Puf6 primes 60S pre-ribosome nuclear export at low temperature

Gerhardy, Stefan; Oborská-Oplová, Michaela; Gillet, Ludovic; Börner, Richard; van Nues, Rob; Leitner, Alexander; Michel, Erich; Petkowski, Janusz J.; Granneman, Sander; Sigel, Roland K. O.; Aebersold, Ruedi; Panse, Vikram Govind

doi:10.1038/s41467-021-24964-2

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Published: 04 August 2021

Puf6 primes 60S pre-ribosome nuclear export at low temperature

Nature Communications volume 12, Article number: 4696 (2021) Cite this article

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Abstract

Productive ribosomal RNA (rRNA) compaction during ribosome assembly necessitates establishing correct tertiary contacts between distant secondary structure elements. Here, we quantify the response of the yeast proteome to low temperature (LT), a condition where aberrant mis-paired RNA folding intermediates accumulate. We show that, at LT, yeast cells globally boost production of their ribosome assembly machinery. We find that the LT-induced assembly factor, Puf6, binds to the nascent catalytic RNA-rich subunit interface within the 60S pre-ribosome, at a site that eventually loads the nuclear export apparatus. Ensemble Förster resonance energy transfer studies show that Puf6 mimics the role of Mg²⁺ to usher a unique long-range tertiary contact to compact rRNA. At LT, puf6 mutants accumulate 60S pre-ribosomes in the nucleus, thus unveiling Puf6-mediated rRNA compaction as a critical temperature-regulated rescue mechanism that counters rRNA misfolding to prime export competence.

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Introduction

Most RNAs exert their function after folding into their native 3D structures. However, intramolecular sequence complementarities make RNA-folding processes promiscuous, thus delaying the acquisition of functionality. Low temperature exacerbates RNA-misfolding due to thermodynamic stabilization of trapped non-native states. To overcome these barriers, cells deploy RNA-chaperones and RNA-helicases that prevent and/or resolve aberrant RNA folding intermediates¹.

The ribosome is one of the most abundant RNA:protein complexes assembled by incorporating ribosomal proteins (r-proteins) into dynamically folding ribosomal RNA (rRNA). In eukaryotes, the large 60S subunit contains three rRNAs (25S, 5.8S, 5S) and 46 r-proteins, whereas the small 40S subunit contains a single rRNA (18) and 33 r-proteins². Eukaryotic ribosome assembly is initiated co-transcriptionally in the nucleolus by RNA polymerase-I driven transcription of rDNA repeats. The emerging pre-rRNA associates with U3 snoRNP, 40S-specific r-proteins, and ~100 assembly factors to form the small subunit precursor³. Cryogenic electron microscopy (cryo-EM) studies suggest that assembly factors and U3 snoRNP encapsulate and guide hierarchical 5′-to-3′-oriented pre-rRNA folding⁴. Following endonucleolytic cleavage and release of the 40S pre-ribosome, the growing 27S pre-rRNA associates with 60S-specific r-proteins and assembly factors to concomitantly fold rRNA domains (I to VI) to form the 60S pre-ribosome. Cryo-EM studies have revealed that the 5′ rRNA domains I and II within 27S pre-rRNA fold to a near-mature conformation and interact with the 3′ terminal rRNA domain VI, to form the characteristic arch-like solvent-exposed backside of the 60S subunit⁵. The internal transcribed spacer 2 (ITS2) located between 5.8S and 25S rRNA within 27S pre-rRNA and associated assembly factors forms the “foot” structure already visible in these early states. However, the central rRNA domains III, IV, and V, which form the catalytic subunit interface remain unresolved. Structural studies implicate non-linear compaction wherein the near-native rRNA domains I, II, and VI establish tertiary contacts with the flexible rRNA domains III, IV, and V^5,6. Mechanisms that drive the correct formation of these long-range contacts during 27S pre-rRNA folding remain unknown.

Establishing correct tertiary contacts within 27S pre-rRNA is critical for polypeptide exit tunnel formation, productive pre-rRNA processing of ITS2, and the incorporation/rotation of the 5S RNP^5,6. These interactions stabilize the rRNA-rich subunit interface and provide a binding platform for the GTPase Nog2, and the assembly factor Sda1 which recruits the Rix1-Ipi-complex and the AAA-ATPase Rea1 to the 60S pre-ribosome^7,8. The coordinated release of Rea1, the Rix1-Ipi-complex, and Nog2 functions as a checkpoint that prevents premature recruitment of the export adaptor Nmd3 for Crm1-mediated transport into the cytoplasm⁹.

Nucleolar ribosome biogenesis steps require coordinated rearrangements of RNA:RNA and RNA:protein interactions that enable hierarchical RNA folding, and incorporation of assembly factors and r-proteins¹⁰. The multitude of possible intramolecular base-pairings and the increased stability of mispaired structural elements pose a formidable barrier for correct pre-rRNA folding, especially at low temperatures^11,12,13. Here, we measured how the yeast proteome adapts to low temperatures (LT). We found that yeast cells boost assembly factor production at LT. We show that the 60S assembly factor, Puf6, is induced at LT to usher a non-canonical tertiary contact between distant secondary structure elements within the catalytic rRNA-rich subunit interface important for recruiting the nuclear export machinery. Our findings provide insights into how Puf6-mediated rRNA compaction at LT primes 60S pre-ribosome nuclear export.

Results

Yeast cells boost the production of ribosome assembly factors at low temperature

To compare proteomes of yeast cells grown at different temperatures, we employed sequential window acquisition of all theoretical fragment ion spectra (SWATH) mass spectrometry (MS)¹⁴. SWATH-MS is an effective approach that has reliably quantified proteomes of diverse model organisms, and tissues from disease states¹⁵.

We subjected lysates derived from WT yeast cells grown at 20, 25, 30, and 37 °C in rich media to SWATH-MS (Fig. 1a). A total of 2821 proteins were detected and their relative abundances at different temperatures were quantified. By employing hierarchical clustering algorithms, we grouped the proteome profiles of individual proteins that showed a more than 1.5-fold change in levels across the different temperatures. Based on these analyses, 426 proteins were organized into nine mutually exclusive clusters (Fig. 1b). We characterized the individual members within each cluster based on their functional GO terminology using the pathway enrichment analysis tool DAVID (Supplementary Data 1; http://david.abcc.ncifcrf.gov/)¹⁶. Components of clusters 5–8 showed increased protein abundance levels with increasing temperatures. These clusters enriched 15 heat shock proteins (HSPs) including members of the HSP70 and the HSP90 families as well as small HSPs and their regulators that are involved in the cellular response to heat stress. Clusters 9 and 3 enriched proteins devoted to different aspects of cellular metabolism including oxidative phosphorylation, and purine/pyrimidine metabolism, respectively (Supplementary Data 1).

**Fig. 1: Quantifying alterations in the proteome by SWATH-MS in yeast cells grown at different temperatures.**

Factors within clusters 1, 2, and 4 showed increased levels at 20 °C (hereafter referred to as low temperature, LT), in comparison to levels at 30 °C. Strong overrepresentation of ribosome assembly factors (1.09E−09, cluster 2) and rRNA processing factors (3.97E−11, cluster 2) was observed in these clusters (Fig. 1c and Supplementary Data 1). Several identified factors are organized as sub-complexes that scaffold pre-rRNA on maturing pre-ribosomes (Supplementary Figs. 2 and 3). For example, the A₃ factors, Nop15, Cic1, Rlp7, Nop7, and N-terminus of Erb1 (Fig. 1c, left panel and Supplementary Fig. 2, in yellow) stabilize ITS2 within the 27S pre-rRNA during 60S assembly^5,6,17. These factors are essential for ITS2 processing and form the “foot structure”, a structural landmark on early 60S pre-ribosomes^17,18. Similarly, the ribosomal-like protein Mrt4 (Fig. 1c, left panel and Supplementary Fig. 3, light green), which scaffolds folding of the rRNA base of the P-stalk during nuclear maturation, and its cytoplasmic release factor Yvh1^19,20 showed increased abundance at LT. Rpf2 and the AAA-ATPase Rea1 (Fig. 1c, left panel and Supplementary Fig. 2, red) were induced at LT; Rpf2 and Rea1 are involved in the process of 5S RNP docking and rotation on the pre-ribosome and maturation of the central protuberance, another structural landmark of the 60S subunit^7,21. Interestingly, several r-proteins located on the solvent-exposed side of the 60S subunit were induced at LT (Fig. 1c, right panel, purple). Finally, several assembly factors (Fig. 1c, left panel, orange and dark red) whose location on maturing pre-ribosomes remain unknown were induced at LT. A (post-hoc) t-test of the protein abundances between 37 °C and 20 °C confirmed that 43 out of the 54 identified assembly factors and r-proteins showed a significant increase in abundance (adjusted p-value < 0.05) with a median fold change of 2.5. We conclude that yeast cells globally boost the production of ribosome assembly factors and r-proteins at LT.

Puf6 induction at LT ensures efficient 60S pre-ribosome export

Cryo-EM studies are pinpointing the RNA-binding sites of assembly factors on 60S pre-ribosomes. Yet, the locations of several factors especially those associated with rRNA domains III, IV, and V during early nucleolar maturation remain unknown^8,22. One such factor is Puf6, which we found to be induced at LT (Fig. 1c, left panel, orange bar). In agreement with the SWATH-MS data, Western analyses showed a significant increase in Puf6 protein levels when yeast cells were grown at 20 °C, as compared to 37 °C (Fig. 2a). Puf6 protein levels were induced when yeast cells growing at 37 °C were shifted to 20 °C. Conversely, Puf6 protein levels decreased when yeast cells growing at 20 °C were shifted to 37 °C (Fig. 2b).

