Abstract
Technical advances have pushed the resolution limit of single-particle cryo-electron microscopy (cryo-EM) throughout the past decade and made the technique accessible to a wide range of samples. Among them, multisubunit DNA-dependent RNA polymerases (Pols) are a prominent example. This review aims at briefly summarizing the architecture and structural adaptations of Pol I, highlighting the importance of cryo-electron microscopy in determining the structures of transcription complexes.
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1 Cryo-Electron Microscopy : The New Standard in Transcription Research
The visualization of macromolecular complexes is essential to our understanding of their function. This is especially true for eukaryotic RNA polymerases (Pol) I, II, and III. These enzymes play a pivotal role within the central dogma of molecular biology by synthesizing the 35S ribosomal RNA precursor (Pol I), messenger and many noncoding RNAs (Pol II), and tRNAs , 5S rRNA , U6 snRNA as well as other small, structured RNAs (Pol III).
Almost 20 years ago, advances in cryo-crystallography allowed solving the structure of RNA polymerase II , first in its 10-subunit form [1], later comprising all 12 subunits [2], providing insights into the function of this molecular machine at an unprecedented level of detail. This gave rise to a number of follow-up studies, resulting in structures of an actively elongating Pol II form [3, 4] and elongation [5, 6] or initiation [7, 8] factor–bound Pol II. Thereby, the molecular mechanisms of transcription , as well as regulatory and catalytic functions of transcription factors , could be deciphered.
However, X-ray diffraction analysis relies on the availability and quality of the analyzed crystals. It is therefore not surprising that a number of transcription factors could never be successfully studied in complex with their respective polymerase by crystallography. This includes the general Pol II initiation factors TFIIF and TFIIE, which are involved in initiation complex formation and promoter DNA melting [9]. A crystal structure of Pol I was solved 10 years after Pol II in an inactive conformation [10, 11], a Pol III crystal structure is still lacking to date. Crystallization depends on high amounts of purified material. Whereas conformational heterogeneity usually is problematic for crystal formation, cryo-EM allows for visualization of different functional states of proteins in vitrified ice, therefore capturing close-to-native states. Technical improvements such as the development of direct electron detectors [10], highly stable microscopes and improved processing software [11, 12] pushed previous limitations of the technique and led to the often quoted “resolution revolution” in cryo-EM [13]. Within this book, we describe protocols for a sample preparation and single-particle cryo-EM screening workflow, adapted to RNA polymerase complexes (Chapter 6 ).
Here, we aim to briefly outline the benefits and limitations of single-particle cryo-EM for the analysis of transcription complexes at the example of RNA polymerase I in the context of functional characterization reviewed by Merkl et al. in the same issue.
2 Pol I Specific Subunits Resemble Built-in Transcription Factors
Yeast Pol I has a molecular weight of 590 kDa and consists of 14 protein subunits. A core of ten subunits includes the large subunits A190 and A135, the subcomplex AC40/AC19 (shared with Pol III), the common subunits Rpb5 , Rpb6 , Rpb8 , Rpb10 , and Rpb12 (also included in Pol II and Pol III) and the subunit A12.2. Pol I also contains the specific subunit complex A14/A43 forming the “stalk” and the specific heterodimer subcomplex A49/A34.5. In Fig. 1, we present a “hybrid model” of Pol I, constructed using the software package COOT [14]. The model combines structural information obtained from cryo-EM reconstructions of elongation and initiation complexes and the dimer crystal structure (see below). The Pol I subunit complex A49/A34.5 structurally and functionally resembles a built-in version of subunits Tfg1/2 constituting the Pol II initiation factor TFIIF [15] and is involved in open complex stabilization as well as promoter escape. Nevertheless, subcomplex A49/A34.5 may also contribute to transcript cleavage activity [16] and may play a role in elongation [17], as reviewed by Merkl et al. in this book. The Pol I subunit A12.2 displays features of the Pol II subunit Rpb9 , as well as the Pol II elongation /cleavage factor TFIIS , explaining the intrinsic ability of Pol I for transcript cleavage [18] and efficient recovery from deep backtracks [19].
