate its conversion to C-Mad2, binding to the Cdc20 KILR motif, and assembly into the MCC (see Sect. 4.3).
4.2 The Mps1 Kinase Coordinates Attachment Sensing with MCC Assembly
As noted above, the kinase Mps1 phosphorylates Knl1 MELT repeats to initiate recruitment of SAC components to unattached kinetochores (the diverse roles of Mps1 are reviewed in Lan and Cleveland 2010; Liu and Winey 2012). Mps1 recruitment, therefore, must be responsive to kinetochore-microtubule attachment status. It is not surprising, therefore, that the key determinant of Mps1 recruitment is the Ndc80 complex, the major kinetochore complex responsible for microtubule binding (Martin-Lluesma et al. 2002; Nijenhuis et al. 2013; Zhu et al. 2013; Hiruma et al. 2015; Ji et al. 2015; Aravamudhan et al. 2015; Dou et al. 2015). Exactly how Mps1 kinase activity is coordinated with Ndc80-microtubule binding is not yet firmly established. One mechanistic model involves a direct competition between Mps1 and microtubules for Ndc80 binding. Supporting this idea, two groups recently showed that Mps1 binds directly to the Ndc80 CH domain, which is also responsible for microtubule binding (Wei et al. 2007; Ciferri et al. 2008; Hiruma et al. 2015; Ji et al. 2015). These studies showed that Mps1-Ndc80 binding is suppressed in vitro by microtubules, suggesting that Mps1 and microtubules compete directly for Ndc80 binding (Hiruma et al. 2015; Ji et al. 2015). Another possible mechanism is that Mps1 remains associated with Ndc80 even after microtubule attachment, but its ability to phosphorylate Knl1 is inhibited once attachment occurs (Aravamudhan et al. 2015). In either case, active Mps1 promotes MCC assembly at unattached kinetochores in several ways. First and most importantly, it phosphorylates the MELT repeats in the N-terminal region of Knl1 (London et al. 2012; Shepperd et al. 2012; Yamagishi et al. 2012), which in turn recruit Bub1:Bub3 as described above. Mps1 also phosphorylates Bub1 directly, and this phosphorylation was recently shown to be required for Bub1’s ability to recruit Mad1:Mad2 to kinetochores (London and Biggins 2014; Ji et al. 2017). Finally, Mps1 phosphorylates Mad1 in its poorly characterized C-terminal RWD domain, promoting a direct Mad1-Cdc20 interaction that contributes to MCC assembly and SAC signaling (Hardwick et al. 1996; Faesen et al. 2017; Ji et al. 2017).
4.3 Assembling the MCC
Once all SAC components are recruited to unattached kinetochores, they participate in a complex structural dance, still incompletely understood, that ultimately results in fully assembled MCC. The first, and rate-limiting, step of MCC assembly is the association of Mad2 with Cdc20 (Simonetta et al. 2009; Faesen et al. 2017). This occurs when kinetochore-localized Mad1:Mad2 recruits soluble O-Mad2 to kinetochores through a pseudo-symmetric Mad2 homodimer interaction (Fig. 6) (Luo et al. 2004; Howell et al. 2004; Shah et al. 2004; de Antoni et al. 2005; Vink et al. 2006; Nezi et al. 2006). The resulting C-Mad2:O-Mad2 dimer has been visualized in two different x-ray crystal structures (Mapelli et al. 2007; Hara et al. 2015), and in both cases the O-Mad2 protomer adopts a subtly altered conformation compared to its structure in solution. This conformational shift is believed to promote dissociation of the C-terminal safety belt motif from its position occluding the closure motif binding site, resulting in a transient partially unfolded state (Mapelli and Musacchio 2007; Hara et al. 2015). Partially unfolded Mad2 is competent to associate with the Cdc20 KILR motif and refold into the closed state. The unique Mad1:Mad2-mediated conversion of soluble O-Mad2 to C-Mad2 has been termed the “Mad2 template model” (de Antoni et al. 2005; Musacchio and Salmon 2007; Mapelli and Musacchio 2007). After Mad2-Cdc20 binding, MCC assembly is completed when BubR1 binds both proteins as described above (Chao et al. 2012).
It has been understood for some time that in solution, O-Mad2 is less stable than C-Mad2 and will spontaneously convert to C-Mad2 with a half-time of several hours (Luo et al. 2004). Given that conversion of O-Mad2 to C-Mad2 is the rate-limiting step of MCC assembly, why does spontaneous conversion in solution not result in Cdc20 binding and MCC assembly? The key difference is likely the presence of Cdc20: binding of Mad2 to a closure motif can probably only occur in the transient partially unfolded state between O-Mad2 and C-Mad2, when the safety belt is disengaged from the HORMA domain core. Thus, the presence of Cdc20 at the time and place of Mad2 conformational conversion is likely key for complex formation. Further control over this assembly could be mediated by Mad1’s functionally mysterious C-terminal RWD domain, which is phosphorylated by Mps1 at unattached kinetochores, interacts directly with Cdc20, and may be required for initial Cdc20-Mad2 association (Faesen et al. 2017; Ji et al. 2017). Away from kinetochores, spontaneous O-Mad2 to C-Mad2 conversion probably results in “empty” C-Mad2 that not only does not nucleate MCC assembly (Fig. 6), but is actively harmful in that it cannot be recruited to kinetochores when needed (as Mad1:Mad2 specifically recruits O-Mad2). For this reason, spontaneous O-Mad2 to C-Mad2 conversion must be continually counteracted in the cell to maintain a functional SAC (see Sect. 5.2 and Fig. 6) (Ma and Poon 2016).
5 Silencing the SAC
5.1 Kinetochore Transformations
After all kinetochores become attached to microtubules, the SAC must be silenced to allow anaphase onset. To accomplish SAC silencing, kinetochores undergo a number of structural and compositional changes. First, Ndc80 binding to microtubules suppresses Mps1 activity, either by removing it from kinetochores or spatially segregating it from its substrates. At the same time, the activity of the Aurora B kinase, which phosphorylates a number of outer kinetochore components when kinetochores are not attached, including the Knl1 SILK/RVSF motif, is suppressed (regulation of Aurora B is discussed in detail in Lampson and Cheeseman 2011; Carmena et al. 2012; van der Horst and Lens 2014; Krenn and Musacchio 2015). The loss of these two kinase activities alters the balance of kinase/phosphatase activity at the outer kinetochore, first enabling Protein Phosphatase 2A (PP2A), recruited by BubR1, to dephosphorylate the Knl1 SILK/RVSF motif (Espert et al. 2014; Nijenhuis et al. 2014). The SILK/RVSF motif then binds protein phosphatase 1 (PP1) (Liu et al. 2010; Rosenberg et al. 2011; Meadows et al. 2011; London et al. 2012), which in turn dephosphorylates the Knl1 MELT repeats, resulting in loss of Bub1:Bub3 and all associated SAC components. The delicate balance of kinase and phosphatase activities at kinetochores, and how this balance is affected by microtubule attachment and other events, is outside the scope of this review but is covered in detail elsewhere (Suijkerbuijk et al. 2012b; Foley and Kapoor 2013; Espert et al. 2014; Nijenhuis et al. 2014; Etemad and Kops 2016). Finally, in organisms that possess the RZZ complex, RZZ and an associated protein called Spindly mediate the active “stripping” of Mad1:Mad2 from kinetochores upon microtubule attachment by linking Mad1:Mad2 to the microtubule minus-end directed motor dynein (Starr et al. 1998; Howell et al. 2001; Gassmann et al. 2008, 2010; Yamamoto et al. 2008; Chan et al. 2009; Barisic et al. 2010). Thus, microtubule attachment sets in motion a series of events that result in the dissociation of all SAC components from kinetochores, thereby halting MCC assembly.
