The CM1 motif of Spc110 interacts with γ-TuSC and is essential for its oligomerization into an active nucleation template (Lin et al., 2014). Sequence alignments indicate that the N-terminus of Spc72 carries a CM1 motif (63–88 aa) that is, however, shorter (25 amino acids in Spc72 versus 78 in Spc110) than the canonical CM1 motifs in budding yeast Spc110, Drosophila CNN and human CDK5RAP2 (Figure 1a) (Lin et al., 2014; Lin et al., 2015; Usui et al., 2003). The CM1 of Spc72 probably only reflects the CM1a portion of Spc110 while CM1b is missing (Lin et al., 2016). We asked whether the truncated CM1 of Spc72 is essential for its function by mutating three conserved residues to alanine (spc72^CM1; K75A, K77A, E83A) (Figure 1a). spc72^CM1 did not support the growth of yeast cells, indicating the essential function of the CM1 motif (Figure 1b).

Figure 1

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Amino acid substitutions in CM1 of Candida albicans Spc110 or human CDK5RAP2 impair binding to the γ-tubulin complexes (Choi et al., 2010; Lin et al., 2016). To test for the interaction of Spc72 with the γ-TuSC,we designed constructs expressing the N-terminal portion from amino acids (aa) 1–267 (Spc72N), a mutant CM1 version (Spc72N^CM1; aa 1–267 with K75A, K77A, E83A) and a Stu2-binding deficient mutant (Spc72N^∆Stu2; Spc72N with deletion of aa 116–230). In pulldown experiments, γ-TuSC showed reduced binding to Spc72N^CM1 in comparison to Spc72N or Spc72N^∆Stu2 (Figure 1c, Spc97-blot). Quantification of the interaction affinities by microscale thermophoresis (MST) determined the dissociation constant (K_d) of the Spc72N–γ-TuSC interaction with the high value of 1.1 µM, which reflects a relatively low binding affinity (Figure 1d). The Spc72N^CM1 mutant protein did not show binding to γ-TuSC in this assay (Figure 1d). Importantly, the binding affinity of γ-TuSC to the truncated N-terminal construct of Spc110 (Spc110N, aa 1–220) was 20-fold higher than that of Spc72N (compare Figure 1d and e). Also in case of Spc110, a mutant CM1 version (Spc110N^CM1, K120Q; E121A) showed reduced binding affinity (Figure 1e). In conclusion, Spc72 can bind the γ-TuSC dependent on the CM1, but with a 20-fold lower affinity than Spc110.

The relatively low affinity (high K_d) of Spc72 for γ-TuSC raises the question of how this receptor recruits the γ-TuSC to the SPB efficiently. Stu2, which interacts with Spc72, could mediate the binding of γ-TuSC to Spc72. To test this notion, we quantified the interactions between Spc72 and Stu2, as well as the Spc72–Stu2 complex and the interaction with γ-TuSC. The requirement for the last 33 aa of Stu2 (Figure 2a) and for aa 116 to 230 of Spc72 (Figure 1a) for the Spc72–Stu2 interaction was confirmed in pulldown experiments (Figure 2—figure supplement 1a and b) (Usui et al., 2003). Quantitative MST measurements determined the K_d of the Spc72N and Stu2 interaction as 115 nM (Figure 2b). This high-affinity binding was dependent on the Stu2-binding site of Spc72 and the C-terminus of Stu2, as Spc72N^∆Stu2 showed 23-fold reduced binding to Stu2 (Figure 2b) and because a Stu2 construct that lacks the 33 C-terminal aa (Stu2^∆C) did not interact with Spc72N (Figure 2b). Surprisingly, Spc72N^CM1also reduced the binding affinity to Stu2 in the quantitative MST assay (Figure 2b). Thus, mutations in the CM1 motif of Spc72 not only affect the interaction of Spc72 with γ-TuSC (Figure 1d) but also Spc72 binding to Stu2, indicating an unexpected interdependency between both binding sites in Spc72.

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To study the Spc72–Stu2 interaction with γ-TuSC, we developed a scheme for the purification of recombinant Spc72N–Stu2 complexes (Figure 2—figure supplement 1c and d). γ-TuSC bound to the pre-assembled Spc72N–Stu2 complex with 22-fold higher affinity than to Spc72N alone (compare Figure 1d and Figure 2c). Next, we asked whether direct binding of Stu2 to the γ-TuSC could be the reason for the enhanced interaction. Indeed, MST measurements indicated high-affinity binding of Stu2 to the γ-TuSC with a K_d of 63.4 nM (Figure 2d). To understand which domain of Stu2 was responsible for this interaction with γ-TuSC, we used pulldown assays with the recombinant TOG domains of Stu2 (Stu2^TOG; described in [Widlund et al., 2012]) and the fragment spanning the MT binding region of Stu2 (Stu2^MT; aa 451–684). As expected, α/β-tubulin bound efficiently to the Stu2^TOG construct (Ayaz et al., 2012; Widlund et al., 2012) but such binding was not observed for the purified γ-TuSC (Figure 2—figure supplement 1e; Tub4-blot). By contrast, Stu2^MT pulled down the γ-TuSC (Figure 2—figure supplement 1f; Spc97-blot) but failed to interact with α/β-tubulin. Thus, we were able to show that the Stu2 protein probably enhances the Spc72–γ-TuSC interaction by binding to both Spc72 and γ-TuSC.

Spc110 oligomerizes γ-TuSC into MT nucleation-competent rings dependent on its CM1 motif (Kollman et al., 2010; Lin et al., 2014). A shift of the γ-TuSC monomer towards earlier elution fractions in size exclusion chromatography is an indication of this activity (Lin et al., 2014). We were interested in whether Spc72 with the shorter CM1 had a similar impact on γ-TuSC. In comparison to Spc110N, Spc72N had only weak γ-TuSC oligomerization activity (compare Figure 2e with Figure 2—figure supplement 2a and b). This weak activity of Spc72N was further decreased in the case of Spc72N^CM1 (compare Figure 2e with Figure 2—figure supplement 2c). In marked contrast, the complex of Spc72N and wildtype (WT) Stu2 (Stu2^WT; complex: Spc72N–Stu2^WT) shifted a larger portion of the γ-TuSC into the Dextran blue marked void volume fractions than did Spc72N alone (Figure 2e). A Stu2 mutant protein carrying a single mutation in each of the two TOG domains (Stu2^TOGAA; R200A, R519A, see Figure 3c for illustration) (Ayaz et al., 2014; Geyer et al., 2015) in complex with Spc72N also shifted γ-TuSC to the void volume fractions similarly to Spc72N–Stu2^WT (Figure 2—figure supplement 2d). Analysis of the γ-TuSC–Spc72N and γ-TuSC–Spc72N-Stu2^WT complexes that eluted in the void volume of the gel filtration column by negative staining electron microscopy identified circular γ-TuSC assemblies that were denser and more complex when Stu2 was present (Figure 2—figure supplement 2e). Thus, the Spc72N–Stu2 complex induces γ-TuSC oligomerization into assemblies.