The constitutive association of subunits A12.2 and A49/A34.5 may be a symptom of the enzyme’s adaptation to transcribing one specific, extraordinarily long gene. A differential regulation of Pol I transcription similar to the conditional, gene-specific regulation of Pols II and III is most likely not required. Instead, a binary activity switch can be achieved by posttranslational modification of the polymerase or its initiation factors [20,21,22,23].
3 The Pol I Transcription Cycle Visualized In Vitro
Throughout transcription of a DNA template, Pols pass through three main phases, which are more or less conserved throughout various organisms. First, the Pol is recruited to the template sequence, melts the DNA duplex with or without the help of additional factors and begins the synthesis of an RNA strand (initiation ). Thereafter, the initial RNA is extended according to the DNA template strand (elongation ). Finally, Pol dissociates from its DNA template and releases its RNA product (termination ) [24].
The Pol I transcription cycle requires few basic transcription factors [25, 26]. Basal initiation in yeast can be achieved with only the factor Rrn3 and the Core Factor (CF) complex , consisting of proteins Rrn6 , Rrn7 , and Rrn11 [27, 28]. Elongation may involve regulatory factors in vivo, but can commence in vitro without them [25, 26]. Termination finally requires a Myb-domain containing protein, Nsi1 in yeast [29, 30]. Pol I can adopt a dimeric state specific to this enzyme, [31], in which both molecules are inactivated [32] and prevented from binding initiation factors Rrn3 and CF [33,34,35]. Dimerization is reversible [33] and may play a role in storage of Pol I molecules during starvation [36, 37]. Using cryo-EM in many variations, our understanding of the Pol I transcription cycle has been significantly improved in recent years. A structural description of the Pol I transcription cycle allowed a detailed structure–function analysis and the comparison to other transcription systems [38,39,40,41].
Specifically, single-particle cryo-EM analyses showed how Pol I monomers are bound by the initiation factor Rrn3 [42], which allows for recruitment of CF subunit Rrn7 [37, 43, 44] that is related to the general Pol II initiation factor TFIIB [45, 46]. The interaction with Rrn3 prevents the formation of transcriptionally inactive Pol I dimers. In baker’s yeast (Saccharomyces cerevisiae ) Pol I dimerization depends on the specialized, nonconserved “connector” domain of subunit A43, suggesting that this mode of regulation is specific to S. cerevisiae [37]. However, recent cryo-EM studies of Pol I from fission yeast (Schizosaccharomyces pombe ) demonstrated that inactive dimers can form independent of the connector domain utilizing divergent structure elements [47]. It is therefore possible that different organisms evolved different dimer interfaces, but use the same strategy of Pol I hibernation by dimerization during periods of starvation.
Monomeric Pol I bound to Rrn3 can be recruited by promoter-engaged CF . Whereas the structure of CF was determined by X-ray crystallography [48], its interaction with the Pol I–Rrn3 complex was apparently too flexible for this method to succeed. Instead, three independent studies used cryo-EM to visualize a reconstituted initially transcribing complex (ITC) that relies on an artificially stabilized, mismatched transcription bubble with a short initial product RNA [48,49,50]. Comparison of these studies shows that seemingly similar experimental cryo-EM approaches may yield different, though highly complementary results. This demonstrates the influence of sample preparation and experimental conditions on the outcome of a cryo-EM experiment and the strength of single-particle cryo-EM to elucidate dynamic processes. Specifically, some complexes exist in conformations that fail to bind Rrn3 [49], which is required essential to the initiation process and dissociates after promoter escape [42, 51, 52]. These complexes may represent later initiation intermediates. In another structure, the RNA primer is lost and the C-terminal domain of subunit A12.2 is inserted into the funnel domain of Pol I, as would be expected during RNA cleavage events [50]. A third reconstruction showed local resolution differences suggesting high flexibility in distal CF regions [48]. More recently, consolidating structures of close-to-native preinitiation complexes were reported [53, 54]. A closed and an open complex could be reconstructed from a small fraction of recorded particles but yielded important information about the roles of a flexible loop in Rrn3 in CF engagement, and the role of the linker/tWH domain of subunit A49 in template DNA melting, open bubble stabilization, and Rrn3 dissociation [53].