5.2 MCC Disassembly and Degradation
In addition to halting assembly of new MCC, SAC silencing requires that existing MCC, both soluble and APC/C-Cdc20 bound, be disassembled and/or degraded. Two separate pathways have been identified that contribute to MCC turnover, one involving ubiquitination and degradation of Cdc20MCC, and the other involving direct disassembly of the MCC complex through the extraction of Mad2.
The first pathway for reactivation of inhibited APC/C-MCC complex involves the ubiquitination and subsequent degradation of Cdc20MCC (Pan and Chen 2004; King et al. 2007; Reddy et al. 2007; Ge et al. 2009; Foe et al. 2011). As noted above, the MCC not only occupies the degron-binding sites of the APC/C, it also sterically occludes binding of E2 enzymes to the APC/C catalytic module. Recent cryo-EM analysis of APC/C-MCC identified a minor conformational state (termed APC/C-MCC-open) in which the bound MCC is rotated away from the catalytic module, allowing binding of an E2 enzyme (Fig. 4) (Alfieri et al. 2016). A structure of the APC/C-MCC-open state with a bound E2, UbcH10, revealed how Cdc20MCC can be ubiquitinated while still bound to the APC/C (Alfieri et al. 2016). This work also revealed why the small APC/C subunit Apc15 is required for Cdc20MCC ubiquitination (Mansfeld et al. 2011; Foster and Morgan 2012; Uzunova et al. 2012): in the absence of Apc15, the APC/C-MCC-open state is not accessed, meaning that E2 binding and Cdc20MCC ubiquitination cannot occur (Alfieri et al. 2016). After ubiquitination of Cdc20MCC, this protein is presumably targeted to the proteasome for degradation, resulting in the reactivation of APC/C-Cdc20.
A second pathway for MCC turnover involves the direct disassembly of MCC by two proteins, p31comet and TRIP13 (Pch2 in yeast). p31comet is a HORMA domain protein distantly related to Mad2, that was first identified as a Mad2-binding protein (Habu et al. 2002; Xia et al. 2004). TRIP13 is a AAA+ family ATPase, which was first identified as a regulator of the Mad2-related HORMAD proteins in meiotic prophase (San-Segundo and Roeder 1999; Borner et al. 2008; Wojtasz et al. 2009; Vader 2015). Recently, TRIP13 was found to cooperate with p31comet in MCC disassembly and SAC inactivation (Teichner et al. 2011; Tipton et al. 2012; Eytan et al. 2014; Wang et al. 2014; Miniowitz-Shemtov et al. 2015; Ma and Poon 2016). Together, p31comet and TRIP13 specifically recognize C-Mad2 and convert it to the unbound O-Mad2 conformation (Ye et al. 2015). This enzymatic activity has multiple important functions, depending on context. First, p31comet and TRIP13 can directly disassemble soluble MCC (Mansfeld et al. 2011; Eytan et al. 2014). p31comet can also bind to APC/C-MCC, and some evidence suggests that Mad2 can be extracted from within APC/C-bound MCC, albeit less efficiently than from soluble MCC (Mansfeld et al. 2011; Westhorpe et al. 2011). Mad2 extraction from either soluble MCC or APC/C-MCC is a possible source of the BBC complex (BubR1, Bub3, Cdc20), which has been found to bind and inhibit the APC/C under certain conditions (Nilsson et al. 2008; Kulukian et al. 2009; Westhorpe et al. 2011; Han et al. 2013). It is likely that after Mad2 extraction, the remaining subunits of the MCC are still able to inhibit APC/C-Cdc20 to some extent. Ultimately, however, Mad2 extraction by p31comet and TRIP13 would destabilize the MCC, promoting dissociation and APC/C-Cdc20 reactivation.
p31comet and TRIP13 are conserved in plants, animals, and insects, but a clear fungal homolog of p31comet is missing, raising doubts about the conservation of the p31comet/TRIP13-mediated MCC disassembly pathway. Recently, however, a radically shortened p31comet relative, termed Tiny yeast comet 1 (Tyc1), has been identified in S. cerevisiae (Schuyler S.C., personal communication). The structural mechanisms of this protein, and how it relates to more canonical p31comet proteins, will be exciting to explore in the future.
Another question that remains largely unexplored is whether the two known pathways for MCC turnover, Cdc20MCC ubiquitination and p31comet/TRIP13-mediated Mad2 extraction, are functionally linked. Addition of p31comet to cell extracts arrested in metaphase by nocodazole treatment has been shown to promote Cdc20 ubiquitination (Reddy et al. 2007), suggesting that Mad2 extraction might promote formation of the APC/C-MCC-open state and thereby promote Cdc20MCC ubiquitination. The two pathways are not perfectly intertwined, however, as RNAi depletion of p31comet and the priming E2 enzyme UbcH10 (necessary for Cdc20 ubiquitination) has an additive effect on SAC inactivation (Reddy et al. 2007). Overall, the functional relationship between Cdc20MCC ubiquitination and MCC disassembly by p31comet and TRIP13 remains to be fully explored.
As noted above, O-Mad2 is unstable and spontaneously converts to C-Mad2 in vitro with a half-time of several hours (Luo et al. 2004). Based on the idea that this spontaneous conversion likely also occurs in the cell, we proposed that p31comet and TRIP13 might be involved in “recycling” this C-Mad2 by converting it back to O-Mad2 (Fig. 6) (Ye et al. 2015). This was recently shown to be the case: knockout of TRIP13 in human cells causes a profound defect in SAC activation, rendering these cells unresponsive to microtubule poisons such as nocodazole (Ma and Poon 2016). Biochemical examination shows that, indeed, Mad2 overwhelmingly adopts the closed conformation in these cells, and there is no detectable Mad2 binding to other MCC subunits (Ma and Poon 2016). Addition of exogenous TRIP13 to extracts from TRIP13-knockout cells re-establishes the predominance of O-Mad2 in solution (Ma and Poon 2016). In overall agreement with these results, work in Caenorhabditis elegans has also shown that p31comet and TRIP13 homologs (CMT-1 and PCH-2, respectively) are important for Mad2 recruitment to unattached kinetochores, and that loss of these factors causes defects in SAC activation (Nelson et al. 2015). Thus, p31comet and TRIP13 contribute to both SAC activation and inactivation by catalyzing the closed-to-open conformational change in Mad2.