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Next, we tested whether Stu2 alone can also induce oligomerization of the γ-TuSC. Incubation of purified Stu2^WT with γ-TuSC for 40 min on ice led to the formation of sedimentable Stu2^WT–γ-TuSC oligomers (Figure 2—figure supplement 2f). Interestingly, this property of Stu2 was dependent on its MT-binding region as a Stu2 mutant in which this domain was deleted (Stu2^∆MT; deletion of aa 550–658, see Figure 3c for illustration) did not have the same impact on γ-TuSC. This indicates that Stu2 can assemble γ-TuSC into larger assemblies dependent on its MT-binding site.

The data presented above indicate that Spc72–Stu2 forms a complex with γ-TuSC and oligomerizes γ-TuSC into circular assemblies. To understand the relative contribution of each of the components in MT formation, we analysed the MT nucleation activity of purified Stu2 and Spc72N and of the Spc72N–Stu2 complex with (Figure 4) and without (Figure 3) recombinant γ-TuSC in an in vitro MT nucleation assay. Fluorescently labelled α/β-tubulin was incubated with purified proteins either individually or in combination. The α/β-tubulin concentration of 12 µM was chosen because it enables the oligomerized Spc110N–γ-TuSC to nucleate microtubules (Kollman et al., 2010; Lin et al., 2014). A similar α/β-tubulin concentration has been used in MT nucleation assays with purified TPX2 and chTOG (Roostalu et al., 2015). Assembled MTs were spun onto cover slips and analysed by fluorescence microscopy.

Figure 4

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Purified Spc72N did not have MT nucleation activity as it behaved similarly to the α/β-tubulin control (Figure 3a; see Figure 4b for quantification). The MT polymerase Stu2 occasionally nucleated MT asters (Figure 3a and b), but the overall MT nucleation activity of Stu2^WT was low (Figure 3—figure supplement 1b). The Spc72N–Stu2^WT complex promoted MT aster formation with greater frequency than did Stu2^WT alone (Figure 3a and b), leading to an increase in MT nucleation activity (Figure 4b). The aster-forming activity was dependent on the preassembled Spc72N–Stu2^WT complex as addition of the individual Spc72N and Stu2^WT proteins to the reaction mixture did not promote aster formation beyond the activity of Stu2 alone (Figure 3—figure supplement 1c; Spc72N + Stu2^WT). Thus, the recombinant Stu2–Spc72^WT complex predominately assembles MTs in the form of asters.

We next analysed the subdomains in Stu2 for their importance in MT nucleation. For this, mutant versions of Stu2 were constructed as outlined in Figure 3c. We confirmed that the recombinant Stu2^TOGAA protein failed to bind α/β-tubulin in gel filtration and pulldown assays (Figure 3—figure supplement 1d and e) (Ayaz et al., 2012). Stu2^∆MT and a Stu2 variant with a deletion of the dimerizing coiled-coil domain (Stu2^∆CC; deletion of aa 658–761, see Figure 3c) were constructed as reported previously (Al-Bassam et al., 2006; Wang and Huffaker, 1997). A yeast growth test indicated that all STU2 sub-regions were important for viability. stu2^∆MT and stu2^TOGAA cells failed to grow at 23°C or 37°C. stu2^∆CC and stu2^∆C cells grew at 23°C but showed reduced growth at 37°C (Figure 3—figure supplements 1f, 5-FOA) and behaved in a dominant-negative manner at 37°C as indicated by growth retardation of cells carrying WT and mutant versions of STU2 (Figure 3—figure supplement 1f; compare growth of cells at 23°C and 37°C on SC-Leu plates).

Next, Stu2 proteins were expressed and purified from insect cells either as a Stu2 version or in complex with Spc72N (Figure 2—figure supplement 1c and d). Stu2^TOGAA, Stu2^∆MT and Stu2^∆CC in combination with α/β-tubulin lacked the weak MT aster-forming ability of the Stu2^WT (Figure 3—figure supplement 1a and c). In addition, Stu2^∆MT and Stu2^∆CC in complex with Spc72N did not assemble MT asters, as was the case for Spc72N–Stu2^WT (Figure 3b and d). Interestingly, Spc72N–Stu2^TOGAA assembled asters with the same frequency as Spc72N–Stu2^WT (Figure 3b and d) that had a similar MT intensity (Figure 3e and f). However, the overall MT nucleation activity of Spc72N–Stu2^WT was slightly higher than that of Spc72–Stu2^TOGAA (Figure 4b). Thus, Stu2 in complex with Spc72 assembles MT asters dependent on its MT-binding site and the dimerizing coiled-coil region. In this assay, mutations in the TOG domains of Stu2 did not affect the density of the MTs in the asters but the overall MT nucleation activity was slightly reduced.

As next a step, we measured the impact of γ-TuSC combined with Spc72N, Stu2 and Spc72N–Stu2 for MT nucleation. Incubation of α/β-tubulin with γ-TuSC led to the formation of single MTs. However, the nucleation activity was low (Figure 4a and b). The addition of Spc72N to γ-TuSC produced a similarly low MT nucleation activity (Figure 4a and b), probably reflecting the poor oligomerization of γ-TuSC by Spc72N (Figure 2e). Interestingly, γ-TuSC enhanced the MT nucleation and aster-forming activities of Stu2–Spc72N by factors of 3.1 and 1.5, respectively (Figure 4a,b and c). For this enhancement, Stu2 had to be in complex with Spc72N as the MT nucleation and aster-formation activity of Stu2 alone was not changed upon the addition of γ-TuSC (Figure 3—figure supplement 1a to c). Thus, γ-TuSC increases the ability of the Spc72–Stu2 complex to nucleate MTs and to form asters.