Following initiation , Pol I adopts an actively elongating conformation. This conformation was never successfully crystallized but was reconstructed by single-particle cryo-EM [55, 56]. It is still under debate, whether dissociation/transient association of the A49/A34.5 heterodimer and formation of a 12-subunit polymerase has a physiological function under some circumstances. Chromatin immunoprecipitation (ChIP ) data does not suggest subunit depletion along the 35S gene body in vivo [57], although a lack of density in cryo-EM reconstructions of S. cerevisiae and S. pombe Pol I ECs suggests that subdomain relocation can take place [47, 58]. Upon initiation , the central DNA-binding cleft contracts and tightly binds downstream DNA and the DNA–RNA hybrid region, thus facilitating processive elongation . Contraction upon activation is apparently common to Pol I regulation in different organisms [47] but differs from Pol II [3] and III [59]. The various Pol I EC reconstructions demonstrated the versatile nature of the specific subunits A12.2, A49, and A34.5 [47, 55, 56, 58], and the importance of a Pol I-specific arginine residue in the “bridge-helix” in stalling at DNA lesions caused by UV radiation [60]. Furthermore, the physiological relevance of a contracted Pol I state was confirmed by the 3D-reconstruction of the enzyme from ex vivo purified, actively transcribing Pol I using electron cryo-tomography [55]. Interestingly enough, the underlying preparation technique has been used to describe Pol I functionality since the 1960s [61].
Structural information on transient and highly dynamic states of the Pol I transcription cycle , such as termination , are still lacking to date.
4 Outlook
Continuing investigation of the Pol I transcription system currently aims at defining the structural basis of promoter recruitment in the context of TATA-binding protein [62] and yeast upstream activating factor (UAF) which are important to achieve full initiation levels under physiological conditions [27, 63]. The structural investigations of these complexes and their interplay with the Pol I enzyme will be the key to understand this initiation systems in comparison with Pol II [64, 65] and Pol III [66, 67]. Ultimately, such comparative structure–function analyses will enable us to understand the particular adaptation of the Pol I transcription system to pre-rRNA transcription .
Cryo-EM has now firmly established itself as the method of choice to analyze the structure of such mega-Dalton sized, dynamic, macromolecular complexes. However, the method has also proven to be prone to certain errors. Especially the lack of tools for intrinsic validation of density interpretation may be an issue for initial sequence assignment at resolutions worse than 4 Å. Continuing method development at the experimental and the computational level continues and may soon overcome issues of flexibility and density assignment. For the time being, however, the interpretation of cryo-EM reconstructions should be carefully evaluated and supported by functional data or mutational analysis. Results can also be strengthened by crystallization or small angle X-ray scattering analysis of flexible domains [68], native mass spectrometry [15], hydrogen–deuterium exchange mass-spectrometry evaluation [69], or single-molecule FRET analysis [70]. Especially distance restrains obtained from protein crosslinking coupled to mass spectrometry provides architectural information and may assist low-resolution density assignment [71, 72].