**Fig. 2: Puf6 is required for 60S pre-ribosome export at LT.**

Puf6 is a conserved assembly factor that contains an atypical Pumilio repeat RNA-binding domain^23,24,25. Puf6-deficient yeast cells accumulate 27S and 7S pre-rRNA and exhibit reduced levels of 60S subunits at 20 °C²³. Puf6 has been implicated in the loading of the r-protein eL43 during 60S assembly^26,27. We initiated functional studies by disrupting the endogenous PUF6 gene encoded by the open reading frame in WT diploid yeast cells. Tetrad analysis yielded two spores with WT growth rates and two spores with a slow-growth phenotype at 25 °C, which carry the PUF6 deletion (puf6∆). In agreement with previous studies²³, we found that growth of the puf6Δ mutant is impaired at 20 and 25 °C, as determined by the size of single colonies. At 30 and 37 °C, the puf6Δ mutant grew nearly like WT cells (Fig. 2c). Next, we examined the localization of 40S and 60S subunits in the puf6Δ mutant at 20 and 30 °C. At 20 and 30 °C, WT cells showed cytoplasmic localization for both 40S and 60S subunit reporters, uS5-GFP and uL18-GFP, respectively. In contrast, puf6Δ cells revealed a nuclear accumulation of uL18-GFP at 20 °C, but not at 30 °C. Localization of the uS5-GFP remained unaffected in puf6∆ cells at 20 and 30 °C (Fig. 2d). Thus, the slow growth of the puf6Δ mutant at 20 °C correlates with impaired 60S pre-ribosome export. Impaired growth of the puf6Δ mutant at 20 °C, and increased Puf6 protein levels in WT cells at 20 °C point to a requirement of Puf6 during 60S assembly at LT. Expression of the human ortholog, Pum3 (also known as Puf-A or KIA0020), rescued the slow growth and 60S pre-ribosome export defect of the puf6Δ mutant at 20 °C, indicating a conserved role during 60S assembly (Fig. 2c, d).

Puf6 co-enriches with early nucleolar 60S pre-ribosomes

Previous studies have suggested a role for Puf6 in the localization and translational repression of specific mRNAs^28,29,30. However, in agreement with cell-biological studies^26,31, we found that Puf6-GFP predominantly co-localizes with Gar1-mCherry, an established nucleolar marker (Fig. 3a). To test whether Puf6 shuttles between the nucleus and cytoplasm, we employed the established heterokaryon assay³². A strain expressing a Puf6-GFP was mated with a kar1-1 expressing strain, in which mating and cell conjugation are not followed by nuclear fusion, leading to heterokaryon formation. In order to distinguish the two nuclei in the resulting heterokaryon, the nuclear pore protein Nup82 was tagged with mCherry in the kar1‐1 strain. As controls, we used the shuttling Arx1-GFP and non‐shuttling Gar1–GFP strains, respectively. While Arx1-GFP localized to both nuclei after mating, Puf6-GFP and Gar1–GFP were never observed in the nucleus of the kar1‐1 strain (Fig. 3b). While these data are consistent with an exclusively nuclear location of Puf6 in vivo, a small undetectable cytoplasmic fraction of Puf6 may repress translation.

**Fig. 3: Puf6 is enriched in the nucleolus and associates with early 60S pre-ribosomes.**

We investigated the maturation stage at which Puf6 is recruited to and released from the 60S pre-ribosome³³. For this, we purified 60S pre-ribosomes at distinct maturation stages using different TAP-tagged bait proteins: Ssf1‐TAP purifies an early nucleolar 60S pre-ribosome; Rix1‐TAP purifies a nucleoplasmic 60S pre-ribosome; Arx1‐TAP purifies a late export competent 60S pre-ribosome; and Kre35‐TAP purifies an exclusively cytoplasmic 60S pre-ribosome. Western analyses revealed that Puf6 co-enriches mainly with the nucleolar Ssf1-TAP particle and to a lesser extent with the nucleoplasmic Rix1-TAP. Puf6 did not co-enrich with Arx1-TAP and Kre35-TAP (Fig. 3c). Consistent with this, we found that the Puf6‐TAP co-enriched assembly factors such as Rrp5, Noc1, Rrp1, Urb1, Mak11, etc. that co-enrich with nucleolar 60S pre-ribosomes (Fig. 3d). We suggest that Puf6 exerts its function during early nucleolar 60S assembly.

The Pumilio repeat domain recruits Puf6 to the 60S pre-ribosome

Puf6 belongs to the Pumilio and fem3 mRNA-binding factor (PUF) family, a large eukaryotic family of RNA-binding proteins. However, within the seven members of the yeast PUF family, Puf6 is the most diverged member³⁴ and exhibits a different domain organization (Fig. 4a). In addition to the C-terminal RNA-binding PUF repeats, the human ortholog Pum3/Puf-A contains an N-terminal extension with three additional PUF repeats³⁵, which are also found in yeast Puf6 (Fig. 4a). Homology modeling and small-angle X-ray scattering (SAXS) indicated the Puf6 structure resembles the L-shaped conformation Puf-A³⁵. Using Pum3/Puf-A (PDB 4WZW) as a template, we generated homology models for yeast Puf6 (residues 118–654) that permitted structure-guided studies (Fig. 4b). We substituted several residues in Puf6 to glutamic acid to induce repulsion with the phosphate backbone of the RNA substrate, and impair Puf6:RNA interactions (Supplementary Fig. 4b, c, d). R172 and Y208 are part of a basic patch shown to be critical for correct 7S pre-rRNA processing and localization of ASH1 mRNA³⁵ and correspond to R181, N217, and K440 in human Pum3 respectively (Fig. 4c). While single mutants showed a minor growth defect at 20 °C (Supplementary Fig. 4b), mutants in repeat 1 (R172E) or repeat 2 (Y208E) when combined with the repeat 5 (R431E) induced a strong growth impairment (Fig. 4d). Like the puf6∆ strain, the puf6 ^{R172E R431E} and puf6 ^{Y208E R431E} mutants accumulated uL18-GFP in the nucleus at 20 and 25 °C, but not at 30 and 37 °C (Fig. 4d, e). Both mutant proteins did not co-enrich with 60S pre-ribosomes (Fig. 4f). This was not due to altered stability and/or localization as Western analyses of whole-cell extracts (WCE), and fluorescence microscopy, revealed that their protein levels and the nucleolar signal were indistinguishable from wild-type Puf6 (Fig. 4f, WCE lower panel, g). We conclude that the PUF repeats target Puf6 to the 60S pre-ribosome.

**Fig. 4: The Pumilio repeat domain recruits Puf6 to 60S pre-ribosomes.**

Puf6 binds to H68 rRNA within a 60S pre-ribosome

Proteomic analyses indicated that Puf6 is co-transcriptionally recruited to rRNA domain IV within 27S pre-rRNA^36,37. However, the RNA-binding site of Puf6 on the 60S pre-ribosome remained unclear. We employed ultraviolet cross-linking and analysis of complementary cDNA (CRAC)³⁸ to localize its RNA-binding site within the 60S pre-ribosome. For this, we generated a yeast strain wherein Puf6 was fused with a C-terminal His₆-ProteinA tag at the genomic locus. In vivo cross-linked RNA:Puf6-His₆-ProteinA complexes were purified under denaturing conditions, and the recovered RNA fragments were amplified after linker ligation and cross-linked sites were mapped by deep sequencing. While specific hits were identified within the ITS2 sequence, the major Puf6 contact sites mapped to helix 66, 68, and 69 (hereafter referred to as H66, H68, and H69) within the rRNA domain IV of 25S rRNA (Fig. 5a). These secondary structure elements are present at the RNA-rich subunit interface and line the catalytic centers on the 60S subunit². During 60S assembly, H66, H68, and H69 provide a binding platform for Nog2, a placeholder for the export adaptor Nmd3 (Fig. 5a, right panel)⁹. During translation, these rRNA helices make contact with the 40S subunit and restrict the tRNA corridor at the P- and E-site.

**Fig. 5: Puf6 binds to H68 within 25S rRNA at the subunit interface.**

To validate the CRAC data, we employed yeast three-hybrid and cross-linking mass spectrometry (XL-MS). Yeast three-hybrid studies revealed a strong interaction between Puf6 and H68, but not H38, H66, or H69 present within 25S rRNA (Fig. 5b). Moreover, both PUF repeat mutant proteins, puf6 ^{R172E R431E} and puf6 ^{Y208E R431E}, that were not recruited to the 60S pre-ribosomes in vivo (Fig. 4f) did not interact with H68 as judged by yeast three-hybrid studies (Fig. 5b). Given that H68 is solvent-exposed at the rRNA-rich subunit interface, we tested whether recombinant Puf6 can bind to a mature 60S subunit. Sedimentation binding assays confirmed a robust interaction between Puf6 and a 60S subunit (Fig. 5c). Saturation of the 60S-bound assembly factor with increasing Puf6 concentrations, and a strong impairment in the binding of recombinant PUF repeat mutants to the 60S subunit confirmed the specificity of the interaction (Fig. 5c, d). We performed crosslinking-mass spectrometry (XL-MS) analyses of a reconstituted 60S:Puf6 complex using disuccinimidyl suberate (DSS) that can covalently link lysine residues that are up to 37 Å apart^39,40. These analyses revealed protein:protein cross-links between Puf6 and the r-protein uL2 (Fig. 5e and Supplementary Data 2). uL2 is located at the subunit interface of the 60S, where it contacts H66–H68 within rRNA domain IV. All identified cross-links involve lysine residues located within the N- and C-terminal extensions flanking the Puf6-Pumilio repeat domain (Fig. 5e).