Subsequently, we tested the domains of Stu2 that were needed for MT nucleation together with γ-TuSC. Aster formation by Spc72N–Stu2–γ-TuSC complex was dependent on the dimerizing coiled-coil region and the MT-binding domain of Stu2 (Figure 4a and b). The two TOG domains of Stu2 did not influence the number of MT asters formed by Spc72N–Stu2–γ-TuSC (Figure 4a and c). However, MT asters, which assembled in the presence of Spc72N–Stu2–γ-TuSC, were denser than those formed by Spc72N–Stu2^TOGAA-γ-TuSC (Figure 3f and Figure 4d). This reduction in aster density was reflected in a lower overall MT nucleation activity of Spc72N–Stu2^TOGAA-γ-TuSC compared to that of Spc72N–Stu2^WT-γ-TuSC (Figure 4b). As Spc72N–Stu2^TOGAA efficiently assembled γ-TuSC oligomers (Figure 2—figure supplement 2d), it is likely that the reduction of the MT density in the Spc72N–Stu2^TOGAA-γ-TuSC asters is caused by a decrease in the MT polymerization activity of Stu2^TOGAA.

This analysis indicates that Spc72N–Stu2 efficiently assembles MTs in cooperation with γ-TuSC. The TOG domains, the MT-binding site and the dimerizing coiled-coil region of Stu2 are required for the full MT nucleation activity of the Spc72N–Stu2–γ-TuSC complex.

We next used a series of in vivo experiments to test the role of Stu2 in maintaining γ-TuSC at the minus end of detached cMTs (Figure 5 and Figure 6) and the function of Stu2 and Tub4 in cMT nucleation (Figure 7). Because the nuclear export of Stu2 is cell-cycle regulated (van der Vaart et al., 2017), we performed these experiments in α-factor-arrested G₁ cells when Stu2 is mainly cytoplasmic to exclude cell-cycle effects.

Figure 5

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In order to obtain detached cMTs with a bound MT nucleation site at the minus end, we treated kar1∆15 cells with α-factor. In the presence of α-factor, it is the Kar1–Spc72 interaction that anchors cMTs to the bridge structure of the SPB (Pereira et al., 1999). The mutated Kar1∆15 protein lacks the region that mediates Spc72 binding. Therefore, in around 40% of kar1∆15 cells, cMTs detach from the SPB into the cytoplasm in response to α-factor treatment (Figure 5a). Previously, we have shown by electron tomography that detached cMTs are single MTs with a Spc72–γ-TuSC cap at their minus end (Erlemann et al., 2012). We noticed that in around 70% of cells, the minus end of detached cMTs (as marked by Spc72 or Tub4) localized within the schmoo tip region (2 µm radius). This orientation is probably a reflection of the association of the minus end motor Kar3 with the schmoo tip (Maddox et al., 2003), pulling the detached cMT minus ends into the schmoo.

We first used this system of detached cMTs to study the localisation of Stu2 at the cMT minus end. In 85% of SPC72 kar1∆15 cells with detached cMTs, Stu2–yeGFP was enriched together with Spc72–mCherry at the minus end of cMTs (Figure 5b, top). About 15% of detached cMTs did not carry a Stu2 peak signal that overlapped with Spc72 (Figure 5b, bottom). Stu2–yeGFP weakly decorated the MT wall of both detached cMT types (Figure 5b). Surprisingly, Stu2–yeGFP also associated with the minus end marker Tub4–mCherry in the majority (61%) of spc72^∆Stu2 kar1∆15 cells with detached cMTs (Figure 5c, top), whereas 39% of detached cMTs did not show Stu2 enrichment with Tub4 (Figure 5c, bottom). Spc72^∆Stu2 still localized to the end of detached cMT (Figure 6—figure supplement 1a). The Spc72–yeGFP and Stu2–yeGFP signals at the minus end of detached cMTs were quantified in order to gain a better understanding of their recruitment to this site. The normalized signal intensity at the cMT minus end was 0.19 for Spc72–yeGFP and 0.95 for Stu2–yeGFP in WT kar1∆15 cells (Figure 5d and e). In spc72^∆Stu2 kar1∆15 cells, the normalized intensity was 0.17 for Spc72^∆Stu2-yeGFP and 1.25 for Stu2–yeGFP (Figure 5d and e). Together, this evidence indicates a five-fold excess of Stu2 over Spc72 at cMT nucleation sites, as well as Spc72-independent recruitment of Stu2 to the cMT minus end.

The existence of another Stu2 interaction partner at the cMT minus end was further supported by fluorescence recovery after photobleaching (FRAP) experiments. Spc72–yeGFP at detached cMTs showed no recovery after bleaching. By contrast, 58% of Stu2–yeGFP recovered with a half time of 3.3 s, indicating a dynamic and stable Stu2 pool (Figure 5f). In spc72^∆Stu2 kar1∆15 cells, Stu2–yeGFP at cMTs ends almost completely recovered with a half time of 5.6 s. The complete recovery in the latter experiment also ruled out the possibility of the limitation of freely available Stu2–yeGFP, as the analyzed spc72^∆Stu2 kar1∆15 cells showed higher Stu2–yeGFP signal intensity at the cMT minus end before bleaching in comparison to SPC72 kar1∆15 (Figure 5f). In conclusion, a stable fraction of Stu2 binds to the minus end of cMTs via Spc72 and a dynamic fraction binds via an additional factor.

We wanted to identify the second recruitment factor for Stu2 at the minus end of cMTs. A possible candidate was the MT-associated protein Kar9, which localises to the SPB in a process that is dependent on the C-terminus of γ-tubulin Tub4 (Cuschieri et al., 2006). In addition, Kar9 is a known interaction partner of Stu2 (Miller et al., 2000; Moore and Miller, 2007). Consistent with these interactions, Kar9 co-localized dot-like with Spc72–mCherry at 81% of detached cMTs (Figure 6a and Figure 6—figure supplement 1b). Quantification of the Kar9–yeGFP single intensity at the minus end of detached cMTs indicated a high relative abundance of 1.79 in SPC72 kar1∆15 cells (normalized to Cse4–yeGFP) that was even further increased to 3.27 in spc72^∆Stu2 kar1∆15 cells (Figure 6—figure supplement 1c). Thus, the lack of the Stu2-binding site in Spc72 increases Kar9 recruitment to the cMT minus end. Considering Stu2 binding to Kar9 (Miller et al., 2000; Moore and Miller, 2007), this result provides an explanation for the enhanced binding of Stu2 to the cMT minus end in spc72^∆Stu2 cells (Figure 5e).