References
Cramer P, Bushnell DA, Kornberg RD (2001) Structural basis of transcription: RNA polymerase II at 2.8 angstrom resolution. Science 292:1863–1876. https://doi.org/10.1126/science.1059493
Armache J-K, Mitterweger S, Meinhart A, Cramer P (2004) Structures of complete RNA polymerase II and its subcomplex, Rpb4/7. J Biol Chem 280(8):7131–7134. https://doi.org/10.1074/jbc.M413038200
Gnatt AL, Cramer P, Fu J, Bushnell DA, Kornberg RD (2001) Structural basis of transcription: an RNA polymerase II elongation complex at 3.3 A resolution. Science 292:1876–1882. https://doi.org/10.1126/science.1059495
Kettenberger H, Armache K-J, Cramer P (2004) Complete RNA polymerase II elongation complex structure and its interactions with NTP and TFIIS. Mol Cell 16:955–965. https://doi.org/10.1016/j.molcel.2004.11.040
Kettenberger H, Armache K-J, Cramer P (2003) Architecture of the RNA polymerase II-TFIIS complex and implications for mRNA cleavage. Cell 114:347–357. https://doi.org/10.1016/S0092-8674(03)00598-1
Wang D, Bushnell DA, Huang X, Westover KD, Levitt M, Kornberg RD (2009) Structural basis of transcription: Backtracked RNA polymerase II at 3.4 Å resolution. Science 324:1203–1206. https://doi.org/10.1126/science.1168729
Liu X, Bushnell DA, Wang D, Calero G, Kornberg RD (2010) Structure of an RNA polymerase II–TFIIB complex and the transcription initiation mechanism. Science 327:206. https://doi.org/10.1126/science.1182015
Sainsbury S, Niesser J, Cramer P (2013) Structure and function of the initially transcribing RNA polymerase II-TFIIB complex. Nature 493:437–440. https://doi.org/10.1038/nature11715
Sainsbury S, Bernecky C, Cramer P (2015) Structural basis of transcription initiation by RNA polymerase II. Nat Rev Mol Cell Biol 16:129–143. https://doi.org/10.1038/nrm3952
McMullan G, Faruqi AR, Henderson R (2016) Direct electron detectors. Methods Enzymol 579:1–17. https://doi.org/10.1016/bs.mie.2016.05.056
Scheres SHW (2012) A Bayesian view on cryo-EM structure determination. J Mol Biol 415:406–418. https://doi.org/10.1016/j.jmb.2011.11.010
Zivanov J, Nakane T, Forsberg B, Kimanius D, Hagen WJH, Lindahl E, Scheres SHW (2018) RELION-3: new tools for automated high-resolution cryo-EM structure determination. bioRxiv. https://doi.org/10.1101/421123
Kühlbrandt W (2014) Biochemistry. The resolution revolution. Science 343:1443–1444. https://doi.org/10.1126/science.1251652
Emsley P, Cowtan K (2004) Coot: model-building tools for molecular graphics. Acta Crystallogr D Biol Crystallogr 60:2126–2132. https://doi.org/10.1107/S0907444904019158
Geiger SR, Lorenzen K, Schreieck A, Hanecker P, Kostrewa D, Heck AJR, Cramer P (2010) RNA polymerase I contains a TFIIF-related DNA-binding subcomplex. Mol Cell 39:583–594. https://doi.org/10.1016/j.molcel.2010.07.028
Kuhn C-D, Geiger SR, Baumli S, Gartmann M, Gerber J, Jennebach S, Mielke T, Tschochner H, Beckmann R, Cramer P (2007) Functional architecture of RNA polymerase I. Cell 131:1260–1272. https://doi.org/10.1016/j.cell.2007.10.051
Merkl PE, Pilsl M, Fremter T, Schwank K, Engel C, Längst G, Milkereit P, Griesenbeck J, Tschochner H (2020) RNA polymerase I (Pol I) passage through nucleosomes depends on Pol I subunits binding its lobe structure. J Biol Chem 295:4782–4795. https://doi.org/10.1074/jbc.RA119.011827
Jennebach S, Herzog F, Aebersold R, Cramer P (2012) Crosslinking-MS analysis reveals RNA polymerase I domain architecture and basis of rRNA cleavage. Nucleic Acids Res 40:5591–5601. https://doi.org/10.1093/nar/gks220