The hairpin-loop of H68 contains a GAAA-tetraloop motif and engages in a non-canonical tertiary contact with a kissing loop on the mature 60S subunit. E. coli H68, however, does not form such a tertiary contact within the 50S subunit⁴¹ and does not interact with Puf6 as judged by yeast three-hybrid studies (Fig. 5f). We generated chimeric constructs between E. coli and yeast H68 to dissect the H68:Puf6 interaction by yeast three-hybrid studies. In one mutant, we swapped the hairpin-stem of yeast H68 with the hairpin-stem from E. coli H68, thus retaining the yeast H68 hairpin-loop region (H68 Tip_Sc). Conversely, we swapped the yeast H68 hairpin-loop region with the E. coli H68 hairpin-loop, thus retaining yeast H68 rRNA hairpin-stem (H68 Tip_{E. coli}; Fig. 5a). We found that Puf6 interacted with the chimeric RNA that contained the yeast H68 hairpin-loop region (Fig. 5f). These analyses are consistent with CRAC studies which revealed a major cross-link between Puf6 and U2217 located very close to the GAAA-tetraloop motif within H68 (Fig. 5a).

Based on CRAC, yeast three-hybrid, and XL-MS analyses, we suggest that Puf6 binds the 60S pre-ribosome through interactions between the Puf6-Pumilio repeat domain and the H68 hairpin-loop region.

Puf6 removal from the 60S pre-ribosome precedes Nog2 recruitment

In addition to their critical role during translation, H68 and H69 within RNA domain IV of 25S rRNA provide a binding platform for Nog2, a placeholder that prevents premature recruitment of Nmd3, until late nuclear stages of 60S assembly⁹. Given that Puf6, Nog2 and Nmd3 share a common binding site (Fig. 5a, right panel) we investigated their order of recruitment to the 60S pre-ribosome. We monitored the co-enrichment of Puf6, Nog2, and Nmd3 with 60S pre-ribosomes representing distinct maturation stages by Western blotting (Fig. 3c). Puf6 co-enriches mainly with the nucleolar Ssf1-TAP, but lower levels of Puf6 were detected on the nucleoplasmic Rix1-TAP particle (Fig. 3c). On the other hand, Nog2 is not found on the Ssf1-TAP but co-enriched only with the Rix1-TAP particle. Nog2 is hardly detected on the export competent Arx1-TAP particle (Fig. 3c). Further, we found that Nog2-TAP did not co-enrich Puf6, and conversely, Puf6-TAP did not co-enrich Nog2 (Fig. 3e). These data are consistent with the notion that Puf6 removal from the 60S pre-ribosome precedes Nog2 recruitment. We suggest that Rix1-TAP purifies a state of a 60S pre-ribosome that is loaded with Puf6, and a later state wherein Puf6 has been evicted and Nog2 has been recruited.

Puf6 promotes an unusual tertiary contact within the 60S pre-ribosome

Within a mature 60S subunit, H68 rRNA engages in a non-canonical tertiary contact at the subunit interface that is conserved in all eukaryotes (Fig. 6a)^2,42. This long-range contact involves a GAAA-tetraloop motif (TL_GAAA) within the hairpin-loop of H68 and a kissing loop (KL) formed between H22 and H88. In early nucleolar states, H22 within rRNA domain I is bound to assembly factors Ebp2 and Brx1 presumably to prevent premature KL formation (Fig. 6b, State 3, left panel)⁶. The rRNA domains IV and V that contain H68 and H88, respectively, are not fully resolved in these states (Fig. 6b)^5,6. We wondered whether Puf6 binding prevents H68 TL_GAAA to prematurely interact with the KL and/or undergo non-productive interactions with other tetraloop receptors within the pre-rRNA. To test this idea, we developed a minimal system using the tip region of H68, H88, and H22 (Fig. 6a, c and Supplementary Table 3) for Förster resonance energy transfer (FRET) experiments. KL formation between H22 and H88 (KL construct) and docking of the TL_GAAA in H68 onto the KL (KL-TL_GAAA construct) in vitro was monitored by FRET using two RNA constructs comprising the same sequence and a sCy3 donor position but differing in the position of sCy5 acceptor dyes (Fig. 6c and Supplementary Table 3). The proximity of dyes on the RNA constructs reports either KL formation (Fig. 6c, KL) or KL-TL_GAAA docking (Fig. 6c, KL-TL_GAAA). A knowledge-based structural model generated using RNA-Composer⁴³ matched well with the structure of H22, H68, and H88 ensemble within the 60S subunit with an RMSD of 1.6 Å (Fig. 6a, right panel).

**Fig. 6: Puf6 ushers rRNA tertiary contact formation.**

RNA folding is sensitive to mono- and divalent cations⁴⁴. The monovalent K⁺ shields the negatively charged phosphate backbone and facilitates RNA folding into secondary structure elements. The divalent Mg²⁺ effectively stabilizes the high charge density during the process of binding and/or docking of distant RNA structure elements. Mg²⁺ alleviates the electrostatic stress arising from closely packed phosphates to a similar extent as two K⁺ ions, but at a lower entropic cost because fewer ions are confined near the RNA^11,45,46. We found a low FRET efficiency at low K⁺ concentrations for both KL and KL-TL_GAAA reporters indicating that these structures are not populated (Fig. 6c, left panel; d, compare white bars of KL and KL-TL_GAAA). Titration with increasing K⁺ concentrations revealed a corresponding increase in FRET efficiency for KL and KL-TL_GAAA reporters (Fig. 6c, left panel; d, compare blue bars of KL and KL-TL_GAAA). A higher FRET efficiency was observed for the KL reporter as compared to the KL-TL_GAAA reporter suggesting that K⁺ supports KL formation (Fig. 6d, compare blue bars of KL and KL-TL_GAAA). Increasing Mg²⁺ concentrations boosted the FRET efficiency for the KL-TL_GAAA reporter as compared to the KL reporter supporting the idea that Mg²⁺ promotes TL_GAAA docking onto the KL in vitro (Fig. 6c, right panel; d, compare blue and green bars within KL and KL-TL_GAAA).

We evaluated the ability of the KL to function as a non-canonical receptor for TL_GAAA. For this, we replaced the KL forming H22-H88 RNA sequence with an established tetraloop receptor (TLR) that is known to bind to the TL_GAAA motif (Fig. 6c, TLR-TL_GAAA)^47,48. Titration with increasing Mg²⁺ concentrations led to a similar increase in FRET efficiency as observed for the KL-TL_GAAA reporter (Fig. 6d, compare green bars of KL-TL_GAAA and TLR-TL_GAAA). Moreover, both KL-TL_GAAA and TLR-TL_GAAA reporters exhibited similar equilibrium binding constants (K_eq,Mg(II) ~ 2 mM) for Mg²⁺ (Fig. 6c, right panel, Supplementary Tables 6–8) supporting the idea that TL_GAAA docks onto to the KL, as efficiently as a canonical TLR. We suggest that the KL functions as a receptor for H68 TL_GAAA, and the stabilization of this tertiary contact requires Mg²⁺.

We monitored the stability of the KL-TL_GAAA RNA construct by UV thermal melting in two buffers containing: (1) 100 mM K⁺, which favors KL formation, and (2) 100 mM K⁺ and 100 mM Mg²⁺, which promotes KL formation and KL-TL_GAAA docking. We found a single melting transition at 66 °C for the RNA construct in buffer conditions that favors KL formation, which we attributed to KL melting (Fig. 6e, upper panel, Supplementary Table 7). In the second condition, which promotes KL formation and KL-TL_GAAA docking, the KL melting temperature increased to 77 °C (Fig. 6e, shift arrow, Supplementary Table 7). In this profile, we observed a second melting transition at 35 °C (Fig. 6e, lower panel, Supplementary Table 7). We attribute this melting transition to the undocking of the TL_GAAA from the KL, given the significant increase in FRET efficiency observed for the KL-TL_GAAA reporter in these buffer conditions (Fig. 6c and Supplementary Fig. 5). These data support the idea that H22 and H88 form a robust KL in the presence of monovalent K⁺ ions. In contrast, the KL-TL_GAAA interaction is less stable and requires the presence of Mg²⁺.

Using the FRET reporters, we investigated the impact of the Puf6-Pumilio repeat domain (Puf6-PUM) on the formation of the KL and the KL-TL_GAAA contact in vitro. We found that Puf6-PUM did not interfere with KL formation and KL-TL_GAAA docking as judged by the increased FRET efficiency for both reporters with increasing Mg²⁺ concentrations (Fig. 6c, right panel, red circles). Surprisingly, we observed a significant increase in FRET efficiency for the KL-TL_GAAA reporter upon Puf6-PUM addition in buffer conditions that favor only KL formation (Fig. 6c, right panel, red circles; d, compare blue and red bars for KL-TL_GAAA). Puf6-PUM also promoted TL_GAAA docking onto the canonical TLR in buffer conditions that do not favor TLR-TL_GAAA interactions (Fig. 6c, right panel, red circles; d, compare blue and red bars for TLR-TL_GAAA). Thus, Puf6 can substitute the role of Mg²⁺ to promote non-canonical KL-TL_GAAA as well as canonical TLR-TL_GAAA tertiary contact formation (Fig. 6f) in vitro. An increase in FRET efficiency was observed for the KL reporter upon Puf6-PUM addition in the presence of KL promoting buffer (Fig. 6c, right panel, red circles; d, compare blue and red bars for KL). This very likely reflects further compaction of KL due to Puf6-mediated TL_GAAA docking.

Finally, we quantitated the interaction of Puf6 with H68 alone and the minimal FRET KL-TL_GAAA RNA by fluorescence anisotropy experiments (Fig. 6g). We found that Puf6 binds to isolated H68 albeit with lower affinity as compared to the KL-TL_GAAA RNA in buffer conditions promoting tertiary contact formation suggesting that, like Mg²⁺, Puf6 stabilizes the KL-TL_GAAA contact.

Puf6 primes a nucleolar 60S pre-ribosome for export

We investigated the impact of Puf6 on the 60S assembly pathway in vivo at LT. For this, we isolated Nop7-TAP from WT and puf6∆ cells grown at 20 °C. Nop7 is an ideal TAP-bait to interrogate delays in 60S assembly since it is recruited to early nucleolar 60S pre-ribosomes and remains associated until late nuclear maturation stages¹⁰. These biochemical studies showed that Sda1 recruitment to the 60S pre-ribosome was strongly impaired in the puf6∆ mutant (Fig. 7a). Cryo-EM studies of 60S pre-ribosomes showed that Sda1 binds to the base of H68 that is engaged in a KL-TL_GAAA contact (Fig. 7b). In light of these studies, we suggest that Sda1 is recruited to the 60S pre-ribosome after the KL-TL_GAAA contact has been formed (Fig. 7b).