6 Conclusion
Recent years have seen tremendous advances in our understanding of the molecular structures and protein–protein interactions underlying the SAC: the structure and mechanisms of the APC/C, its mode of inhibition by the MCC, and the mechanisms of MCC assembly and disassembly. We know much less about what occurs at kinetochores, including how they promote MCC assembly, and how their structure and composition changes in response to microtubule attachment/detachment and other signals. Finally, our understanding of SAC dynamics, particularly how it is able to respond quickly to changes in kinetochore-microtubule attachment status, is in its infancy. Thus, while recent advances in molecular understanding of SAC mechanisms represent an important step forward, a true holistic understanding of this fascinatingly complex pathway still awaits.
References
Alfieri C, Chang L, Zhang Z et al (2016) Molecular basis of APC/C regulation by the spindle assembly checkpoint. Nature 536:431–436. doi:10.1038/nature19083
Aravamudhan P, Goldfarb AA, Joglekar AP (2015) The kinetochore encodes a mechanical switch to disrupt spindle assembly checkpoint signalling. Nat Cell Biol 17:868–879. doi:10.1038/ncb3179
Aravind L, Koonin EV (1998) The HORMA domain: a common structural denominator in mitotic checkpoints, chromosome synapsis and DNA repair. Trends Biochem Sci 23:284–286
Barford D (2015) Understanding the structural basis for controlling chromosome division. Philos Trans A Math Phys Eng Sci 373:20130392. doi:10.1098/rsta.2013.0392
Barisic M, Geley S (2011) Spindly switch controls anaphase: spindly and RZZ functions in chromosome attachment and mitotic checkpoint control. Cell Cycle 10:449–456. doi:10.4161/cc.10.3.14759
Barisic M, Sohm B, Mikolcevic P et al (2010) Spindly/CCDC99 is required for efficient chromosome congression and mitotic checkpoint regulation. Mol Biol Cell 21:1968–1981. doi:10.1091/mbc.E09-04-0356
Borner GV, Barot A, Kleckner N (2008) Yeast Pch2 promotes domainal axis organization, timely recombination progression, and arrest of defective recombinosomes during meiosis. Proc Natl Acad Sci U S A 105:3327–3332. doi:10.1073/pnas.0711864105
Brown NG, VanderLinden R, Watson ER et al (2015) RING E3 mechanism for ubiquitin ligation to a disordered substrate visualized for human anaphase-promoting complex. Proc Natl Acad Sci U S A 112:5272–5279. doi:10.1073/pnas.1504161112
Brown NG, VanderLinden R, Watson ER et al (2016) Dual RING E3 architectures regulate multiubiquitination and ubiquitin chain elongation by APC/C. Cell 165:1440–1453. doi:10.1016/j.cell.2016.05.037
Buffin E, Lefebvre C, Huang J et al (2005) Recruitment of Mad2 to the kinetochore requires the Rod/Zw10 complex. Curr Biol 15:856–861. doi:10.1016/j.cub.2005.03.052
Burton JL, Xiong Y, Solomon MJ (2011) Mechanisms of pseudosubstrate inhibition of the anaphase promoting complex by Acm1. EMBO J 30:1818–1829. doi:10.1038/emboj.2011.90
Buschhorn BA, Petzold G, Galova M et al (2011) Substrate binding on the APC/C occurs between the coactivator Cdh1 and the processivity factor Doc1. Nat Struct Mol Biol 18:6–13. doi:10.1038/nsmb.1979
Caldas GV, Lynch TR, Anderson R et al (2015) The RZZ complex requires the N-terminus of KNL1 to mediate optimal Mad1 kinetochore localization in human cells. Open Biol 5:150160. doi:10.1098/rsob.150160
Carmena M, Wheelock M, Funabiki H, Earnshaw WC (2012) The chromosomal passenger complex (CPC): from easy rider to the godfather of mitosis. Nat Rev Mol Cell Biol 13:789–803. doi:10.1038/nrm3474
Chan YW, Fava LL, Uldschmid A et al (2009) Mitotic control of kinetochore-associated dynein and spindle orientation by human Spindly. J Cell Biol 185:859–874. doi:10.1083/jcb.200812167
Chang L, Barford D (2014) Insights into the anaphase-promoting complex: a molecular machine that regulates mitosis. Curr Opin Struct Biol 29:1–9. doi:10.1016/j.sbi.2014.08.003
Chang L, Zhang Z, Yang J et al (2014) Molecular architecture and mechanism of the anaphase-promoting complex. Nature 513:388–393. doi:10.1038/nature13543
Chang L, Zhang Z, Yang J et al (2015) Atomic structure of the APC/C and its mechanism of protein ubiquitination. Nature 522:450–454. doi:10.1038/nature14471
Chao WCH, Kulkarni K, Zhang Z et al (2012) Structure of the mitotic checkpoint complex. Nature 484:208–213. doi:10.1038/nature10896
Cheeseman IM, Niessen S, Anderson S et al (2004) A conserved protein network controls assembly of the outer kinetochore and its ability to sustain tension. Genes Dev 18:2255–2268. doi:10.1101/gad.1234104
Cheeseman IM, Chappie JS, Wilson-Kubalek EM, Desai A (2006) The conserved KMN network constitutes the core microtubule-binding site of the kinetochore. Cell 127:983–997. doi:10.1016/j.cell.2006.09.039
Ciferri C, Pasqualato S, Screpanti E et al (2008) Implications for kinetochore-microtubule attachment from the structure of an engineered Ndc80 complex. Cell 133:427–439. doi:10.1016/j.cell.2008.03.020
Ciosk R, Zachariae W, Michaelis C et al (1998) An ESP1/PDS1 complex regulates loss of sister chromatid cohesion at the metaphase to anaphase transition in yeast. Cell 93:1067–1076
Cohen-Fix O, Peters JM, Kirschner MW, Koshland D (1996) Anaphase initiation in Saccharomyces cerevisiae is controlled by the APC-dependent degradation of the anaphase inhibitor Pds1p. Genes Dev 10:3081–3093
da Fonseca PCA, Kong EH, Zhang Z et al (2011) Structures of APC/C(Cdh1) with substrates identify Cdh1 and Apc10 as the D-box co-receptor. Nature 470:274–278. doi:10.1038/nature09625
Davey NE, Morgan DO (2016) Building a regulatory network with short linear sequence motifs: lessons from the degrons of the anaphase-promoting complex. Mol Cell 64:12–23. doi:10.1016/j.molcel.2016.09.006