To show that a fraction of Stu2 is indeed recruited to the cMT minus end via Kar9, we constructed endogenous KAR9 gene fusions with the auxin-induced degron (AID)-tag (Nishimura et al., 2009). Addition of the auxin homologue IAA to KAR9–AID kar1∆15 cells promoted the degradation of Kar9–AID (Figure 6—figure supplement 1d) and decreased Stu2–yeGFP intensity at cMT minus ends from 0.95 to 0.44 (Figure 6b). By contrast, Spc72 was not affected by the depletion of Kar9 (Figure 6c). These data support the notion that Kar9 is the second Stu2-binding factor at the cMT minus end. Therefore, the depletion of Kar9 in spc72^∆Stu2 cells should further decrease Stu2–yeGFP intensity at the minus end of detached cMTs. However, as outlined below, these measurements were complicated by the instability of cMTs in spc72^∆Stu2 KAR9–AID kar1∆15 cells and by the observation that of the surviving detached cMTs only half carried Tub4 (Figure 6f and g). The normalized Stu2–yeGFP signal intensity at these rare Tub4-positive cMT minus ends was measured with ~0.82, which is clearly higher than the signal in KAR9–AID cells (0.44; compare Figure 5e with Figure 6b). This suggests that Kar9–AID was not fully degraded in these spc72^∆Stu2 KAR9–AID cells with detached cMTs. Indeed, variations between yeast cells in the efficiency of the auxin-induced degradation of proteins have been reported (Papagiannakis et al., 2017). This residual amount of Kar9–AID in the small number of spc72^∆Stu2 KAR9–AID cells with cMTs was, however, below the detection limit of the immunoblot in Figure 6—figure supplement 1d. Taken together, this evidence suggests that Kar9 and Spc72 recruit Stu2 to the minus end of cMTs.

Subsequently, we aimed to analyse the function of Stu2 at the minus end of detached cMTs. We used KAR9–AID in combination with the spc72^∆Stu2 mutation in order to reduce Stu2 specifically at the minus end of cMTs. kar1∆15 cells were incubated with α-factor for 60 min simultaneously with the addition of IAA or the solvent control. spc72^∆Stu2 KAR9–AID kar1∆15 cells that were exposed to IAA showed a reduction in cMT numbers (33%; attached and detached) in comparison to the SPC72 KAR9–AID kar1∆15 cells (Figure 6d), indicating a function for Stu2 in the nucleation or stability of cMTs.

The C-terminal 33 aa of Stu2 mediate binding with Spc72 and Kar9 (Moore and Miller, 2007; Usui et al., 2003). Therefore, we would expect that stu2^∆C kar1∆15 cells would show a reduction in cMT number similar to that shown by spc72^∆Stu2 KAR9–AID kar1∆15 cells that have been exposed to IAA. This was indeed the case (Figure 6—figure supplement 1e). Using immunoblotting, we confirmed that Stu2^∆C was expressed similarly to WT Stu2 (Figure 6—figure supplement 1f). Together, these experiments led us to conclude that the impairment of both Stu2-binding sites at the cMT minus end affects cMT stability or nucleation.

To further clarify the role of Stu2 in cMT function, we performed a time course experiment with spc72^∆Stu2 KAR9 kar1∆15 cells and spc72^∆Stu2 KAR9–AID kar1∆15 cells (Figure 6e). In this experiment, Kar9 was depleted after detachment of cMTs from the SPB, meaning that we analysed the function of Stu2 on the preassembled γ-TuSC oligomere. We observed that the number of detached cMTs in spc72^∆Stu2 KAR9–AID kar1∆15 cells gradually decreased from 50% (t = 0) to 25% within 60 min after the addition of IAA (Figure 6f). This decrease coincided with a general decline in cMT-number in spc72^∆Stu2 KAR9–AID kar1∆15 cells in the presence of IAA from 83% to 27%. Thus, Stu2 at the minus end of detached cMTs is probably needed for their stability.

One possible interpretation of the outcome of the experiment in Figure 6f is the detachment of the γ-TuSC cap, followed by MT depolymerisation when Stu2 is removed from the cMT minus end. Indeed, IAA addition to spc72^∆Stu2 KAR9–AID kar1∆15 cells reduced not only the number of cMTs but also the percentage of detached cMTs with a Tub4 signal from close to 100% to 54% (Figure 6g). This analysis suggests that Stu2 removal from the cMT minus end triggers the disassembly of γ-TuSC cap followed by cMT depolymerisation. It is in agreement with the in vitro data illustrated in Figure 2, indicating a stabilizing role for Stu2 in the Spc72–γ-TuSC interaction.

Figure 6 has shown a function of Stu2 in maintaining the γ-TuSC oligomer at the minus end of assembled cMTs. To judge the impact of Tub4 and Stu2 on MT nucleation, we developed an in vivo cMT nucleation assay using TUB4–AID or STU2–AID degron cells with the SPB marker SPC42–mCherry and the MT marker GFP–TUB1.

We first analysed the role of Tub4 in cMT nucleation. The addition of IAA to TUB4–AID cells induced the degradation of Tub4–AID below the critical threshold that was needed for viability (Figure 7—figure supplement 1a). However, we noticed that ~10% of Tub4–AID resisted degradation (Figure 7—figure supplement 1b). Next, TUB4 and TUB4–AID cells were arrested with α-factor in G₁ followed by the addition of nocodazole to depolymerize MTs and of IAA to induce degradation of Tub4–AID. Finally, nocodazole was washed out to promote MT re-nucleation (Figure 7a). In all strain backgrounds, close to 100% of the cells invariably lacked MTs upon nocodazole treatment (Adams and Pringle, 1984; Gombos et al., 2013). In response to nocodazole wash out, MTs re-polymerized in WT TUB4 cells as analysed after 30 min (Figure 7b). Only the nuclear MTs overlapped with the NLS–BFP (the nuclear localization signal fused to a blue fluorescence protein) staining region, whereas cMTs did not (Figure 7b), so we were able to distinguish the two MT-types clearly. About 97% of WT cells carried cMTs after 30 min of nocodazole wash out (Figure 7b). Most (86%) of these cMTs were associated with the Spc42–mCherry-marked SPB. Surprisingly, IAA-induced depletion of Tub4 only mildly affected cMT nucleation efficiency as 90% of the cells carried cMTs after 30 min (Figure 7b). Strikingly, about 45% of these cMTs were not associated with the SPB but resided in the cytoplasm away from the NLS–BFP-marked nucleus. Analysis of the localization of the γ-TuSC receptor Spc72–mCherry, and of the γ-TuSC complex components Spc97–mCherry and Spc98–mCherry in TUB4–AID cells after nocodazole wash out, indicated that the free cMTs did not contain Spc72, Spc97 or Spc98 (Figure 7c, left). In a control experiment, we established that these proteins were detected at the minus end of detached cMTs of kar1∆15 cells (Figure 7c, right) (Erlemann et al., 2012). Thus, our detection system was sensitive enough to visualize Spc72, Spc97 and Spc98 at the minus end of single cMTs. These data suggest γ-TuSC-independent cMT nucleation in TUB4–AID cells.