**Fig. 7: Puf6 primes a 60S pre-ribosome for nuclear export.**

Sda1 forms part of a cluster of assembly factors (Rix1-Ipi-complex, AAA-ATPase Rea1, Rsa4, and the GTPase Nog2)⁴⁹, whose release from 60S pre-ribosomes licenses recruitment of the export machinery⁹. Sda1 has been proposed to promote the downstream recruitment of the Rix1-Ipi-complex and Rea1 to the 60S pre-ribosome^7,8. Consistent with this, we observed a significant impairment in the recruitment of the Rea1 to the Nop7-TAP particle isolated from the puf6∆ mutant (Fig. 7a). CRAC studies suggest that the Puf6 location on the 60S pre-ribosome overlaps with the binding site of Nog2 (Fig. 4a), a placeholder for the export adaptor Nmd3⁹. Western analyses revealed that Nog2 recruitment to the Nop7-TAP particle was also severely impaired in the puf6∆ mutant at LT. In view of FRET studies and the biochemical data, we infer that failure to correctly form the KL-TL_GAAA contact impairs the recruitment of checkpoint factors that license a 60S pre-ribosome for nuclear export.

Discussion

The multitude of possible intramolecular base-pairing during early pre-rRNA folding and the increased stability of mispaired RNA intermediates at LT negatively impacts ribosome assembly^13,50. We interrogated the yeast proteome by SWATH-MS to reveal how the ribosome assembly pathway adapts to LT. We found that yeast cells boost production of assembly factors at LT (20 °C) in comparison to optimal 30 °C, the optimal growth temperature for yeast (Fig. 1c and Supplementary Data 1). The induced factors interact with pre-ribosomes at different maturation stages and contact rRNA-rich centers including the stalk base, the ITS2 “foot” and the rRNA helices that form the catalytic subunit interface (Fig. 1c and Supplementary Figs. 2 and 3).

One LT-induced factor, Puf6, whose location on the 60S pre-ribosome remained unresolved caught our attention (Figs. 1c and 2a, b). Puf6 belongs to the Pumilio and fem3 mRNA-binding factor (PUF) family which shares an RNA binding domain composed of several α-helical repeats^25,51,52. PUF proteins are involved in the post-transcriptional regulation of mRNA expression by binding to regulatory elements of mRNA targets⁵³. Yeast Puf6 and its human ortholog Pum3/Puf-A adopt an atypical L-shaped confirmation and are the most distant member of the yeast PUF family^34,35. In addition to the eight PUF repeats, both Pum3/Puf-A and Puf6 contain three PUF repeats at the N-terminus (Fig. 4a)³⁵. Structure-guided studies demonstrated that these non-canonical repeats participate in recruiting Puf6 to the 60S pre-ribosome (Fig. 4d, e, f). The identified mutants partly overlap with the previously identified interaction surface that (Fig. 4b) contributes to Puf6 function in 7S pre-rRNA processing and ASH1 mRNA localization³⁵. CRAC and yeast three-hybrid studies identified the hairpin-loop tip region within H68 of 25S rRNA as an interaction platform for Puf6. However, Puf6 does not interact with H38 and H66 that contain TL_GAAA motifs within their hairpin-loops suggesting that additional features within the H68 stem region contribute to Puf6:H68 interactions (Fig. 5b).

On the 60S subunit, the H68 TL_GAAA motif (rRNA domain IV) engages in an unusual tertiary contact with a kissing loop (KL) formed between H22 (rRNA domain I) and H88 (rRNA domain V) bringing together distant secondary structure elements. Cryo-EM studies suggest this contact contributes to the compaction of the flexible subunit interface (rRNA domains III–V) with the rigid solvent-exposed side (rRNA domains I, II, and VI) on the 60S pre-ribosome^8,54. Using FRET reporters, we provide evidence for the reconstitution of the KL, and docking of the TL_GAAA onto the KL in vitro. Our studies show that the KL functions as a non-canonical TL_GAAA receptor, as the TL_GAAA motif of H68 docked onto a canonical tetraloop receptor with a similar FRET efficiency. Moreover, we found that Mg²⁺ is required to promote TL_GAAA docking onto the KL similar to canonical TLR-TL_GAAA interactions (Fig. 6d, compare green bars for KL-TL_GAAA and TLR-TL_GAAA). Structural analyses of the 60S subunit revealed that >100 Mg²⁺ ions and >50 monovalent cations are bound to rRNA, the majority of which decorate the RNA-rich subunit interface, in particular the rRNA-rich peptidyl transferase center, where stabilizing cationic tails of r-proteins are absent⁵⁵. These cations stabilize the tertiary structure by mediating interactions between its rRNA domains⁵⁵. We found that Puf6 does not interfere in the formation of the KL-TL_GAAA contact. Instead, FRET studies indicate that Puf6 replaces the need for Mg²⁺ to dock the TL_GAAA onto the KL in vitro (Fig. 6c, d, compare blue and red bar for KL-TL_GAAA). We speculate that Puf6 shields the negative charges of the rRNA backbone to establish correct tertiary interactions between flexible rRNA helices, prior to final stabilization by Mg²⁺^12,47. Puf6 interacts only with H68, but not with isolated H22 and H88 in vivo (Supplementary Fig. 4) supporting the idea that Puf6 ushers H68 docking onto a pre-formed H22-H88 KL.

Cryo-EM structures of early nucleolar states implicate a non-linear pathway to compact 27S pre-rRNA. Initially, the 5′ rRNA domains I and II of 27S pre-rRNA adopt a near mature conformation through tertiary contacts with the 3′ terminal domain VI, to form the solvent-exposed backside of the 60S subunit. In contrast, the central rRNA domains III, IV, and V, which eventually form the subunit interface appear to be dynamic and are not resolved in these early states^5,6. This open arch-like conformation of 60S pre-ribosome undergoes compaction through several long-range tertiary contacts with the central RNA domains III, IV, and V. TL_GAAA/TL_GNRA are prevalent motifs that direct higher-order folding and compaction of RNAs. On a mature 60S subunit, there are >15 GAAA/GNRA motifs located within hairpin loops and bulges engaged in tertiary contacts². A particular challenge for each of these motifs during pre-rRNA folding/compaction is to search and pair with their cognate tetraloop receptors. A productive search is critical at LT where TL_GAAA/TL_GNRA motifs mispaired with non-cognate receptors are stabilized, thus posing a barrier to correct rRNA folding and compaction^11,12,13. We propose that yeast cells induce Puf6 production at LT to ensure that H68 TL_GAAA establishes a correct contact with the pre-formed KL. Puf6 showed an enhanced affinity to H68 when TL_GAAA is bound to KL then to H68 in isolation in buffer conditions promoting tertiary contact formation (Fig. 6g). These data suggest that like Mg²⁺, Puf6 stabilizes the KL-TL_GAAA tertiary contact, and the conformation of the H68 tip region within the tertiary contact is likely to be the state recognized by Puf6. Our SWATH-MS studies revealed additional non-essential assembly factors that were induced at LT (Fig. 1c). These include Nop12, Pwp1, and Arx1 whose depletion, like Puf6, renders yeast cells cold-sensitive and impairs pre-rRNA folding/processing^56,57. Work from the Woolford laboratory revealed how Nop12 ensures correct folding of 5.8S rRNA, thus endorsing the requirement of dedicated factors to direct pre-rRNA folding events at LT⁵⁷.

We propose a model for the order of events that lead to the formation of the KL-TL_GAAA contact and export competent 60S pre-ribosomes (Fig. 8). The emerging 27S pre-rRNA co-transcriptionally folds into different pre-rRNA domains which recruit assembly factors and r-proteins. rRNA domains I, II, and VI fold their near-native conformation to form the solvent-exposed backside of the 60S subunit^5,6. The transition from an open-arch to a compacted 60S pre-ribosome necessitates rRNA domains III, IV, and V to establish tertiary contacts with the folded solvent backside of the 60S subunit, including the KL-TL_GAAA contact. While H68 and H88 are not fully resolved in early nucleolar 60S pre-ribosome intermediates, H22 (rRNA domain I) is visible and is bound to assembly factors Ebp2 and Brx1^5,6. Ebp2:Brx1 prevents H22 to prematurely form a KL with the H88 hairpin-loop within RNA domain V (Fig. 6b). Puf6 is co-transcriptionally recruited to H68, where it awaits the formation of its cognate RNA receptor, the H22:H88 KL. Ebp2-Brx1 removal from the 60S pre-ribosome, via a yet unknown mechanism, re-orients H22 (NE1 particle) making it competent to interact with the hairpin-loop of H88 to form the KL (NE2 particle)⁸. Puf6 bound to the H68 hairpin-loop region promotes docking of the TL_GAAA motif onto the KL and stabilizes the tertiary contact. Docking of the TL_GAAA onto the KL is visible only on a later Nog2-particle implicating a multi-step process to connect distant H22, H68, and H88 rRNA secondary structures (Fig. 6b). Given that Puf6 and H68 are not resolved in the early NE2 state⁸, and that Puf6 release precedes Nog2 recruitment to the 60S pre-ribosome (Figs. 3c, e and 6b), we suggest that Puf6-directed H68 docking onto the KL occurs between the NE2 state and Nog2 recruitment to the 60S pre-ribosome (Figs. 6b and 8).