de Antoni A, Pearson CG, Cimini D et al (2005) The Mad1/Mad2 complex as a template for Mad2 activation in the spindle assembly checkpoint. Curr Biol 15:214–225. doi:10.1016/j.cub.2005.01.038
Desai A, Rybina S, Müller-Reichert T et al (2003) KNL-1 directs assembly of the microtubule-binding interface of the kinetochore in C. elegans. Genes Dev 17:2421–2435. doi:10.1101/gad.1126303
Di Fiore B, Davey NE, Hagting A et al (2015) The ABBA motif binds APC/C activators and is shared by APC/C substrates and regulators. Dev Cell 32:358–372. doi:10.1016/j.devcel.2015.01.003
Di Fiore B, Wurzenberger C, Davey NE, Pines J (2016) The mitotic checkpoint complex requires an evolutionary conserved cassette to bind and inhibit active APC/C. Mol Cell 64:1144–1153. doi:10.1016/j.molcel.2016.11.006
Diaz-Martinez LA, Tian W, Li B et al (2015) The Cdc20-binding Phe box of the spindle checkpoint protein BubR1 maintains the mitotic checkpoint complex during mitosis. J Biol Chem 290:2431–2443. doi:10.1074/jbc.M114.616490
Dou Z, Liu X, Wang W et al (2015) Dynamic localization of Mps1 kinase to kinetochores is essential for accurate spindle microtubule attachment. Proc Natl Acad Sci U S A 112:E4546–E4555. doi:10.1073/pnas.1508791112
Espert A, Uluocak P, Bastos RN et al (2014) PP2A-B56 opposes Mps1 phosphorylation of Knl1 and thereby promotes spindle assembly checkpoint silencing. J Cell Biol 206:833–842. doi:10.1083/jcb.201406109
Etemad B, Kops GJPL (2016) Attachment issues: kinetochore transformations and spindle checkpoint silencing. Curr Opin Cell Biol 39:101–108. doi:10.1016/j.ceb.2016.02.016
Eytan E, Wang K, Miniowitz-Shemtov S et al (2014) Disassembly of mitotic checkpoint complexes by the joint action of the AAA-ATPase TRIP13 and p31(comet). Proc Natl Acad Sci U S A 111:12019–12024. doi:10.1073/pnas.1412901111
Faesen AC, Thanasoula M, Maffini S et al (2017) In vitro reconstitution of spindle assembly checkpoint signaling identifies the determinants of catalytic assembly of the mitotic checkpoint complex. Nature 542:498–502. doi:10.1038/nature21384
Fang G (2002) Checkpoint protein BubR1 acts synergistically with Mad2 to inhibit anaphase-promoting complex. Mol Biol Cell 13:755–766. doi:10.1091/mbc.01-09-0437
Fang G, Yu H, Kirschner MW (1998) The checkpoint protein MAD2 and the mitotic regulator CDC20 form a ternary complex with the anaphase-promoting complex to control anaphase initiation. Genes Dev 12:1871–1883
Foe IT, Foster SA, Cheung SK et al (2011) Ubiquitination of Cdc20 by the APC occurs through an intramolecular mechanism. Curr Biol 21:1870–1877. doi:10.1016/j.cub.2011.09.051
Foley EA, Kapoor TM (2013) Microtubule attachment and spindle assembly checkpoint signalling at the kinetochore. Nat Rev Mol Cell Biol 14:25–37. doi:10.1038/nrm3494
Foster SA, Morgan DO (2012) The APC/C subunit Mnd2/Apc15 promotes Cdc20 autoubiquitination and spindle assembly checkpoint inactivation. Mol Cell 47:921–932. doi:10.1016/j.molcel.2012.07.031
Gassmann R, Essex A, Hu J-S et al (2008) A new mechanism controlling kinetochore-microtubule interactions revealed by comparison of two dynein-targeting components: SPDL-1 and the Rod/Zwilch/Zw10 complex. Genes Dev 22:2385–2399. doi:10.1101/gad.1687508
Gassmann R, Holland AJ, Varma D et al (2010) Removal of spindly from microtubule-attached kinetochores controls spindle checkpoint silencing in human cells. Genes Dev 24:957–971. doi:10.1101/gad.1886810
Ge S, Skaar JR, Pagano M (2009) APC/C- and Mad2-mediated degradation of Cdc20 during spindle checkpoint activation. Cell Cycle 8:167–171. doi:10.4161/cc.8.1.7606
Glotzer M, Murray AW, Kirschner MW (1991) Cyclin is degraded by the ubiquitin pathway. Nature 349:132–138. doi:10.1038/349132a0
Golan A, Yudkovsky Y, Hershko A (2002) The cyclin-ubiquitin ligase activity of cyclosome/APC is jointly activated by protein kinases Cdk1-cyclin B and Plk. J Biol Chem 277:15552–15557. doi:10.1074/jbc.M111476200
Habu T, Kim SH, Weinstein J, Matsumoto T (2002) Identification of a MAD2-binding protein, CMT2, and its role in mitosis. EMBO J 21:6419–6428
Han JS, Holland AJ, Fachinetti D et al (2013) Catalytic assembly of the mitotic checkpoint inhibitor BubR1-Cdc20 by a Mad2-induced functional switch in Cdc20. Mol Cell 51:92–104. doi:10.1016/j.molcel.2013.05.019
Hara M, Özkan E, Sun H et al (2015) Structure of an intermediate conformer of the spindle checkpoint protein Mad2. Proc Natl Acad Sci U S A 112:11252–11257. doi:10.1073/pnas.1512197112
Hardwick KG, Johnston RC, Smith DL, Murray AW (2000) MAD3 encodes a novel component of the spindle checkpoint which interacts with Bub3p, Cdc20p, and Mad2p. J Cell Biol 148:871–882. doi:10.1083/jcb.148.5.871
Hardwick KG, Weiss E, Luca FC et al (1996) Activation of the budding yeast spindle assembly checkpoint without mitotic spindle disruption. Science 273:953–956
He J, Chao WCH, Zhang Z et al (2013) Insights into degron recognition by APC/C coactivators from the structure of an Acm1-Cdh1 complex. Mol Cell 50:649–660. doi:10.1016/j.molcel.2013.04.024
Hendrickx A, Beullens M, Ceulemans H et al (2009) Docking motif-guided mapping of the interactome of protein phosphatase-1. Chem Biol 16:365–371. doi:10.1016/j.chembiol.2009.02.012
Herzog F, Primorac I, Dube P et al (2009) Structure of the anaphase-promoting complex/cyclosome interacting with a mitotic checkpoint complex. Science 323:1477–1481. doi:10.1126/science.1163300
Hiruma Y, Sacristan C, Pachis ST et al (2015) CELL DIVISION CYCLE. Competition between MPS1 and microtubules at kinetochores regulates spindle checkpoint signaling. Science 348:1264–1267. doi:10.1126/science.aaa4055