Lisica A, Engel C, Jahnel M, Roldán É, Galburt EA, Cramer P, Grill SW (2016) Mechanisms of backtrack recovery by RNA polymerases I and II. Proc Natl Acad Sci U S A 113:2946–2951. https://doi.org/10.1073/pnas.1517011113
Fath S, Kobor MS, Philippi A, Greenblatt J, Tschochner H (2004) Dephosphorylation of RNA polymerase I by Fcp1p is required for efficient rRNA synthesis. J Biol Chem 279:25251–25259. https://doi.org/10.1074/jbc.M401867200
Clemente-Blanco A, Mayán-Santos M, Schneider DA, Machín F, Jarmuz A, Tschochner H, Aragón L (2009) Cdc14 inhibits transcription by RNA polymerase I during anaphase. Nature 458:219–222. https://doi.org/10.1038/nature07652
Mayer C, Zhao J, Yuan X, Grummt I (2004) mTOR-dependent activation of the transcription factor TIF-IA links rRNA synthesis to nutrient availability. Genes Dev 18:423–434. https://doi.org/10.1101/gad.285504
Hannan KM, Brandenburger Y, Jenkins A, Sharkey K, Cavanaugh A, Rothblum L, Moss T, Poortinga G, McArthur GA, Pearson RB, Hannan RD (2003) mTOR-dependent regulation of ribosomal gene transcription requires S6K1 and is mediated by phosphorylation of the carboxy-terminal activation domain of the nucleolar transcription factor UBF. Mol Cell Biol 23:8862–8877. https://doi.org/10.1128/mcb.23.23.8862-8877.2003
Cheung ACM, Cramer P (2012) A movie of RNA polymerase II transcription. Cell 149:1431–1437. https://doi.org/10.1016/j.cell.2012.06.006
Moss T, Langlois F, Gagnon-Kugler T, Stefanovsky V (2007) A housekeeper with power of attorney: the rRNA genes in ribosome biogenesis. Cell Mol Life Sci 64:29–49. https://doi.org/10.1007/s00018-006-6278-1
Goodfellow SJ, Zomerdijk JCBM (2013) Basic mechanisms in RNA polymerase I transcription of the ribosomal RNA genes. Subcell Biochem 61:211–236. https://doi.org/10.1007/978-94-007-4525-4_10
Keener J, Josaitis CA, Dodd JA, Nomura M (1998) Reconstitution of yeast RNA polymerase I transcription in vitro from purified components. TATA-binding protein is not required for basal transcription. J Biol Chem 273:33795–33802
Milkereit P, Tschochner H (1998) A specialized form of RNA polymerase I, essential for initiation and growth-dependent regulation of rRNA synthesis, is disrupted during transcription. EMBO J 17:3692–3703. https://doi.org/10.1093/emboj/17.13.3692
Reiter A, Hamperl S, Seitz H, Merkl P, Perez-Fernandez J, Williams L, Gerber J, Németh A, Léger I, Gadal O, Milkereit P, Griesenbeck J, Tschochner H (2012) The Reb1-homologue Ydr026c/Nsi1 is required for efficient RNA polymerase I termination in yeast. EMBO J 31:3480–3493. https://doi.org/10.1038/emboj.2012.185
Merkl P, Perez-Fernandez J, Pilsl M, Reiter A, Williams L, Gerber J, Böhm M, Deutzmann R, Griesenbeck J, Milkereit P, Tschochner H (2014) Binding of the termination factor Nsi1 to its cognate DNA site is sufficient to terminate RNA polymerase I transcription in vitro and to induce termination in vivo. Mol Cell Biol 34:3817–3827. https://doi.org/10.1128/MCB.00395-14
Bischler N, Brino L, Carles C, Riva M, Tschochner H, Mallouh V, Schultz P (2002) Localization of the yeast RNA polymerase I-specific subunits. EMBO J 21:4136–4144. https://doi.org/10.1093/emboj/cdf392
Milkereit P, Schultz P, Tschochner H (1997) Resolution of RNA polymerase I into dimers and monomers and their function in transcription. Biol Chem 378:1433–1443
Engel C, Sainsbury S, Cheung AC, Kostrewa D, Cramer P (2013) RNA polymerase I structure and transcription regulation. Nature 502:650–655. https://doi.org/10.1038/nature12712
Fernández-Tornero C, Moreno-Morcillo M, Rashid UJ, Taylor NMI, Ruiz FM, Gruene T, Legrand P, Steuerwald U, Müller CW (2013) Crystal structure of the 14-subunit RNA polymerase I. Nature 502:644–649. https://doi.org/10.1038/nature12636