**Fig. 8: Schematic for Puf6 function during 60S assembly.**

Cryo-EM studies of the Nog2-particle suggest that H68 recruits Sda1 after it has established the KL-TL_GAAA contact⁵⁴. In agreement with these data, we found that, at LT, Sda1 recruitment to 60S pre-ribosomes is severely impaired in puf6∆ cells (Fig. 7a). The formation of the polypeptide exit tunnel (PET) also requires correct compaction of 27S pre-rRNA. Cryo-EM studies of nuclear 60S pre-ribosomes (class R1) isolated from an rpl4∆63-87 mutant (which misassembles the PET) revealed a non-native H68 conformation, that also failed to recruit Sda1⁵⁸. We speculate that correct compaction of 27S pre-rRNA licenses formation of the long-range KL-TL_GAAA tertiary contact which in turn permits recruitment of Sda1 and checkpoint factors, that drive a correctly assembled 60S pre-ribosome towards export competence (Fig. 8).

Why are ribosome assembly factors induced at LT? A series of findings regarding misfolding of 16 rRNA within the bacterial small ribosome subunit (30S), perhaps, provide an insight^50,59,60. These studies describe a cold-sensitive bacterial strain wherein a C23U mutation within 16S rRNA alters the base pair of the 5′ terminal pseudoknot helix to a G-U pair which presumably weakens the 5′ helix. Overexpression of a KH-domain protein RbfA, which is typically induced in wild-type E. coli at LT, rescued the cold-sensitive phenotype of the 16S rRNA mutant strain, suggesting that the C23U mutation decreases the affinity of RbfA for its rRNA-binding site. Notably, E. coli lacking the RbfA gene is cold-sensitive like the C23U mutant. Thus, it seems that the correct formation of the pseudoknot helix within 16S rRNA, at LT, requires the dedicated service of RbfA. It is tempting to speculate that, at LT, frequent pre-rRNA mispairing decreases productive encounters with the ribosome assembly machinery. Alternatively, it is possible that r-proteins and assembly factors are recruited only to correctly folded pre-rRNA, whose levels, at LT, fall significantly due to mispairing/misfolding. Therefore, increasing levels of r-proteins and assembly factors might compensate for the altered equilibrium state and steer pre-rRNA folding towards productive ribosome formation. How yeast cells sense LT to boost r-protein and assembly factor production remains unclear. Strikingly, assembly factor mutants from diverse model organisms including E. coli, S. cerevisiae, D. melanogaster, and A. thaliana, very often exhibit cold-sensitive phenotypes^{49,54,58,59,61,62,63,64,65}. We propose that inducing assembly factors at LT might be a conserved response to counter pre-rRNA misfolding and guarantee efficient ribosome production.

Methods

Yeast strains and plasmids

The Saccharomyces cerevisiae strains used in this study are listed in Supplementary Table 1. Preparation of media, yeast transformations, and genetic manipulations were performed according to established procedures⁶⁶.

All plasmids used in this study are listed in Supplementary Table 2. All recombinant DNA techniques were performed according to established procedures using Escherichia coli XL1 blue cells for cloning and plasmid propagation. Mutations in PUF6 were generated using the QuikChange site-directed mutagenesis kit (Agilent Technologies, Santa Clara, CA, USA). All cloned DNA fragments and mutagenized plasmids were verified by sequencing.

SWATH-MS sample preparation for the LC-MS/MS analyses

Three series of wildtype yeast cells (BY4741) were grown in liquid YPD media at 20 °C, 25 °C, 30 °C, and 37 °C and harvested at OD₆₀₀ ~ 3. 4 OD units of the cells were collected by centrifugation at 1500 × g 5 min at 4 °C. The supernatants were discarded, and the cells were washed three times with cold (−20 °C) acetone. Cells were disrupted five times through 5 min mechanical lysis³² at 4 °C in 8 M urea, 0.1 M NH₄CO₃, and 5 mM EDTA. The total protein amount was determined using BCA Protein Assay Kit (Thermo). In total, 1 mg of yeast proteins was reduced with 12 mM DTT at 37 °C for 30 min and alkylated with 40 mM iodoacetamide at room temperature in the dark for 30 min. Samples were diluted with 0.1 M NH₄HCO₃ to reach a final urea concentration of 1 M and digested with sequencing grade porcine trypsin (Promega, 1:100 trypsin:protein). Digestion was stopped by adding formic acid to a final concentration of 1%. Peptides were desalted using 1cc reverse-phase Sep-Pak tC18 cartridges (Waters, Milford MA) according to the following procedure: Cartridges were wetted with one volume (1 ml) 100% methanol, washed with two volumes of 80% acetonitrile, 0.1% formic acid (FA) and equilibrated with three volumes of 0.1% FA. The acidified peptides were loaded twice on the cartridge, washed with three volumes of 0.1% FA, and eluted with two volumes of 50% acetonitrile, 0.1% FA. Peptide was dried in a speedvac and resolubilized in 50 μl of 0.1% formic acid and frozen at −20 °C. The peptide concentration was measured on nanodrop and adjusted to 1 μg/μl and spiked with 1:20 (v:v) of iRT peptides⁶⁷ for mass spectrometry acquisition. 1 μg of yeast tryptic peptides was injected on a 6600 TripleTof mass spectrometer (ABSciex, Concord, Ontario) interfaced with an Eksigent NanoLC Ultra 1D Plus system (Eksigent, Dublin, CA). The peptides were separated on a 75-μm-diameter, 40 cm-long newObjective emitters packed with Magic C18 AQ 3 μm resin (Michrom BioResources) and eluted at 300 nl/min with a linear gradient of 2-to-30% Buffer A for 120 min (Buffer A: 2% acetonitrile, 0.1% formic acid; Buffer B: 98% acetonitrile, 0.1% formic acid). MS data acquisition was performed in either data-dependent acquisition (DDA, top20, with 20 s dynamic exclusion after 1 MS/MS) or data-independent acquisition (DIA) SWATH-MS mode (64 variable windows setup acquired each for 50 ms and MS1 scan for 250 ms)⁶⁸. For either mode, the collision energy was set to 0.0625 × m/z—10.5 with a 15-eV collision energy spread regardless of the precursor charge state.

DDA data analysis

A detailed description for DDA search and spectral library construction¹⁵ can be found in the Supplementary Information.

SWATH-MS data analyses

A detailed description of SWATH-MS data extraction⁴⁹ can be found in Supplementary Information. The nine most significant clusters as suggested by the Dmin and overlap functions of mFuzz (Supplementary Fig. 1j, k) (embedding 429 of the significantly regulated proteins) are provided in Supplementary Data 1. The dataset has been deposited to the ProteomeXchange Consortium via the PRIDE⁶⁹ partner repository with the dataset identifier PXD016320.

Temperature shift assay and whole-cell extract preparation

Wildtype yeast cells (BY4741) were grown until the late log phase at indicated temperatures. Cells were diluted into pre-cooled or pre-warmed media to OD600 = 0.5. Samples were retrieved at indicated timepoints and whole-cell extracts were prepared. 4 OD units were harvested by centrifugation at 5422×g for 3 min and cells were prechilled on ice for 5 min. In total, 150 μl lysis solution (1.85 M NaOH, 8% β-mercaptoethanol) was added to the cells and then lysed on ice for 10 min. In total, 150 μl 50% TCA were added and proteins were precipitated on ice for 10 min. Samples were centrifuged for 2 min at 25,199×g at 4 °C. Pellet was washed with 1 ml 100% ice-cold acetone and afterward air-dried. Pellet was resuspended in 100 μl 1× LDS sample buffer (Invitrogen, Carlsbad, CA, USA), heated for 10 min at 70 °C before loading on an SDS gel.

CRAC analysis

CRAC analysis was performed using the Puf6-HTP strain^38,70. Briefly, S. cerevisiae cells were grown in YPD media until an OD600 of ~0.5 was reached and UV irradiated. Cells were cross-linked in the Vari-X-linker for 12 s and CRAC libraries were paired-end sequenced (50 bp) on a HiSeq2500 at Edinburgh Genomics, University of Edinburgh. The CRAC data were processed using pyCRAC-1.42 software suite (https://git.ecdf.ed.ac.uk/sgrannem/pycrac) and mapped to the reference sequence Saccharomyces_cerevisiae. R64-1-1.75 using NovoAlign-2.07 (http://www.novocraft.com). Plots of reads aligned to the 35S rRNA sequence were made with the pyPileup module of pyCRAC. The data have been deposited in the Gene Expression Omnibus (GEO) database under accession no. GSE174587. For CRAC data analysis, data from two biological replicates were analyzed⁷⁰; yielding essentially the same outcomes; the data set with the better coverage (Puf6-data-set II) has been used for the presented figure.

Yeast-3-hybrid assay

For yeast-3-hybrid assays⁷¹ different rRNA helices were cloned into a p3AMS2-1 plasmid and Puf6 was cloned into pACT2 vector (Supplementary Table 2). Transformed L40 coat cells were spotted in 10-fold serial dilutions on selective SD-Leu-Ura and SD-His plates with indicated concentrations of 3-Amino-1,2,4-triazole (Sigma).

Cross-linking MS

Reconstituted Puf6:60S complexes were analyzed by XL-MS using chemical cross-linking with disuccinimidyl suberate (DSS)^72,73. In total, 100 μM purified 60S ribosome was incubated with 200 μM Puf6 at 20 °C for 10 min in 60S binding buffer (150 mM NaCl, 20 mM HEPES pH7.5, 5 mM MgCl₂, 5 mM β-mercaptoethanol) and cross-linked with DSS-d0/d12 (25 mM stock solution in anhydrous dimethylformamide; Creative Molecules) to a final concentration of 1 mM. The reaction was incubated at 37 °C for 30 min and subsequently quenched using 50 mM ammonium bicarbonate. Cross-linked complexes were reduced, alkylated, and digested sequentially with endoproteinase Lys-C and trypsin^72,73. The digest was fractionated with size exclusion chromatography (Superdex Peptide, GE) and fractions were analyzed by LC-MS/MS on an Orbitrap Elite mass spectrometer⁷². Data analysis was performed using xQuest/xProphet (v2.1.3) and results were filtered to a false discovery rate of <5% at the cross-linked peptide pair level⁷⁴. The identifications are summarized in Supplementary Data 2, and the mass spectrometry data is deposited to the ProteomeXchange Consortium via the PRIDE⁶⁹ partner repository with the identifier PXD024131.