Howell BJ, McEwen BF, Canman JC et al (2001) Cytoplasmic dynein/dynactin drives kinetochore protein transport to the spindle poles and has a role in mitotic spindle checkpoint inactivation. J Cell Biol 155:1159–1172. doi:10.1083/jcb.200105093
Howell BJ, Moree B, Farrar EM et al (2004) Spindle checkpoint protein dynamics at kinetochores in living cells. Curr Biol 14:953–964. doi:10.1016/j.cub.2004.05.053
Hoyt MA, Totis L, Roberts BT (1991) S. cerevisiae genes required for cell cycle arrest in response to loss of microtubule function. Cell 66:507–517
Hwang LH, Lau LF, Smith DL et al (1998) Budding yeast Cdc20: a target of the spindle checkpoint. Science 279:1041–1044
Izawa D, Pines J (2012) Mad2 and the APC/C compete for the same site on Cdc20 to ensure proper chromosome segregation. J Cell Biol 199:27–37. doi:10.1083/jcb.201205170
Izawa D, Pines J (2014) The mitotic checkpoint complex binds a second CDC20 to inhibit active APC/C. Nature. doi:10.1038/nature13911
Jaspersen SL, Charles JF, Morgan DO (1999) Inhibitory phosphorylation of the APC regulator Hct1 is controlled by the kinase Cdc28 and the phosphatase Cdc14. Curr Biol 9:227–236
Ji Z, Gao H, Yu H (2015) Cell division cycle. Kinetochore attachment sensed by competitive Mps1 and microtubule binding to Ndc80C. Science 348:1260–1264. doi:10.1126/science.aaa4029
Ji Z, Gao H, Jia L et al (2017) A sequential multi-target Mps1 phosphorylation cascade promotes spindle checkpoint signaling. Elife 6:e22513. doi:10.7554/eLife.22513
Kallio M, Weinstein J, Daum JR et al (1998) Mammalian p55CDC mediates association of the spindle checkpoint protein Mad2 with the cyclosome/anaphase-promoting complex, and is involved in regulating anaphase onset and late mitotic events. J Cell Biol 141:1393–1406
Kamenz J, Hauf S (2016) Time to split up: dynamics of chromosome separation. Trends Cell Biol. doi:10.1016/j.tcb.2016.07.008
Karess R (2005) Rod-Zw10-Zwilch: a key player in the spindle checkpoint. Trends Cell Biol 15:386–392. doi:10.1016/j.tcb.2005.05.003
Kim SH, Lin DP, Matsumoto S et al (1998) Fission yeast Slp1: an effector of the Mad2-dependent spindle checkpoint. Science 279:1045–1047
King RW, Peters JM, Tugendreich S et al (1995) A 20S complex containing CDC27 and CDC16 catalyzes the mitosis-specific conjugation of ubiquitin to cyclin B. Cell 81:279–288
King EMJ, van der Sar SJA, Hardwick KG (2007) Mad3 KEN boxes mediate both Cdc20 and Mad3 turnover, and are critical for the spindle checkpoint. PLoS ONE 2:e342. doi:10.1371/journal.pone.0000342
Kops GJPL, Kim Y, Weaver BAA et al (2005) ZW10 links mitotic checkpoint signaling to the structural kinetochore. J Cell Biol 169:49–60. doi:10.1083/jcb.200411118
Kraft C, Herzog F, Gieffers C et al (2003) Mitotic regulation of the human anaphase-promoting complex by phosphorylation. EMBO J 22:6598–6609. doi:10.1093/emboj/cdg627
Kramer ER, Scheuringer N, Podtelejnikov AV et al (2000) Mitotic regulation of the APC activator proteins CDC20 and CDH1. Mol Biol Cell 11:1555–1569
Krenn V, Musacchio A (2015) The Aurora B kinase in chromosome bi-orientation and spindle checkpoint signaling. Front Oncol 5:225. doi:10.3389/fonc.2015.00225
Krenn V, Overlack K, Primorac I et al (2014) KI motifs of human Knl1 enhance assembly of comprehensive spindle checkpoint complexes around MELT repeats. Curr Biol 24:29–39. doi:10.1016/j.cub.2013.11.046
Kulukian A, Han JS, Cleveland DW (2009) Unattached kinetochores catalyze production of an anaphase inhibitor that requires a Mad2 template to prime Cdc20 for BubR1 binding. Dev Cell 16:105–117. doi:10.1016/j.devcel.2008.11.005
Labit H, Fujimitsu K, Bayin NS et al (2012) Dephosphorylation of Cdc20 is required for its C-box-dependent activation of the APC/C. EMBO J 31:3351–3362. doi:10.1038/emboj.2012.168
Lahav-Baratz S, Sudakin V, Ruderman JV, Hershko A (1995) Reversible phosphorylation controls the activity of cyclosome-associated cyclin-ubiquitin ligase. Proc Natl Acad Sci U S A 92:9303–9307
Lampson MA, Cheeseman IM (2011) Sensing centromere tension: Aurora B and the regulation of kinetochore function. Trends Cell Biol 21:133–140. doi:10.1016/j.tcb.2010.10.007
Lan W, Cleveland DW (2010) A chemical tool box defines mitotic and interphase roles for Mps1 kinase. J Cell Biol 190:21–24. doi:10.1083/jcb.201006080
Lara-Gonzalez P, Westhorpe FG, Taylor SS (2012) The Spindle Assembly Checkpoint. Curr Biol 22:R966–R980. doi:10.1016/j.cub.2012.10.006
Larsen NA, Al-Bassam J, Wei RR, Harrison SC (2007) Structural analysis of Bub3 interactions in the mitotic spindle checkpoint. Proc Natl Acad Sci U S A 104:1201–1206. doi:10.1073/pnas.0610358104
Li R, Murray AW (1991) Feedback control of mitosis in budding yeast. Cell 66:519–531
Li Y, Gorbea C, Mahaffey D et al (1997) MAD2 associates with the cyclosome/anaphase-promoting complex and inhibits its activity. Proc Natl Acad Sci U S A 94:12431–12436
Lischetti T, Zhang G, Sedgwick GG et al (2014) The internal Cdc20 binding site in BubR1 facilitates both spindle assembly checkpoint signalling and silencing. Nat Commun 5:5563. doi:10.1038/ncomms6563
Liu X, Winey M (2012) The MPS1 family of protein kinases. Annu Rev Biochem 81:561–585. doi:10.1146/annurev-biochem-061611-090435
Liu D, Vleugel M, Backer CB et al (2010) Regulated targeting of protein phosphatase 1 to the outer kinetochore by KNL1 opposes Aurora B kinase. J Cell Biol 188:809–820. doi:10.1083/jcb.201001006
London N, Biggins S (2014) Mad1 kinetochore recruitment by Mps1-mediated phosphorylation of Bub1 signals the spindle checkpoint. Genes Dev 28:140–152. doi:10.1101/gad.233700.113