Kostrewa D, Kuhn C-D, Engel C, Cramer P (2015) An alternative RNA polymerase I structure reveals a dimer hinge. Acta Crystallogr D Biol Crystallogr 71:1850–1855. https://doi.org/10.1107/S1399004715012651
Fernández-Tornero C (2018) RNA polymerase I activation and hibernation: unique mechanisms for unique genes. Transcription 9:248–254. https://doi.org/10.1080/21541264.2017.1416267
Torreira E, Louro JA, Pazos I, González-Polo N, Gil-Carton D, Duran AG, Tosi S, Gallego O, Calvo O, Fernández-Tornero C (2017) The dynamic assembly of distinct RNA polymerase I complexes modulates rDNA transcription. elife 6:e20832. https://doi.org/10.7554/eLife.20832
Hanske J, Sadian Y, Müller CW (2018) The cryo-EM resolution revolution and transcription complexes. Curr Opin Struct Biol 52:8–15. https://doi.org/10.1016/j.sbi.2018.07.002
Engel C, Neyer S, Cramer P (2018) Distinct mechanisms of transcription initiation by RNA polymerases I and II. Annu Rev Biophys 47:425–446. https://doi.org/10.1146/annurev-biophys-070317-033058
Jochem L, Ramsay EP, Vannini A (2017) RNA polymerase I, bending the rules? EMBO J 36:2664–2666. https://doi.org/10.15252/embj.201797924
Jackobel AJ, Han Y, He Y, Knutson BA (2018) Breaking the mold: structures of the RNA polymerase I transcription complex reveal a new path for initiation. Transcription 9:255–261. https://doi.org/10.1080/21541264.2017.1416268
Blattner C, Jennebach S, Herzog F, Mayer A, Cheung ACM, Witte G, Lorenzen K, Hopfner K-P, Heck AJR, Aebersold R, Cramer P (2011) Molecular basis of Rrn3-regulated RNA polymerase I initiation and cell growth. Genes Dev 25:2093–2105. https://doi.org/10.1101/gad.17363311
Engel C, Plitzko J, Cramer P (2016) RNA polymerase I-Rrn3 complex at 4.8 Å resolution. Nat Commun 7:12129. https://doi.org/10.1038/ncomms12129
Pilsl M, Crucifix C, Papai G, Krupp F, Steinbauer R, Griesenbeck J, Milkereit P, Tschochner H, Schultz P (2016) Structure of the initiation-competent RNA polymerase I and its implication for transcription. Nat Commun 7:12126. https://doi.org/10.1038/ncomms12126
Knutson BA, Hahn S (2011) Yeast Rrn7 and human TAF1B are TFIIB-related RNA polymerase I general transcription factors. Science 333:1637–1640. https://doi.org/10.1126/science.1207699
Naidu S, Friedrich JK, Russell J, Zomerdijk JCBM (2011) TAF1B is a TFIIB-like component of the basal transcription machinery for RNA polymerase I. Science 333:1640–1642. https://doi.org/10.1126/science.1207656
Heiss FB, Daiß JL, Becker P, Engel C (2021) Conserved strategies of RNA polymerase I hibernation and activation. Nat Commun 12:758. https://doi.org/10.1038/s41467-021-21031-8
Engel C, Gubbey T, Neyer S, Sainsbury S, Oberthuer C, Baejen C, Bernecky C, Cramer P (2017) Structural basis of RNA polymerase I transcription initiation. Cell 169:120–131.e22. https://doi.org/10.1016/j.cell.2017.03.003
Han Y, Yan C, Nguyen THD, Jackobel AJ, Ivanov I, Knutson BA, He Y (2017) Structural mechanism of ATP-independent transcription initiation by RNA polymerase I. elife 6:e27414. https://doi.org/10.7554/eLife.27414
Sadian Y, Tafur L, Kosinski J, Jakobi AJ, Wetzel R, Buczak K, Hagen WJ, Beck M, Sachse C, Müller CW (2017) Structural insights into transcription initiation by yeast RNA polymerase I. EMBO J 36:2698–2709. https://doi.org/10.15252/embj.201796958
Bier M, Fath S, Tschochner H (2004) The composition of the RNA polymerase I transcription machinery switches from initiation to elongation mode. FEBS Lett 564:41–46. https://doi.org/10.1016/S0014-5793(04)00311-4