Purification of pre-ribosomal particles

Tandem Affinity Purification (TAP) of pre-ribosomal particles was carried out using established procedures³². Calmodulin eluates were separated on NuPAGE 4–12% Bis-Tris gradient gels (Invitrogen) and analyzed by Silver staining or Western blotting using indicated antibodies. Primary antibodies were used in the following dilutions: α-Puf6 (1:2000; this study), α-Nog2 (1:1000, this study), α-Nmd3 (1:1000, A. Johnson, University of Texas, Austin, USA), α-Sda1 (1:1000, this study), α-Nog2 (1:500, this study), α-TAP (CBP) (1:1000, Merck AG, Darmstadt, Germany #07-482), α-uL29 (1:2000)³², α-Arc1 (1:4000, E Hurt, University of Heidelberg, Heidelberg, Germany). The secondary HRP-conjugated αrabbit antibody (Sigma-Aldrich, St Louis, MO, USA) was used at 1:2000 dilution. Protein signals were detected using immune-Star HRP chemiluminescence kit (Bio-Rad Laboratories, Hercules, CA, USA) and captured on Fuji Super RX X-ray films (Fujifilm, Japan) or digitally using ImageQuant Analyzer (GE, Healthcare).

Fluorescence microscopy and heterokaryon assay

Ribosome export was monitored using extrachromosomal uL18-GFP and uS5-GFP reported constructs³². Cells were grown at indicated temperatures to early log phase and visualized with a DM6000B microscope (Leica, Germany). Images were acquired with a fitted digital camera (ORCA-ER; Hamamatsu Photonics, Hamamatsu, SZK, Japan) using Openlab software (Perkin-Elmer, Waltham, MA, USA) and analysis was performed using ImageJ (NIH, Bethesda, Maryland, U.S) For the heterokaryon assay³² different yeast strains were grown until OD600 of ~1. Formating, Arx1–GFP, Gar1–GFP, Puf6-GFP cells were mixed with kar1-1 cells expressing endogenously tagged Nup82-mCherry. The mixture was concentrated onto 0.45 mm nitrocellulose filters and subsequently placed on YPD plates. After 1 h at 30 °C, filters were transferred to YPD plates containing 50 mg/ml cycloheximide and incubated for another 1–2 h before cells were analyzed by fluorescence microscopy.

Recombinant protein expression

Recombinant His6-Puf6 protein was expressed in E. coli BL21 pRARE cells (Merck Millipore, Darmstadt, Germany) at 20 °C for 18 h and 0.5 mM IPTG. His6-tagged proteins were affinity purified by gravity flow batch purification using cOmplete His-Tag purification Resin (Roche AG, Basel, Switzerland) in 500 mM NaCl, 20 mM HEPES pH 7.5, 5 mM MgCl₂, 5 mM β-mercaptoethanol, 1 mM TCEP. Eluates were concentrated and further purified through size exclusion chromatography in 150 mM NaCl, 20 mM HEPES pH7.5, 5 mM MgCl₂, 5 mM β-mercaptoethanol on a Superdex 200 10/300 GL column (GE Healthcare). For ensemble FRET, His6-GB1-Puf6-PUM (161-656aa) was expressed and purified as described above in 500 mM KCl, 20 mM HEPES pH 7.4, 1 mM DTT, 1 mM TCEP, 0.05% Triton-X. Eluates were concentrated, dialyzed into 100 mM KCl, 20 mM HEPES pH 7.5, 1 mM DTT, and further purified through size exclusion chromatography in 100 mM KCl, 20 mM HEPES pH7.5, 1 mM DTT on a Superdex 200 10/300 GL column (GE Healthcare).

60S pelleting assay

The binding of the purified Puf6 and its mutants to the mature 60S subunit was investigated by sucrose pelleting assay⁷⁵. Briefly, purified proteins were incubated with 150 nM mature 60S subunit in binding buffer (150 mM NaCl, 20 mM HEPES pH 7.5, 5 mM MgCl2, 5 mM β-mercaptoethanol) for 10 min at 20 °C and layered onto a 30% (w/v) sucrose cushion. The samples were centrifuged for 105 min at 385,840 × g in a TLA-100 ultracentrifuge rotor. After removing the supernatant, the pellet was resuspended in buffer A (500 mM NaCl, 20 mM HEPES pH 7.5, 5 mM MgCl₂, 5 mM β-mercaptoethanol). A negative control lacking 60S subunits was treated identically to serve as a control for protein precipitation. All samples were analyzed subsequently on a NuPAGE 4–12% Bis-Tris gradient gel (Invitrogen, Carlsbad, CA, USA).

Ensemble FRET measurements

Ensemble emission spectra of the fluorescently labeled (sCy3/5) RNA constructs (Supplementary Table 3) with varying amounts of mono- and divalent cations (K⁺, Mg²⁺) were measured with a fluorescence spectrometer (Cary Eclipse, Agilent) at room temperature and corrected for bleed-through and direct-excitation. FRET proximity ratios were calculated and plotted against [K⁺], [Mg²⁺] (with and without 10 µM Puf6-PUM). Details are provided in Supplementary Information. Data analysis and plots were made using OriginPro 2020 (64-bit) SR1 (9.7.0.188).

RNA UV melting

UV thermal melting curves (absorption @260 nm) of the RNA construct (Supplementary Table 7) with varying amounts of divalent cations (Mg²⁺) in presences of 100 mM monovalent cations (K⁺) were recorded with a UV/VIS absorption spectrometer (Cary 100, Agilent) between 15 and 90 °C. More details can be found in the Supplementary Information.

Figures and structural modeling

Figures of molecular structures were created using PyMOL (2.2.0)⁷⁶. Sequence alignments were generated using MAFFT (v7) JalView (2.11.1.4). Structural models of Puf6 were generated with Phyre2 server⁷⁷ and visualized using PyMOL (2.2.0)⁷⁶. Structure models of the in vitro RNA construct were generated using RNA composer⁴³ based on prior knowledge (kissing loop formation H22 and H88 and base-paired helices H22, H68, H88 in PDB ID: 4V7R)² and secondary structure prediction using ViennaRNA⁷⁸.

Statistics and reproducibility

Unless otherwise indicated, error bars represent the mean ± standard deviation of at least three biological replicates (i.e., n ≥ 3). Statistical analysis was performed using Prism (version 8.4.2; GraphPad Software Inc., La Jolla, CA, USA). Experiments in Figs. 2b, d; 3a–f, 4g; 5c, d; 7a and Supplementary Fig. 4c were performed at least three times and one representative result was used for figure preparation.

Reporting summary

Further information on research design is available in the Nature Research Reporting Summary linked to this article.

Data availability

The data that support this study are available from the corresponding author upon reasonable request. The datasets generated in this study are available in the following repositories: The SWATH-MS and XL-MS data analyses have been deposited to the ProteomeXchange Consortium via the PRIDE partner repository with unique identifiers PXD016320 and PXD024131, respectively. The sequencing data have been deposited in the Gene Expression Omnibus database; accession no. GSE174587. Source data are provided with this paper.