London N, Ceto S, Ranish JA, Biggins S (2012) Phosphoregulation of Spc105 by Mps1 and PP1 regulates Bub1 localization to kinetochores. Curr Biol 22:900–906. doi:10.1016/j.cub.2012.03.052
Lukas C, Sørensen CS, Kramer E et al (1999) Accumulation of cyclin B1 requires E2F and cyclin-A-dependent rearrangement of the anaphase-promoting complex. Nature 401:815–818. doi:10.1038/44611
Luo X, Yu H (2008) Protein metamorphosis: the two-state behavior of Mad2. Structure 16:1616–1625. doi:10.1016/j.str.2008.10.002
Luo X, Fang G, Coldiron M et al (2000) Structure of the Mad2 spindle assembly checkpoint protein and its interaction with Cdc20. Nat Struct Biol 7:224–229. doi:10.1038/73338
Luo X, Tang Z, Rizo J, Yu H (2002) The Mad2 spindle checkpoint protein undergoes similar major conformational changes upon binding to either Mad1 or Cdc20. Mol Cell 9:59–71
Luo X, Tang Z, Xia G et al (2004) The Mad2 spindle checkpoint protein has two distinct natively folded states. Nat Struct Mol Biol 11:338–345. doi:10.1038/nsmb748
Ma HT, Poon RYC (2016) TRIP13 regulates both the activation and inactivation of the spindle-assembly checkpoint. Cell Reports 14:1086–1099. doi:10.1016/j.celrep.2016.01.001
Mansfeld J, Collin P, Collins MO et al (2011) APC15 drives the turnover of MCC-CDC20 to make the spindle assembly checkpoint responsive to kinetochore attachment. Nat Cell Biol 13:1234–1243. doi:10.1038/ncb2347
Mapelli M, Musacchio A (2007) MAD contortions: conformational dimerization boosts spindle checkpoint signaling. Curr Opin Struct Biol 17:716–725. doi:10.1016/j.sbi.2007.08.011
Mapelli M, Massimiliano L, Santaguida S, Musacchio A (2007) The Mad2 conformational dimer: structure and implications for the spindle assembly checkpoint. Cell 131:730–743. doi:10.1016/j.cell.2007.08.049
Martin-Lluesma S, Stucke VM, Nigg EA (2002) Role of Hec1 in spindle checkpoint signaling and kinetochore recruitment of Mad1/Mad2. Science 297:2267–2270. doi:10.1126/science.1075596
Matyskiela ME, Morgan DO (2009) Analysis of activator-binding sites on the APC/C supports a cooperative substrate-binding mechanism. Mol Cell 34:68–80. doi:10.1016/j.molcel.2009.02.027
Meadows JC, Shepperd LA, Vanoosthuyse V et al (2011) Spindle checkpoint silencing requires association of PP1 to both Spc7 and kinesin-8 motors. Dev Cell 20:739–750. doi:10.1016/j.devcel.2011.05.008
Miniowitz-Shemtov S, Eytan E, Kaisari S et al (2015) Mode of interaction of TRIP13 AAA-ATPase with the Mad2-binding protein p31comet and with mitotic checkpoint complexes. Proc Natl Acad Sci U S A 112:11536–11540. doi:10.1073/pnas.1515358112
Morgan DO (1997) Cyclin-dependent kinases: engines, clocks, and microprocessors. Annu Rev Cell Dev Biol 13:261–291. doi:10.1146/annurev.cellbio.13.1.261
Moyle MW, Kim T, Hattersley N et al (2014) A Bub1-Mad1 interaction targets the Mad1-Mad2 complex to unattached kinetochores to initiate the spindle checkpoint. J Cell Biol 204:647–657. doi:10.1083/jcb.201311015
Murray AW, Solomon MJ, Kirschner MW (1989) The role of cyclin synthesis and degradation in the control of maturation promoting factor activity. Nature 339:280–286. doi:10.1038/339280a0
Musacchio A (2015) The molecular biology of spindle assembly checkpoint signaling dynamics. Curr Biol 25:R1002–R1018. doi:10.1016/j.cub.2015.08.051
Musacchio A, Salmon ED (2007) The spindle-assembly checkpoint in space and time. Nat Rev Mol Cell Biol 8:379–393. doi:10.1038/nrm2163
Nagpal H, Fukagawa T (2016) Kinetochore assembly and function through the cell cycle. Chromosoma 125:645–659. doi:10.1007/s00412-016-0608-3
Nekrasov VS, Smith MA, Peak-Chew S, Kilmartin JV (2003) Interactions between centromere complexes in Saccharomyces cerevisiae. Mol Biol Cell 14:4931–4946. doi:10.1091/mbc.E03-06-0419
Nelson CR, Hwang T, Chen P-H, Bhalla N (2015) TRIP13/PCH-2 promotes Mad2 localization to unattached kinetochores in the spindle checkpoint response. J Cell Biol 211:503–516. doi:10.1083/jcb.201505114
Nezi L, Rancati G, de Antoni A et al (2006) Accumulation of Mad2-Cdc20 complex during spindle checkpoint activation requires binding of open and closed conformers of Mad2 in Saccharomyces cerevisiae. J Cell Biol 174:39–51. doi:10.1083/jcb.200602109
Nijenhuis W, von Castelmur E, Littler D et al (2013) A TPR domain-containing N-terminal module of MPS1 is required for its kinetochore localization by Aurora B. J Cell Biol 201:217–231. doi:10.1083/jcb.201210033
Nijenhuis W, Vallardi G, Teixeira A et al (2014) Negative feedback at kinetochores underlies a responsive spindle checkpoint signal. Nat Cell Biol 16:1257–1264. doi:10.1038/ncb3065
Nilsson J, Yekezare M, Minshull J, Pines J (2008) The APC/C maintains the spindle assembly checkpoint by targeting Cdc20 for destruction. Nat Cell Biol 10:1411–1420. doi:10.1038/ncb1799
Overlack K, Primorac I, Vleugel M et al (2015) A molecular basis for the differential roles of Bub1 and BubR1 in the spindle assembly checkpoint. Elife 4:e05269. doi:10.7554/eLife.05269
Pan J, Chen R-H (2004) Spindle checkpoint regulates Cdc20p stability in Saccharomyces cerevisiae. Genes Dev 18:1439–1451. doi:10.1101/gad.1184204
Pesenti ME, Weir JR, Musacchio A (2016) Progress in the structural and functional characterization of kinetochores. Curr Opin Struct Biol 37:152–163. doi:10.1016/j.sbi.2016.03.003
Pfleger CM, Kirschner MW (2000) The KEN box: an APC recognition signal distinct from the D box targeted by Cdh1. Genes Dev 14:655–665
Primorac I, Musacchio A (2013) Panta rhei: the APC/C at steady state. J Cell Biol 201:177–189. doi:10.1083/jcb.201301130
Primorac I, Weir JR, Chiroli E et al (2013) Bub3 reads phosphorylated MELT repeats to promote spindle assembly checkpoint signaling. Elife 2:e01030. doi:10.7554/eLife.01030