The nuclear MTs at the SPB of TUB4–AID cells were, however, associated with Spc97 and Spc98 (Figure 7c). The residual Tub4 in these cells (Figure 7—figure supplement 1b) was probably sufficient to assemble γ-TuSC, which then became concentrated in the nucleus by the nuclear localization signal in Spc98 (Pereira et al., 1998).

It was important to exclude the possibility that detached cMTs of TUB4–AID cells nucleate first at the SPB and then detach from this localization. For this, we performed live-cell image analysis of cells after nocodazole wash out. In Tub4-depleted TUB4–AID SPC42–mCherry GFP–TUB1 cells, cMTs were assembled spontaneously away from the SPB (Videos 1 and 2). By contrast, in TUB4 WT cells, cMTs formed at the Spc42–mCherry marked SPB (Video 3). This analysis eliminates the possibility of cMT formation at the SPB in TUB4–AID cells followed by their detachment.

Video 1

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To judge the efficiency of cMT assembly in Tub4-depleted cells, we compared the kinetics of cMT formation in WT TUB4 and TUB4–AID cells using the live-cell imaging data. Upon nocodazole wash out, TUB4–AID cells assembled cMTs with kinetics and efficiency that were similar to those observed in WT cells, with the difference that the majority of cMTs in TUB4–AID cells were not associated with the SPB (Figure 7d; note that the free cMTs of TUB4–AID cells were more frequent in the MatTek dish live-cell imaging experiment than in the flask experiment in Figure 7b). Taken together, these experiments indicate that cells can efficiently nucleate cMTs without the involvement of the receptor Spc72 and the γ-TuSC. However, Tub4 activity is important to direct cMT nucleation to the SPB.

The in vitro analysis (Figures 1–3) has shown the ability of Stu2 to nucleate MTs even without γ-TuSC. Thus, Stu2 could be the nucleating factor that promotes cMT formation in cells with strongly reduced Tub4 levels. To assess this possibility, we asked whether the cMTs in Tub4-depleted cells require Stu2 for formation using the assay described in Figure 7a and whether Stu2 associates with detached cMTs in TUB4–AID cells. As hypothesized, cells with double depletion of Tub4 and Stu2 (TUB4–AID STU2–AID cells) failed to assemble cMTs (Figure 7b and Figure 7—figure supplement 1b). In addition, Stu2 localization analysis indicated that 51% of the free cMTs in TUB4–AID cells carried a strong enrichment of Stu2–mCherry at one end (Figure 7c, left). Frequently, this was the end in the schmoo tip region. The other detached cMTs (49%) were decorated with Stu2–mCherry. This evidence raises the possibility of a function of Stu2 in the assembly of cMTs when Tub4 levels are low.

We then asked whether Stu2 is also important for cMT nucleation in cooperation with γ-TuSC. To test this notion, we analysed the impact of Stu2–AID depletion on the nucleation of cMTs in TUB4 cells using the assay described in Figure 7a. IAA depleted the Stu2–AID protein below the critical threshold that is needed for viability (Figure 7—figure supplement 1a and b). Stu2 depletion dramatically impaired the formation of cMTs without affecting the assembly of nuclear MTs (Figure 7b). This phenotype was complemented by an integrated WT STU2 construct (Figure 7e). Thus, Stu2 is important for cMT nucleation in vivo in the presence of γ-TuSC.

Finally, we tested the role of Stu2 domains (Figure 2a) on cMT assembly in vivo. STU2 WT and mutant versions were expressed in STU2–AID cells. Upon Stu2–AID depletion, stu2^TOGAA was expressed as WT STU2 (Figure 7—figure supplement 1c). The expression of stu2^∆MT and stu2^∆C was, in fact, slightly higher than that of WT STU2. stu2^∆CC showed lower expression levels compared to STU2. STU2–AID STU2 cells nucleated SPB-associated cMTs after nocodazole wash out (Figure 7e) as efficiently as WT STU2 cells (Figure 7b, WT). These cMTs were ~1.8 µm long and connected the SPB with the schmoo tip (Figure 7e and f). By contrast, most stu2^TOGAA and stu2^∆CC cells were impaired in cMT formation (Figure 7e). Only about 20% of stu2^TOGAA and stu2^∆CC cells re-assembled cMTs, which were shorter and much less robust than cMTs in STU2–AID STU2 cells (Figure 7e and f). About half of the stu2^∆MT and stu2^∆C cells assembled cMTs that were shorter than those of STU2 WT cells. The other half of stu2^∆MT and stu2^∆C cells was devoid of cMTs (Figure 7e, quantification). Whenever STU2 mutant cells assembled cMTs, these were associated with the SPB (Figure 7e, top). Thus, the TOG domains and the dimerizing coiled-coil domain of Stu2 were most important for cMT formation in the presence of γ-TuSC. Stu2^MT had an important impact on cMT formation.

Taken together, our experiments indicate two in vivo functions for Stu2. (1) Stu2 is important for stabilization of the γ-TuSC oligomer at the minus end of detached cMTs (Figure 6). (2) Stu2 is crucial for the nucleation of cMTs independently of the presence of γ-TuSC (Figure 7).

Most yeast strains that were used in this study are derivatives of ESM356-1 (MATa ura3-52 trp1Δ63 his3Δ200 leu2Δ1) and are listed in Supplementary file 1. Supplementary file 2 lists the plasmids used in this study. Genes were deleted or tagged endogenously using PCR-based methods (Janke et al., 2004; Knop et al., 1999). Tagging was verified by PCR, microscopy and immunoblotting. Plasmids with the backbone of pRS304, pRS305 and pRS306 (Sikorski and Hieter, 1989) were linearized and stably integrated into the yeast genome by homologous recombination. For the G₁ arrest, cells were treated with 10 μg/ml α-factor. For nocodazole arrest in SC-complete medium, cells were incubated with 1% peptone and 15 µg/ml nocodazole. For auxin-depletion experiments, proteins were tagged with 3HA-IAA and depleted with an IAA (3-Indoleacetic acid, Sigma-Aldrich I2886) concentration of 1 mM at 30°C. For drop tests, cells derived from S288C (YPH499; Sikorski and Hieter, 1989) were serially diluted 1:10 and spotted on either SC-Leu or 5-FOA plates. Plates were incubated at 30°C for 2 d or 5 d. We used alkaline lysis and TCA to prepare protein extracts from yeast cells (Knop et al., 1999).