References

Ganser, L. R., Kelly, M. L., Herschlag, D. & Al-Hashimi, H. M. The roles of structural dynamics in the cellular functions of RNAs. Nat. Rev. Mol. Cell Biol. 20, 474–489 (2019).
Article CAS PubMed PubMed Central Google Scholar
Ben-Shem, A. et al. The structure of the eukaryotic ribosome at 3.0 Å resolution. Science (80-.) 334, 1524–1529 (2011).
Article ADS CAS Google Scholar
Dragon, F. et al. A large nucleolar U3 ribonucleoprotein required for 18S ribosomal RNA biogenesis. Nature 417, 967–970 (2002).
Article ADS CAS PubMed Google Scholar
Kornprobst, M. et al. Architecture of the 90S pre-ribosome: a structural view on the birth of the Eukaryotic Ribosome. Cell 166, 380–393 (2016).
Article CAS PubMed Google Scholar
Kater, L. et al. Visualizing the assembly pathway of nucleolar pre-60S ribosomes. Cell 171, 1599–1610.e14 (2017).
Article CAS PubMed PubMed Central Google Scholar
Sanghai, Z. A. et al. Modular assembly of the nucleolar pre-60S ribosomal subunit. Nature 556, 126–129 (2018).
Article ADS CAS PubMed PubMed Central Google Scholar
Barrio-Garcia, C. et al. Architecture of the Rix1-Rea1 checkpoint machinery during pre-60S-ribosome remodeling. Nat. Struct. Mol. Biol. 23, 37–44 (2016).
Article CAS PubMed Google Scholar
Kater, L. et al. Construction of the central protuberance and L1 stalk during 60S subunit biogenesis ll construction of the central protuberance and L1 stalk during 60S subunit biogenesis. Mol. Cell 79, 615–628.e5 (2020).
Article CAS PubMed Google Scholar
Matsuo, Y. et al. Coupled GTPase and remodelling ATPase activities form a checkpoint for ribosome export. Nature 505, 112–116 (2014).
Article ADS PubMed CAS Google Scholar
Klinge, S. & Woolford, J. L. Ribosome assembly coming into focus. Nat. Rev. Mol. Cell Biol. 20, 116–131 (2019).
Article CAS PubMed PubMed Central Google Scholar
Herschlag, D. RNA chaperones and the RNA folding problem. J. Biol. Chem. 270, 20871–20874 (1995).
Article CAS PubMed Google Scholar
Woodson, S. A. Compact intermediates in RNA folding. Annu. Rev. Biophys. 39, 61–77 (2010).
Article CAS PubMed PubMed Central Google Scholar
ClatterbuckSoper, S. F., Dator, R. P., Limbach, P. A. & Woodson, S. A. InVivo X-Ray footprinting of pre-30S ribosomes reveals chaperone-dependent remodeling of late assembly intermediates. Mol. Cell 52, 506–516 (2013).
Article CAS Google Scholar
Gillet, L. C. et al. Targeted data extraction of the MS/MS spectra generated by data-independent acquisition: a new concept for consistent and accurate proteome analysis. Mol. Cell. Proteom. 11, O111.016717 (2012).
Schubert, O. T. et al. Building high-quality assay libraries for targeted analysis of SWATH MS data. Nat. Protoc. 10, 426–441 (2015).
Article CAS PubMed Google Scholar
Huang, D. W., Sherman, B. T. & Lempicki, R. A. Systematic and integrative analysis of large gene lists using DAVID bioinformatics resources. Nat. Protoc. 4, 44–57 (2009).
Article CAS Google Scholar
Wu, S. et al. Diverse roles of assembly factors revealed by structures of late nuclear pre-60S ribosomes. Nature 534, 133–137 (2016).
Article ADS CAS PubMed PubMed Central Google Scholar
Granneman, S., Petfalski, E. & Tollervey, D. A cluster of ribosome synthesis factors regulate pre-rRNA folding and 5.8S rRNA maturation by the Rat1 exonuclease. EMBO J. 30, 4006–4019 (2011).
Article CAS PubMed PubMed Central Google Scholar
Kemmler, S., Occhipinti, L., Veisu, M. & Panse, V. G. Yvh1 is required for a late maturation step in the 60S biogenesis pathway. J. Cell Biol. 186, 863–880 (2009).
Article CAS PubMed PubMed Central Google Scholar
Lo, K. Y., Li, Z., Wang, F., Marcotte, E. M. & Johnson, A. W. Ribosome stalk assembly requires the dual-specificity phosphatase Yvh1 for the exchange of Mrt4 with P0. J. Cell Biol. 186, 849–862 (2009).
Article CAS PubMed PubMed Central Google Scholar
Zhang, J. et al. Assembly factors Rpf2 and Rrs1 recruit 5S rRNA and ribosomal proteins rpL5 and rpL11 into nascent ribosomes. Genes Dev. 21, 2580–2592 (2007).
Article CAS PubMed PubMed Central Google Scholar
Kater, L. et al. Visualizing the assembly pathway of nucleolar pre-60S ribosomes. Cell 171, 1599–1610.e14 (2017).
Li, Z. et al. Rational extension of the ribosome biogenesis pathway using network-guided genetics. PLoS Biol. 7, e1000213 (2009).
Quenault, T., Lithgow, T. & Traven, A. PUF proteins: repression, activation and mRNA localization. Trends Cell Biol. 21, 104–112 (2011).
Article CAS PubMed Google Scholar
Zamore, P. D., Williamson, J. R. & Lehmann, R. The Pumilio protein binds RNA through a conserved domain that defines a new class of RNA-binding proteins. RNA 3, 1421–1433 (1997).
CAS PubMed PubMed Central Google Scholar
Yang, Y. T., Ting, Y. H., Liang, K. J. & Lo, K. Y. The roles of Puf6 and Loc1 in 60S biogenesis are interdependent, and both are required for efficient accommodation of Rpl43. J. Biol. Chem. 291, 19312–19323 (2016).
Article CAS PubMed PubMed Central Google Scholar
Liang, K. J., Yueh, L. Y., Hsu, N. H., Lai, J. S. & Lo, K. Y. Puf6 and Loc1 are the dedicated chaperones of ribosomal protein Rpl43 in Saccharomyces cerevisiae. Int. J. Mol. Sci. 20, 5941 (2019).
Gu, W., Deng, Y., Zenklusen, D. & Singer, R. H. A new yeast PUF family protein, Puf6p, represses ASH1 mRNA translation and is required for its localization. Genes Dev. 18, 1452–1465 (2004).
Article CAS PubMed PubMed Central Google Scholar
Shahbabian, K., Jeronimo, C., Forget, A., Robert, F. & Chartrand, P. Co-transcriptional recruitment of Puf6 by She2 couples translational repression to mRNA localization. Nucleic Acids Res. 42, 8692–8704 (2014).
Article CAS PubMed PubMed Central Google Scholar
Jung, D., Seo, J. S., Nam, J. & Kim, J. Functional association of Loc1 and Puf6 with RNA helicase Dhh1 in translational regulation of Saccharomyces cerevisiae Ste12. PLoS ONE 14, e0220137 (2019).
Article CAS PubMed PubMed Central Google Scholar
Huh, W. K. et al. Global analysis of protein localization in budding yeast. Nature 425, 686–691 (2003).
Article ADS CAS PubMed Google Scholar
Altvater, M., Schütz, S., Chang, Y. & Panse, V. G. Dissecting ribosome assembly and transport in budding yeast. in Methods in Cell Biology vol. 122 437–461 (Academic Press Inc., 2014).
Nissan, T. A., Baßler, J., Petfalski, E., Tollervey, D. & Hurt, E. 60S pre-ribosome formation viewed from assembly in the nucleolus until export to the cytoplasm. EMBO J. 21, 5539–5547 (2002).
Article CAS PubMed PubMed Central Google Scholar
Zhang, C. D. et al. Characteristics and evolution of the PUF gene family in Bombyx mori and 27 other species. Mol. Biol. Rep. 39, 675–683 (2012).
Article CAS PubMed Google Scholar
Qiu, C., McCann, K. L., Wine, R. N., Baserga, S. J. & Hall, T. M. T. A divergent Pumilio repeat protein family for pre-rRNA processing and mRNA localization. Proc. Natl Acad. Sci. USA 111, 18554–18559 (2014).
Article ADS CAS PubMed PubMed Central Google Scholar
Chen, W., Xie, Z., Yang, F. & Ye, K. Stepwise assembly of the earliest precursors of large ribosomal subunits in yeast. Nucleic Acids Res. 45, 6837–6847 (2017).
Article CAS PubMed PubMed Central Google Scholar
Chaker-Margot, M. & Klinge, S. Assembly and early maturation of large subunit precursors. RNA 25, 465–471 (2019).
Article CAS PubMed PubMed Central Google Scholar
Granneman, S., Kudla, G., Petfalski, E. & Tollervey, D. Identification of protein binding sites on U3 snoRNA and pre-rRNA by UV cross-linking and high-throughput analysis of cDNAs. Proc. Natl Acad. Sci. USA 106, 9613–9618 (2009).
Article ADS CAS PubMed PubMed Central Google Scholar
Leitner, A. et al. Probing native protein structures by chemical cross-linking, mass spectrometry, and bioinformatics. Mol. Cell. Proteom. 9, 1634–1649 (2010).
Article CAS Google Scholar
Tüting, C., Iacobucci, C., Ihling, C. H., Kastritis, P. L. & Sinz, A. Structural analysis of 70S ribosomes by cross-linking/mass spectrometry reveals conformational plasticity. Sci. Rep. 10, 12618 (2020).
Article ADS PubMed PubMed Central CAS Google Scholar
Noeske, J. et al. High-resolution structure of the Escherichia coli ribosome. Nat. Struct. Mol. Biol. 22, 336–341 (2015).
Article CAS PubMed PubMed Central Google Scholar
Anger, A. M. et al. Structures of the human and Drosophila 80S ribosome. Nature 497, 80–85 (2013).
Article ADS CAS PubMed Google Scholar
Antczak, M. et al. New functionality of RNAComposer: an application to shape the axis of miR160 precursor structure. Acta Biochim. Pol. 63, 737–744 (2016).
CAS PubMed Google Scholar
Woodson, S. A. Metal ions and RNA folding: A highly charged topic with a dynamic future. Curr. Opin. Chem. Biol. 9, 104–109 (2005).
Article CAS PubMed Google Scholar
Freisinger, E. & Sigel, R. K. O. From nucleotides to ribozymes-A comparison of their metal ion binding properties. Coord. Chem. Rev. 251, 1834–1851 (2007).
Article CAS Google Scholar
Pyle, A. M. Metal ions in the structure and function of RNA. J. Biol. Inorg. Chem. 7, 679–690 (2002).
Article CAS PubMed Google Scholar
Fiore, J. L., Holmstrom, E. D. & Nesbitt, D. J. Entropic origin of Mg 2+-facilitated RNA folding. Proc. Natl Acad. Sci. USA 109, 2902–2907 (2012).
Article ADS CAS PubMed PubMed Central Google Scholar
Hodak, J. H., Fiore, J. L., Nesbitt, D. J., Downey, C. D. & Pardi, A. Docking kinetics and equilibrium of a GAAA tetraloop-receptor motif probed by single-molecule FRET. Proc. Natl Acad. Sci. USA 102, 10505–10510 (2005).
Article ADS CAS PubMed PubMed Central Google Scholar
Klingauf-Nerurkar, P. et al. The gtpase nog1 co-ordinates the assembly, maturation and quality control of distant ribosomal functional centers. Elife 9,e52474 (2020).
Dammel, C. S. & Noller, H. F. A cold-sensitive mutation in 16S rRNA provides evidence for helical switching in ribosome assembly. Genes Dev. 7, 660–670 (1993).
Article CAS PubMed Google Scholar
Wang, X., Zamore, P. D. & Tanaka Hall, T. M. Crystal structure of a Pumilio homology domain. Mol. Cell 7, 855–865 (2001).
Article CAS PubMed Google Scholar
Wang, M., Ogé, L., Perez-Garcia, M. D., Hamama, L. & Sakr, S. The PUF protein family: overview on PUF RNA targets, biological functions, and post transcriptional regulation. Int. J. Mol. Sci. 19, 410 (2018).
Wang, X., McLachlan, J., Zamore, P. D. & Hall, T. M. T. Modular recognition of RNA by a human Pumilio-homology domain. Cell 110, 501–512 (2002).
Article CAS PubMed Google Scholar
Micic, J. et al. Coupling of 5S RNP rotation with maturation of functional centers during large ribosomal subunit assembly. Nat. Commun. 11, 1–16 (2020).
Article ADS CAS Google Scholar
Klein, D. J., Moore, P. B. & Steitz, T. A. The contribution of metal ions to the structural stability of the large ribosomal subunit. RNA 10, 1366–1379 (2004).
Article CAS PubMed PubMed Central Google Scholar
Meyer, A. E., Hung, N. J., Yang, P., Johnson, A. W. & Craig, E. A. The specialized cytosolic J-protein, Jjj1, functions in 60S ribosomal subunit biogenesis. Proc. Natl Acad. Sci. USA 104, 1558–1563 (2007).
Article ADS CAS PubMed PubMed Central Google Scholar
Talkish, J., Campbell, I. W., Sahasranaman, A., Jakovljevic, J. & Woolford, J. L. Ribosome assembly factors Pwp1 and Nop12 are important for folding of 5.8S rRNA during ribosome biogenesis in Saccharomyces cerevisiae. Mol. Cell. Biol. 34, 1863–1877 (2014).
Article CAS PubMed PubMed Central Google Scholar
Wilson, D. M. et al. Structural insights into assembly of the ribosomal nascent polypeptide exit tunnel. Nat. Commun. 11, 5111 (2020).
Dammel, C. S. & Noller, H. F. Suppression of a cold-sensitive mutation in 16s rRNA by overexpression of a novel ribosome-binding factor, RbfA. Genes Dev. 9, 626–637 (1995).
Article CAS PubMed Google Scholar
Jones, P. G. & Inouye, M. RbfA, a 30S ribosomal binding factor, is a cold-shock protein whose absence triggers the cold-shock response. Mol. Microbiol. 21, 1207–1218 (1996).
Article CAS PubMed Google Scholar
Guthrie, C., Nashimoto, H. & Nomura, M. Structure and function of E. coli ribosomes. 8. Cold-sensitive mutants defective in ribosome assembly. Proc. Natl Acad. Sci. USA 63, 384–391 (1969).
Article ADS CAS PubMed PubMed Central Google Scholar
Falke, E. V. & Wright, T. R. F. Cold-sensitive mutants of drosophila melanogaster defective in Ribosome assembly. Genetics 81, 655–682 (1975).
Ursic, D. & Davies, J. A cold-sensitive mutant of Saccharomyces cerevisiae defective in ribosome processing. MGG Mol. Gen. Genet. 175, 313–323 (1979).
Article CAS PubMed Google Scholar
Connolly, K., Rife, J. P. & Culver, G. Mechanistic insight into the ribosome biogenesis functions of the ancient protein KsgA. Mol. Microbiol. 70, 1062–1075 (2008).
Article CAS PubMed PubMed Central Google Scholar
Liu, Y., Tabata, D. & Imai, R. A cold-inducible DEAD-box RNA helicase from arabidopsis thaliana regulates plant growth and development under low temperature. PLoS ONE 11, e0154040–e0154040 (2016).
Article PubMed PubMed Central CAS Google Scholar
Longtine, M. S. et al. Additional modules for versatile and economical PCR-based gene deletion and modification in Saccharomyces cerevisiae. Yeast 14, 953–961 (1998).
Article CAS PubMed Google Scholar
Escher, C. et al. Using iRT, a normalized retention time for more targeted measurement of peptides. Proteomics 12, 1111–1121 (2012).
Article CAS PubMed PubMed Central Google Scholar
Navarro, P. et al. A multicenter study benchmarks software tools for label-free proteome quantification. Nat. Biotechnol. 34, 1130–1136 (2016).
Article CAS PubMed PubMed Central Google Scholar
Perez-Riverol, Y. et al. The PRIDE database and related tools and resources in 2019: Improving support for quantification data. Nucleic Acids Res. 47, D442–D450 (2019).
Article CAS PubMed Google Scholar
Van Nues, R. et al. Kinetic CRAC uncovers a role for Nab3 in determining gene expression profiles during stress. Nat. Commun. 8, 1–18 (2017).
ADS CAS Google Scholar
SenGupta, D. J. et al. A three-hybrid system to detect RNA-protein interactions in vivo. Proc. Natl Acad. Sci. USA 93, 8496–8501 (1996).
Article ADS CAS PubMed PubMed Central Google Scholar
Greber, B. J. et al. Architecture of the large subunit of the mammalian mitochondrial ribosome. Nature 505, 515–519 (2014).
Article ADS CAS PubMed Google Scholar
Leitner, A. et al. Expanding the chemical cross-linking toolbox by the use of multiple proteases and enrichment by size exclusion chromatography. Mol. Cell. Proteom. 11, M111 (2012).
Walzthoeni, T. et al. False discovery rate estimation for cross-linked peptides identified by mass spectrometry. Nat. Methods 9, 901–903 (2012).
Article CAS PubMed Google Scholar
Greber, B. J., Boehringer, D., Montellese, C. & Ban, N. Cryo-EM structures of Arx1 and maturation factors Rei1 and Jjj1 bound to the 60S ribosomal subunit. Nat. Struct. Mol. Biol. 19, 1228–1233 (2012).
Article CAS PubMed Google Scholar
Delano, W. L. PyMOL: An Open-Source Molecular Graphics Tool.
Kelley, L. A., Mezulis, S., Yates, C. M., Wass, M. N. & Sternberg, M. J. E. The Phyre2 web portal for protein modeling, prediction and analysis. Nat. Protoc. 10, 845–858 (2015).
Article CAS PubMed PubMed Central Google Scholar
Lorenz, R. et al. ViennaRNA Package 2.0. Algorithms Mol. Biol. 6, 26 (2011).
Article PubMed PubMed Central Google Scholar