Qiao R, Weissmann F, Yamaguchi M et al (2016) Mechanism of APC/CCDC20 activation by mitotic phosphorylation. Proc Natl Acad Sci U S A 113:E2570–E2578. doi:10.1073/pnas.1604929113
Reddy SK, Rape M, Margansky WA, Kirschner MW (2007) Ubiquitination by the anaphase-promoting complex drives spindle checkpoint inactivation. Nature 446:921–925. doi:10.1038/nature05734
Reis A, Levasseur M, Chang H-Y et al (2006) The CRY box: a second APCcdh1-dependent degron in mammalian cdc20. EMBO Rep 7:1040–1045. doi:10.1038/sj.embor.7400772
Rieder CL, Cole RW, Khodjakov A, Sluder G (1995) The checkpoint delaying anaphase in response to chromosome monoorientation is mediated by an inhibitory signal produced by unattached kinetochores. J Cell Biol 130:941–948
Rosenberg JS, Cross FR, Funabiki H (2011) KNL1/Spc105 recruits PP1 to silence the spindle assembly checkpoint. Curr Biol 21:942–947. doi:10.1016/j.cub.2011.04.011
San-Segundo PA, Roeder GS (1999) Pch2 links chromatin silencing to meiotic checkpoint control. Cell 97:313–324
Schwab M, Neutzner M, Möcker D, Seufert W (2001) Yeast Hct1 recognizes the mitotic cyclin Clb2 and other substrates of the ubiquitin ligase APC. EMBO J 20:5165–5175. doi:10.1093/emboj/20.18.5165
Sczaniecka M, Feoktistova A, May KM et al (2008) The spindle checkpoint functions of Mad3 and Mad2 depend on a Mad3 KEN box-mediated interaction with Cdc20-anaphase-promoting complex (APC/C). J Biol Chem 283:23039–23047. doi:10.1074/jbc.M803594200
Shah JV, Botvinick E, Bonday Z et al (2004) Dynamics of centromere and kinetochore proteins; implications for checkpoint signaling and silencing. Curr Biol 14:942–952. doi:10.1016/j.cub.2004.05.046
Shepperd LA, Meadows JC, Sochaj AM et al (2012) Phosphodependent recruitment of Bub1 and Bub3 to Spc7/KNL1 by Mph1 kinase maintains the spindle checkpoint. Curr Biol 22:891–899. doi:10.1016/j.cub.2012.03.051
Shirayama M, Toth A, Gálová M, Nasmyth K (1999) APC(Cdc20) promotes exit from mitosis by destroying the anaphase inhibitor Pds1 and cyclin Clb5. Nature 402:203–207. doi:10.1038/46080
Shteinberg M, Protopopov Y, Listovsky T et al (1999) Phosphorylation of the cyclosome is required for its stimulation by Fizzy/cdc20. Biochem Biophys Res Commun 260:193–198. doi:10.1006/bbrc.1999.0884
Silió V, McAinsh AD, Millar JB (2015) KNL1-Bubs and RZZ provide two separable pathways for checkpoint activation at human kinetochores. Dev Cell 35:600–613. doi:10.1016/j.devcel.2015.11.012
Simonetta M, Manzoni R, Mosca R et al (2009) The influence of catalysis on mad2 activation dynamics. PLoS Biol 7:e10. doi:10.1371/journal.pbio.1000010
Sironi L, Mapelli M, Knapp S et al (2002) Crystal structure of the tetrameric Mad1-Mad2 core complex: implications of a “safety belt” binding mechanism for the spindle checkpoint. EMBO J 21:2496–2506. doi:10.1093/emboj/21.10.2496
Starr DA, Williams BC, Hays TS, Goldberg ML (1998) ZW10 helps recruit dynactin and dynein to the kinetochore. J Cell Biol 142:763–774
Sudakin V, Chan GK, Yen TJ (2001) Checkpoint inhibition of the APC/C in HeLa cells is mediated by a complex of BUBR1, BUB3, CDC20, and MAD2. J Cell Biol 154:925–936. doi:10.1083/jcb.200102093
Sudakin V, Ganoth D, Dahan A et al (1995) The cyclosome, a large complex containing cyclin-selective ubiquitin ligase activity, targets cyclins for destruction at the end of mitosis. Mol Biol Cell 6:185–197
Suijkerbuijk SJE, van Dam TJP, Karagöz GE et al (2012a) The vertebrate mitotic checkpoint protein BUBR1 is an unusual pseudokinase. Dev Cell 22:1321–1329. doi:10.1016/j.devcel.2012.03.009
Suijkerbuijk SJE, Vleugel M, Teixeira A, Kops GJPL (2012b) Integration of kinase and phosphatase activities by BUBR1 ensures formation of stable kinetochore-microtubule attachments. Dev Cell 23:745–755. doi:10.1016/j.devcel.2012.09.005
Tang Z, Bharadwaj R, Li B, Yu H (2001) Mad2-Independent inhibition of APCCdc20 by the mitotic checkpoint protein BubR1. Dev Cell 1:227–237
Taylor SS, Ha E, McKeon F (1998) The human homologue of Bub3 is required for kinetochore localization of Bub1 and a Mad3/Bub1-related protein kinase. J Cell Biol 142:1–11
Teichner A, Eytan E, Sitry-Shevah D et al (2011) p31comet Promotes disassembly of the mitotic checkpoint complex in an ATP-dependent process. Proc Natl Acad Sci U S A 108:3187–3192. doi:10.1073/pnas.1100023108
Thornton BR, Ng TM, Matyskiela ME et al (2006) An architectural map of the anaphase-promoting complex. Genes Dev 20:449–460. doi:10.1101/gad.1396906
Tipton AR, Wang K, Link L et al (2011) BUBR1 and closed MAD2 (C-MAD2) interact directly to assemble a functional mitotic checkpoint complex. J Biol Chem 286:21173–21179. doi:10.1074/jbc.M111.238543
Tipton AR, Wang K, Oladimeji P et al (2012) Identification of novel mitosis regulators through data mining with human centromere/kinetochore proteins as group queries. BMC Cell Biol 13:15. doi:10.1186/1471-2121-13-15
Uzunova K, Dye BT, Schutz H et al (2012) APC15 mediates CDC20 autoubiquitylation by APC/C(MCC) and disassembly of the mitotic checkpoint complex. Nat Struct Mol Biol 19:1116–1123. doi:10.1038/nsmb.2412
Vader G (2015) Pch2(TRIP13): controlling cell division through regulation of HORMA domains. Chromosoma 124:333–339. doi:10.1007/s00412-015-0516-y
van der Horst A, Lens SMA (2014) Cell division: control of the chromosomal passenger complex in time and space. Chromosoma 123:25–42. doi:10.1007/s00412-013-0437-6
Varma D, Salmon ED (2012) The KMN protein network–chief conductors of the kinetochore orchestra. J Cell Sci 125:5927–5936. doi:10.1242/jcs.093724
Vink M, Simonetta M, Transidico P et al (2006) In vitro FRAP identifies the minimal requirements for Mad2 kinetochore dynamics. Curr Biol 16:755–766. doi:10.1016/j.cub.2006.03.057