Antibodies were mouse anti-GFP (1:1000; Roche 11814460001), rabbit anti-GFP (1:2000; homemade rabbit BS 23.4.08), goat anti-GST (1:2000; GE Healthcare 27-4577-01), mouse anti-HA (1:50; 12CA5), rabbit anti-Spc97 (1:500; homemade rabbit AT), rabbit anti-Stu2 (1:200; homemade), goat anti-Tub4 (1:250; homemade), rabbit anti-Spc72 (1:300; homemade) and mouse anti-tubulin (1:100; homemade WA3 antibodies). Secondary antibodies were donkey anti-rabbit IRDye 800CW (1:10,000; LI-COR Product-number: 926–32213), donkey anti-goat A680 (1:10,000; Invitrogen, A21084), donkey anti-mouse A680 (1:10,000; Invitrogen, A10038), goat anti-mouse HRP (1:10,000; Jackson 115-035-068), rabbit anti-goat HRP (1:5,000; Jackson 305-035-045), donkey anti-rabbit HRP (1:5,000; Jackson 711-035-152) and goat anti-rabbit HRP (1:10,000; Jackson 111-035-045).

Microscopy was performed in sterile filtered synthetic complete (SC) medium at 30°C. Log-phase cells were treated as annotated and immobilized on a glass bottom dish (P35G-1.5–14C; MatTek Corporation). In advance, the dish was coated with 100 μl of ConA (6% Concanavalin A type IV, 25 mM Tris-HCl pH 7, 1 mM MnCl₂) for 2 min and then washed twice with water. Cells were allowed to attach for 5 to 15 min, subsequently washed with water, and finally SC medium was added. For imaging, a DeltaVision RT system (Olympus IX71 based; Applied Precision Ltd.) equipped with a Photometrics CoolSnap HQ camera (Roper Scientific), a 100 × 1.4 NA Super–Plan Apochromat oil objective (Olympus), a four-color Standard InsightSSI module light source including a laser-based hardware autofocus, and a Workstation with a CentOS operating system and SoftWoRx software (Applied Precision Ltd.) was used. For photobleaching experiments, a 50 mW 488 nm laser system was used on the same microscope. For deconvolution of images, the softWoRx software package of DeltaVision was used. For live-cell imaging, the system was prewarmed to 30°C and imaging was done with binning 2 × 2. Image analysis was performed with ImageJ 1.46 r (National Institutes of Health, USA) and GraphPad Prism (GraphPad Software).

For line scans of detached cMTs of kar1Δ15 cells both wavelengths were acquired for each z-stack, followed by the next stack. After deconvolution of the images, MTs from single z-planes were analysed in ImageJ by drawing a line along the MT, and signal intensities were measured with the plot profile command. Signal normalization was performed against the highest signal intensity of the measured signal in Excel (Microsoft).

For measuring molecule numbers of proteins tagged with yeGFP, kar1Δ15 cells and CSE4-yeGFP Δste2 cells were α-factor treated and mixed. First, all 21 stacks of the yeGFP wavelength were acquired followed by all stacks of the second fluorescence signal in order to localize the yeGFP signal on the detached cMT. A reference image of an empty Matek dish was acquired with the imaging buffer and the same acquisition settings to correct for variations of the field illumination in the GFP-channel. After subtracting the reference image from all the GFP-stacks, the brightest signal intensity from single z-planes of the 21 stacks was analysed in ImageJ and corrected for the background close to the measured signal as published (Erlemann et al., 2012).

For FRAP experiments examining kar1Δ15 cells with a yeGFP-tag on the protein of interest, the yeGFP signal was first focused in the z-plane. Three pre-bleach images were taken, followed by 50 images after photobleaching, for an expected signal recovery halftime of 1 s. Photobleaching was performed with a 100x objective and a 488 nm laser with the power of 12% for Stu2 and 17% for Spc72 for 50 msec. Normalization of the FRAP data was performed as described by Erlemann et al. (2012) with the GraphPad Prism plotting function with some changes. Fluorescence intensities of the yeGFP-tagged proteins were measured and normalized using the Phair double-normalization method (Phair et al., 2004), setting the fluorescence intensity at the moment of bleaching to 0. A curve reflecting the total mean of the fluorescence recovery was corrected for overall bleaching by measuring the fluorescence intensity decrease of a neighbouring cell with the formula y=(y₀–Plateau)*e^(–Kd*x)+Plateau (One-phase decay in GraphPad Prism). The constant K_d was extracted from the control measurement and the recovery curve was calculated with y=y₀+(Plateau–y₀)*(1-e^–(K+Kd)x) (as in One-phase association in GraphPad Prism). The half-time was extracted from that curve with ln(2)/K.

The γ-TuSC was purified as described by Gombos et al. (2013).

The purification protocol for 6His-Stu2 and its mutant versions is a variation of the published protocols (Al-Bassam et al., 2006; van Breugel et al., 2003). 6His-Stu2 proteins were expressed in SF21 insect cells after infection for 48 hr with 1% baculovirus. Cells were harvested by centrifugation at 2000 rpm for 10 min and stored at −80°C. The pellet from 800 ml culture was resuspended in HB200 (50 mM Hepes, pH 7.5, 200 mM KCl, 1 mM MgCl₂, 5% glycerol[(w/v]) together with one tablet of Protease Inhibitor Cocktail (Roche, 11873580001) and 1 mM DTT. Cells were lysed on ice with a Polytron (Polytron PT 3100 dispersion unit, Kinematica) for 5 min at 4000 rpm. The lysate was incubated with 0.25% Brij35 for 10 min at 4°C and centrifuged at 4°C for 30 min at 15,000 rpm in a SS-34 rotor. The supernatant was bound to 500 mg equilibrated Ni-beads (Protino Ni-TED; Machery-Nagel) for 2 hr at 4°C. Beads were washed four times with HB200, and proteins were eluted in 500 mM imidazole. The eluate was injected into an ÄKTA system (GE Healthcare), which was equilibrated with HB200 and purified through size exclusion chromatography (HiLoad 16/60 Superdex 200 column, GE Healthcare) at 4°C. The fractions were analysed by SDS-PAGE and those containing Stu2 were pooled, concentrated and stored at −80°C. The bar graphs were designed with DOG1.0 (Ren et al., 2009).