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Acknowledgements

We thank M. Peter and E. Hurt for generously sharing yeast strains, plasmids, and antibodies. We thank all members of the Panse laboratory for enthusiastic discussions and the Center for Microscopy and Image Analysis, UZH for maintaining the imaging equipment. M.O.-O. acknowledges support from the Boehringer Ingelheim Fonds Ph.D. fellowship program. J.J.P. was the recipient of an ETH Zurich Postdoctoral Fellowship supported by the Marie Curie Actions for People COFUND program. Research in the Granneman lab was supported by grants from the Wellcome Trust (091549 to S.G.) and a Medical Research Council Non-Clinical Senior Research Fellowship (MR/R008205/1 to S.G.). R.K.O.S. acknowledges support from the Swiss National Science Foundation and the UZH. V.G.P. is supported by grants from the Swiss National Science Foundation (310030_188527), NCCR in RNA and Disease, ETH Zurich, Novartis Foundation, Olga Mayenfisch Stiftung, and a Starting Grant Award (EURIBIO260676) from the European Research Council.

Author information

Stefan Gerhardy
Present address: Department of Early Discovery Biochemistry, Genentech Inc., South San Francisco, CA, USA
Richard Börner
Present address: Laserinstitut Hochschule Mittweida, University of Applied Sciences Mittweida, Mittweida, Germany
Janusz J. Petkowski
Present address: Department of Earth, Atmospheric, and Planetary Sciences, Massachusetts Institute of Technology, Cambridge, MA, USA
These authors contributed equally: Stefan Gerhardy, Michaela Oborská-Oplová.

Authors and Affiliations

Institute of Medical Microbiology, University of Zurich, Zurich, Switzerland
Stefan Gerhardy, Michaela Oborská-Oplová & Vikram Govind Panse
Institute of Biochemistry, ETH Zurich, Zurich, Switzerland
Stefan Gerhardy, Michaela Oborská-Oplová & Janusz J. Petkowski
Institute of Molecular Systems Biology, ETH Zurich, Zurich, Switzerland
Ludovic Gillet, Alexander Leitner & Ruedi Aebersold
Department of Chemistry, University of Zurich, Zurich, Switzerland
Richard Börner & Roland K. O. Sigel
Centre for Synthetic and Systems Biology (SynthSys), University of Edinburgh, Edinburgh, UK
Rob van Nues & Sander Granneman
Institute of Cell Biology, University of Edinburgh, Edinburgh, UK
Rob van Nues
Department of Biochemistry, University of Zurich, Zurich, Switzerland
Erich Michel
Faculty of Science, University of Zurich, Zurich, Switzerland
Ruedi Aebersold & Vikram Govind Panse

Authors

Stefan Gerhardy
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Michaela Oborská-Oplová
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Ludovic Gillet
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Richard Börner
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Rob van Nues
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Alexander Leitner
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Erich Michel
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Janusz J. Petkowski
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Sander Granneman
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Roland K. O. Sigel
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Ruedi Aebersold
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Vikram Govind Panse
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Contributions

Experimental design: S. Gerhardy, M.O.-O., L.G., R.B., R.V.N., A.L., E.M., J.J.P., S. Granneman, R.K.O.S., R.A., V.G.P.; experiment execution: S. Gerhardy, M.O.-O., L.G., R.B., R.V.N., A.L., E.M., J.J.P.; data analysis: S. Gerhardy, M.O.-O., L.G., R.B., R.V.N., A.L., E.M., J.J.P.; scientific input and supervision: S. Granneman, R.K.O.S., R.A., V.G.P.; writing—original draft: S. Gerhardy, M.O.-O., V.G.P.; writing—review & editing: S. Gerhardy, M.O.-O., L.G., R.B., R.V.N., A.L., E.M., J.J.P., S. Granneman, R.K.O.S., R.A.,V.G.P.

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Correspondence to Vikram Govind Panse.

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Gerhardy, S., Oborská-Oplová, M., Gillet, L. et al. Puf6 primes 60S pre-ribosome nuclear export at low temperature. Nat Commun 12, 4696 (2021). https://doi.org/10.1038/s41467-021-24964-2

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Received: 26 March 2021
Accepted: 16 July 2021
Published: 04 August 2021
DOI: https://doi.org/10.1038/s41467-021-24964-2

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