Vleugel M, Hoogendoorn E, Snel B, Kops GJPL (2012) Evolution and function of the mitotic checkpoint. Dev Cell 23:239–250. doi:10.1016/j.devcel.2012.06.013
Vleugel M, Tromer E, Omerzu M et al (2013) Arrayed BUB recruitment modules in the kinetochore scaffold KNL1 promote accurate chromosome segregation. J Cell Biol 203:943–955. doi:10.1083/jcb.201307016
Vleugel M, Hoek TA, Tromer E et al (2015a) Dissecting the roles of human BUB1 in the spindle assembly checkpoint. J Cell Sci 128:2975–2982. doi:10.1242/jcs.169821
Vleugel M, Omerzu M, Groenewold V et al (2015b) Sequential multisite phospho-regulation of KNL1-BUB3 interfaces at mitotic kinetochores. Mol Cell 57:824–835. doi:10.1016/j.molcel.2014.12.036
Vodermaier HC, Gieffers C, Maurer-Stroh S et al (2003) TPR subunits of the anaphase-promoting complex mediate binding to the activator protein CDH1. Curr Biol 13:1459–1468
Wang X, Babu JR, Harden JM et al (2001) The mitotic checkpoint protein hBUB3 and the mRNA export factor hRAE1 interact with GLE2p-binding sequence (GLEBS)-containing proteins. J Biol Chem 276:26559–26567. doi:10.1074/jbc.M101083200
Wang H, Hu X, Ding X et al (2004) Human Zwint-1 specifies localization of Zeste White 10 to kinetochores and is essential for mitotic checkpoint signaling. J Biol Chem 279:54590–54598. doi:10.1074/jbc.M407588200
Wang K, Sturt-Gillespie B, Hittle JC et al (2014) Thyroid hormone receptor interacting protein 13 (TRIP13) AAA-ATPase is a novel mitotic checkpoint-silencing protein. J Biol Chem 289:23928–23937. doi:10.1074/jbc.M114.585315
Wei RR, Al-Bassam J, Harrison SC (2007) The Ndc80/HEC1 complex is a contact point for kinetochore-microtubule attachment. Nat Struct Mol Biol 14:54–59. doi:10.1038/nsmb1186
Westhorpe FG, Tighe A, Lara-Gonzalez P, Taylor SS (2011) p31comet-mediated extraction of Mad2 from the MCC promotes efficient mitotic exit. J Cell Sci 124:3905–3916. doi:10.1242/jcs.093286
Wojtasz L, Daniel K, Roig I et al (2009) Mouse HORMAD1 and HORMAD2, two conserved meiotic chromosomal proteins, are depleted from synapsed chromosome axes with the help of TRIP13 AAA-ATPase. PLoS Genet 5:e1000702. doi:10.1371/journal.pgen.1000702
Xia G, Luo X, Habu T et al (2004) Conformation-specific binding of p31(comet) antagonizes the function of Mad2 in the spindle checkpoint. EMBO J 23:3133–3143. doi:10.1038/sj.emboj.7600322
Yamagishi Y, Yang C-H, Tanno Y, Watanabe Y (2012) MPS1/Mph1 phosphorylates the kinetochore protein KNL1/Spc7 to recruit SAC components. Nat Cell Biol 14:746–752. doi:10.1038/ncb2515
Yamaguchi M, VanderLinden R, Weissmann F et al (2016) Cryo-EM of mitotic checkpoint complex-bound APC/C reveals reciprocal and conformational regulation of ubiquitin ligation. Mol Cell 63:593–607. doi:10.1016/j.molcel.2016.07.003
Yamamoto TG, Watanabe S, Essex A, Kitagawa R (2008) SPDL-1 functions as a kinetochore receptor for MDF-1 in Caenorhabditis elegans. J Cell Biol 183:187–194. doi:10.1083/jcb.200805185
Yang M, Li B, Tomchick DR et al (2007) p31comet blocks Mad2 activation through structural mimicry. Cell 131:744–755. doi:10.1016/j.cell.2007.08.048
Ye Q, Rosenberg SC, Moeller A et al (2015) TRIP13 is a protein-remodeling AAA + ATPase that catalyzes MAD2 conformation switching. Elife 4:213. doi:10.7554/eLife.07367
Zachariae W, Schwab M, Nasmyth K, Seufert W (1998) Control of cyclin ubiquitination by CDK-regulated binding of Hct1 to the anaphase promoting complex. Science 282:1721–1724
Zhang Y, Lees E (2001) Identification of an overlapping binding domain on Cdc20 for Mad2 and anaphase-promoting complex: model for spindle checkpoint regulation. Mol Cell Biol 21:5190–5199. doi:10.1128/MCB.21.15.5190-5199.2001
Zhang G, Lischetti T, Nilsson J (2014) A minimal number of MELT repeats supports all the functions of KNL1 in chromosome segregation. J Cell Sci 127:871–884. doi:10.1242/jcs.139725
Zhang G, Lischetti T, Hayward DG, Nilsson J (2015) Distinct domains in Bub1 localize RZZ and BubR1 to kinetochores to regulate the checkpoint. Nat Commun 6:7162. doi:10.1038/ncomms8162
Zhang G, Mendez BL, Sedgwick GG, Nilsson J (2016a) Two functionally distinct kinetochore pools of BubR1 ensure accurate chromosome segregation. Nat Commun 7:12256. doi:10.1038/ncomms12256
Zhang H, Liu S-T, Department of Biological Sciences, University of Toledo, 2801 West Bancroft St., Toledo, OH 43606, USA (2016b) The mitotic checkpoint complex (MCC): looking back and forth after 15 years. AIMS Mol Sci 3:597–634. doi:10.3934/molsci.2016.4.597
Zhang S, Chang L, Alfieri C et al (2016c) Molecular mechanism of APC/C activation by mitotic phosphorylation. Nature 533:260–264. doi:10.1038/nature17973
Zhu T, Dou Z, Qin B et al (2013) Phosphorylation of microtubule-binding protein Hec1 by mitotic kinase Aurora B specifies spindle checkpoint kinase Mps1 signaling at the kinetochore. J Biol Chem 288:36149–36159. doi:10.1074/jbc.M113.507970
Acknowledgements
Thanks to Dhanya Cheerambathur, Pablo Lara-Gonzalez, and Arshad Desai for critical reading and input on the manuscript, and Andrea Musacchio and Scott Schuyler for sharing unpublished results. K.D.C. gratefully acknowledges support from the March of Dimes Foundation, National Institutes of Health (R01 GM104141), and the Ludwig Institute for Cancer Research.
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Corbett, K.D. (2017). Molecular Mechanisms of Spindle Assembly Checkpoint Activation and Silencing. In: Black, B. (eds) Centromeres and Kinetochores. Progress in Molecular and Subcellular Biology, vol 56. Springer, Cham. https://doi.org/10.1007/978-3-319-58592-5_18
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