The purification of GST–Spc72N followed a variation of the protocol published by Lin et al. (2014). A preculture of Escherichia coli BL21-CodonPlus was incubated at 37°C in LB-Amp-Cam (100 μg/ml Ampicillin, 30 μg/ml Chloramphenicol) overnight, diluted to OD₆₀₀ 0.2 in LB-Amp-Cam and incubated at 22°C for 1 hr at 100 rpm. Induction was carried with 200 µM IPTG for 20 hr at 22°C. Cell pellets of 1 l culture were harvested by centrifugation at 3000 g for 15 min and stored at −80°C. The pellet was resuspended in lysis buffer (40 mM K-Hepes pH 7.5, 250 mM KCl, 10 mM EDTA, 1 mM EGTA, 10% glycerol [w/v], 4 mM DTT) together with one tablet of Protease Inhibitor Cocktail and 1 mM PMSF. Cells were lysed on ice by sonication (Bandelin Sonopuls GM 200 equipped with a Bandelin electronic UW200) with a KE76 tip five times for 30 s with 50% power. The lysate was centrifuged for 30 min at 4°C at 26,890 g in a SS-34 rotor. The supernatant was incubated with 750 μl equilibrated GST-beads (Protino Gluathione Agarose 4B; Machery-Nagel) for 2 hr at 4°C. The beads were washed three times with lysis buffer and the protein was eluted with 30 mM L-glutathione in lysis buffer. The eluate was injected into an ÄKTA system (GE Healthcare) and purified through size-exclusion chromatography (HiLoad 16/60 Superdex 200 column, GE Healthcare) at 4°C. The chromatography was done with TB150 (50 mM Tris-HCl pH7.0, 150 mM KCl, 1 mM MgCl₂, 1 mM EDTA). The fractions were analysed by SDS-PAGE and those containing Spc72 were pooled, concentrated and stored with 10% glycerol at −80°C.

An E. coli pellet of 1 l from GST–Spc72N-expressing cells was resuspended in HB200 together with one tablet of Protease Inhibitor Cocktail and 1 mM DTT. Lysis and centrifugation were carried out as for Spc72 purification. The supernatant containing GST–Spc72N was bound to equilibrated GST-beads for 2.5 hr at 4°C. Meanwhile, a pellet of 800 ml SF21 insect cells expressing 6His–Stu2 was resuspended in HB200 together with one tablet of Protease Inhibitor Cocktail and 1 mM DTT. Cells were lysed with the Polytron, 0.25% Brij35 was added for 10 min and the lysate was centrifuged as mentioned in Stu2 purification. The GST–Spc72N beads were washed five times with HB200 and the 6His–Stu2 lysate was added after dilution with HB200 containing 0.125% Brij35. After incubation overnight at 4°C, the beads were washed five times with HB200 containing 0.125% Brij35 and proteins were eluted with 50 mM L-glutathione in HB200 with 0.125% Brij35. The elutions were loaded on an ÄKTA system (GE Healthcare) with an HiLoad 16/60 Superdex 200 column (GE Healthcare), which was equilibrated with HB200 at 4°C. Gel filtration fractions were analysed by SDS-PAGE and those containing GST–Spc72N and 6His–Stu2 were pooled. The purified complexes were stored at −80°C with 0.125% Brij and 5% glycerol.

Purification of the N-terminal version of Spc110N (GST–Spc110N^1-220) and its mutant version Spc110N^CM1 (GST–Spc110^1-220-QA) were performed as described by Lin et al. (2014).

The pulldown protocol is a variation of a protocol published by Lin et al. (2014). Recombinant proteins (see purification of proteins) were pre-cleared by centrifugation at 20,817 g at 4°C. 6His–Stu2 and γ-TuSC proteins were diluted with HB100 (40 mM Hepes pH 7.5, 100 mM KCl, 1 mM EGTA, 1 mM MgCl₂) and incubated with GST-beads for 30 min on ice. The supernatant was mixed with GST or GST–Spc72N to a final concentration of 2 μM for Stu2, 150 nM for γ-TuSC, 1 μM for GST and 1 μM for GST–Spc72N. The GST–Stu2^TOG (aa 1–590 of Stu2) and GST–Stu2^MT (aa 451–684 of Stu2) were purified as described previously (Widlund et al., 2012). Pig brain tubulin and γ-TuSC were diluted with HB100 and incubated with glutathion beads for 30 min on ice. The supernatant was mixed with GST, GST–Stu2^TOG or GST–Stu2^MT to a final concentration of 500 nM for tubulin or γ-TuSC and 1 μM for GST, GST–Stu2^TOG or GST–Stu2^MT. After an incubation for 30 min, the protein mixture was incubated at 4°C for 1 hr with equilibrated glutathion beads. Beads were washed once with washing buffer (pulldown buffer with 0.1% Nonidet P40; Biochemica) and transferred to a new tube. Beads were washed six times and the remaining buffer was removed with a squeezed pipette tip. Samples were incubated with sample buffer at 65°C for 5 min and analysed by immunoblotting.

Pig brain tubulin was diluted to 30 μM together with 30 μM nocodazole in BRB80 (80 mM PIPES, pH 6.8, 1 mM MgCl₂, 1 mM EGTA), precleared by centrifugation in a S100AT3 rotor at 4°C for 5 min at 353,000 g, and half of the supernatant was incubated with Ni-beads (Qiagen) equilibrated with HB300 (50 mM K-Hepes, pH 7.5, 300 mM NaCl, 1 mM MgCl₂, 5% glycerol) for 30 min at 4°C. The tubulin supernatant was taken without transferring any beads. 2 μM of Stu2 proteins (which were pre-cleared by centrifugation at 20,817 g at 4°C) were incubated together with 2 μM tubulin from the supernatant on equilibrated Ni-beads in HB300 for 1 hr at 4°C. Beads were washed once with HB300 supplemented with 0.5% Nonidet P40 (Biochemica) and 20 mM imidazole, and transferred to a new tube. Then beads were washed two more times and the remaining buffer was removed with a squeezed pipette tip. Beads were treated with sample buffer at 65°C for 5 min and the supernatant was analysed by immunoblotting.

Pig brain tubulin was diluted with BRB80 12.5% glycerol (w/v), centrifuged at 4°C for 5 min at 353,000 g in a S100AT3 rotor, and half of the supernatant was used for the experiments. Stu2 (which was pre-cleared by centrifugation at 20,817 g at 4°C) and tubulin were diluted together to 5 μM in HB100 supplemented with 10% glycerol and incubated for 40 min on ice. Size-exclusion chromatography was performed with a Superose six column (10/300 GL, GE Healthcare) on an ÄKTA system (GE Healthcare). Fractions were treated with sample buffer and analysed by immunoblotting.

For in vitro nucleation of MTs, unlabelled and Cy3-labelled (following protocol by Hyman et al. (1991)) pig brain tubulin was melted by hand, diluted to 40 μM in BRB80 with 12.5% glycerol and centrifuged in a S100AT3 rotor at 4°C for 5 min at 353,000 g. The upper half of the supernatant was adjusted to 24 µM. Proteins were mixed and incubated for 1 hr in BRB80 with 12.5% glycerol and 1 mM GTP on ice. 2.5 μl of protein mixture was mixed with 2.5 μl tubulin (final tubulin concentration 12 µM) and incubated for 10 min on ice. The following concentrations were used: 50 nM for γ-TuSC and 100 nM for Stu2, Spc72N or the purified Spc72N–Stu2 complexes. Each assay was incubated at 37°C for 16 min and 20 µl of 1% glutaraldehyde was added with a cut pipette tip. After 7 min 30 s incubation at 23°C, 400 μl of cold BRB80 was added and the tube was inverted for mixing. Coated coverslips (15 min of Poly-L-lysine [Sigma-Aldrich P8920]) were added on top of adaptors for Corex tubes (15 ml, No 8441) and supplied with 5 ml of BRB80 in 10% glycerol. An assay volume of 50 μl was added just underneath the liquid cushion and spun at 25,530 g, at 4°C for 1 hr in a HB6 rotor. Coverslips were fixed with ice-cold methanol and washed twice with cold PBS. Drops of Citifluor fixed the coverslips on objective slides, which were finally sealed with nail polish. Twenty images were acquired for the asters with a 63x objective and for the MTs with a 100x objective on a Zeiss Axiovert 200M equipped with a Cascade 1 k EMCCD camera (Cascade Photometrics, Roper Scientific, Inc.) and with a 63 × 1.4 NA Plan Apochromat oil objective (Zeiss) and a 100 × 1.46 NA Plan Apochromat oil objective (Zeiss), a HBO100 lamp and a Ludl MAC 5000 (Ludl Electronic Products Ltd.) with FWSHCDC controlling a DIC/488/555/647 filter wheel. The system was managed with the software VisiView (Version 2.1.4, Visitron Systems GmbH). Analysis was performed with ImageJ and the aster number was corrected by the mean number of nucleated MTs in 20 fields of the tubulin-only control taken with a 100x objective. The MT formation activity was derived by a measurement of the mean intensity of the maximum projection of 20 acquired images. The tubulin-only control intensity was subtracted from other values to correct for the background.

Purified γ-TuSC was mixed with GST–Spc72N^CM1 or GST–Spc110N complex in 1:4 molar ratio (4.6 µM:18.6 µM) in HB100-50 buffer (50 mM Hepes, pH7.5, 100 mM KCl, 1 mM EGTA, 1 mM MgCl₂) with salt as indicated in the figure legends. After incubating for 15 min at 4°C, the protein mixture was applied to a gel filtration column (Superose 6 PC 3.2/30, GE Healthcare, UK). Elution profiles were recorded at absorbance at 280 nm. Proteins were detected by Coomassie Blue or immunoblotting. For Figure 2e and Figure 2—figure supplement 2d, purified γ-TuSC was mixed with GST–Spc72N, GST–Spc72N–6His–Stu2^WT or GST–Spc72N–6His–Stu2^TOGAA to a final concentration of 4.6 µM for γ-TuSC and 2.3 µM for the other proteins in HB100 buffer with 10% glycerol. Proteins were incubated on ice for 40 min, centrifuged at 20,817 g for 10 min at 4°C and 50 µl were loaded on a gel filtration column (Superose 6 PC 3.2/30) equilibrated with HB100. Proteins were detected by immunoblotting. Electron microscopy analysis was performed as described by Lin et al., 2016. A High Molecular Weight (HMW) Kit (GE Healthcare, 28-4038-42) was used for calibration of the Superose 6 PC 3.2/30 column.

MST assays were carried out with a Monolith NT.115 instrument (NanoTemper, Munich, Germany). Each titration curve consisted of 16 points prepared from a serial dilution of analytes and a constant concentration of the fluorescein-labelled ligand. Purified γ-TuSC and Stu2 were fluorescently labelled with GREEN-NHS (NanoTemper, Munich, Germany). To measure the affinity between γ-TuSC and its binding partners, 2X serial diluted recombinant Spc110N, Spc72N, Stu2 or Spc72N-Stu2 complexes were titrated against 50 nM of labelled γ-TuSC. To measure the binding affinity between Stu2 and Spc72N, increasing concentrations of recombinant Spc72N were titrated against 150 nM of labelled Stu2. Experiments were carried out in HB100-50 buffer supplemented with 0.05% (w/v) Tween-20. The samples were loaded into standard glass capillaries (Monolith NT capillaries, NanoTemper, Munich, Germany). MST assays were performed with 60% and 80% LED power using a green filter and 40%, 60% and 80% MST power. The normalized fluorescence readings (Thermophoresis + T jump or T-jump only) were plotted as a function of analyte concentration and the curve fitting and dissociation constant K_d calculation were performed with Nanotemper software. In all cases, MST data were fitted on the based of a single-site model.

Statistical analysis of the data was carried out with GraphPad Prism and performed as two-tailed unpaired t-tests with a confidence interval of 95%. For MST measurements, the statistical analysis was done in Excel. The number of repeated experiments is indicated in the figure legend together with the sample size and the P-values. In the MST measurements, when the data points of a single concentration value were deviated from normal intensity range, they were considered as outliers and excluded from the analysis. Otherwise no data points were excluded. Experiments are technical replicates if not stated differently. The experiments were not randomized and the investigators were not blinded to allocation during the experiments and outcome assessment.

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

The authors thank Dr. M Mayer (ZMBH) for the use of the MST equipment. JG is a member of the Hartmut Hoffmann-Berling International Graduate School.

1. Received: July 10, 2018
2. Accepted: September 14, 2018
3. Accepted Manuscript published: September 17, 2018 (version 1)
4. Version of Record published: September 26, 2018 (version 2)

© 2018, Gunzelmann et al.

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