Herdman C, Mars J-C, Stefanovsky VY, Tremblay MG, Sabourin-Felix M, Lindsay H, Robinson MD, Moss T (2017) A unique enhancer boundary complex on the mouse ribosomal RNA genes persists after loss of Rrn3 or UBF and the inactivation of RNA polymerase I transcription. PLoS Genet 13:e1006899. https://doi.org/10.1371/journal.pgen.1006899
Sadian Y, Baudin F, Tafur L, Murciano B, Wetzel R, Weis F, Müller CW (2019) Molecular insight into RNA polymerase I promoter recognition and promoter melting. Nat Commun 10:5543. https://doi.org/10.1038/s41467-019-13510-w
Pilsl M, Engel C (2020) Structural basis of RNA polymerase I pre-initiation complex formation and promoter melting. Nat Commun 11:1206. https://doi.org/10.1038/s41467-020-15052-y
Neyer S, Kunz M, Geiss C, Hantsche M, Hodirnau V-V, Seybert A, Engel C, Scheffer MP, Cramer P, Frangakis AS (2016) Structure of RNA polymerase I transcribing ribosomal DNA genes. Nature 540(7634):607–610. https://doi.org/10.1038/nature20561
Tafur L, Sadian Y, Hoffmann NA, Jakobi AJ, Wetzel R, Hagen WJH, Sachse C, Müller CW (2016) Molecular structures of transcribing RNA polymerase I. Mol Cell 64:1135–1143. https://doi.org/10.1016/j.molcel.2016.11.013
Beckouet F, Labarre-Mariotte S, Albert B, Imazawa Y, Werner M, Gadal O, Nogi Y, Thuriaux P (2008) Two RNA polymerase I subunits control the binding and release of Rrn3 during transcription. Mol Cell Biol 28:1596–1605. https://doi.org/10.1128/MCB.01464-07
Tafur L, Sadian Y, Hanske J, Wetzel R, Weis F, Müller CW (2019) The cryo-EM structure of a 12-subunit variant of RNA polymerase I reveals dissociation of the A49-A34.5 heterodimer and rearrangement of subunit A12.2. elife 8:e43204. https://doi.org/10.7554/eLife.43204
Hoffmann NA, Jakobi AJ, Moreno-Morcillo M, Glatt S, Kosinski J, Hagen WJH, Sachse C, Müller CW (2015) Molecular structures of unbound and transcribing RNA polymerase III. Nature 528:231–236. https://doi.org/10.1038/nature16143
Sanz-Murillo M, Xu J, Belogurov GA, Calvo O, Gil-Carton D, Moreno-Morcillo M, Wang D, Fernández-Tornero C (2018) Structural basis of RNA polymerase I stalling at UV light-induced DNA damage. Proc Natl Acad Sci U S A 115:8972–8977. https://doi.org/10.1073/pnas.1802626115
Miller OL, Beatty BR (1969) Visualization of nucleolar genes. Science 164:955–957. https://doi.org/10.1126/science.164.3882.955
Kramm K, Engel C, Grohmann D (2019) Transcription initiation factor TBP: old friend new questions. Biochem Soc Trans 47:411–423. https://doi.org/10.1042/BST20180623
Bedwell GJ, Appling FD, Anderson SJ, Schneider DA (2012) Efficient transcription by RNA polymerase I using recombinant core factor. Gene 492:94–99. https://doi.org/10.1016/j.gene.2011.10.049
Schilbach S, Hantsche M, Tegunov D, Dienemann C, Wigge C, Urlaub H, Cramer P (2017) Structures of transcription pre-initiation complex with TFIIH and mediator. Nature 551:204–209. https://doi.org/10.1038/nature24282
He Y, Yan C, Fang J, Inouye C, Tjian R, Ivanov I, Nogales E (2016) Near-atomic resolution visualization of human transcription promoter opening. Nature 533:359–365. https://doi.org/10.1038/nature17970
Abascal-Palacios G, Ramsay EP, Beuron F, Morris E, Vannini A (2018) Structural basis of RNA polymerase III transcription initiation. Nature 553:301–306. https://doi.org/10.1038/nature25441
Vorländer MK, Khatter H, Wetzel R, Hagen WJH, Müller CW (2018) Molecular mechanism of promoter opening by RNA polymerase III. Nature 553:295–300. https://doi.org/10.1038/nature25440
Ramsay EP, Abascal-Palacios G, Daiß JL, King H, Gouge J, Pilsl M, Beuron F, Morris E, Gunkel P, Engel C, Vannini A (2020) Structure of human RNA polymerase III. Nat Commun 11:6409. https://doi.org/10.1038/s41467-020-20262-5
Shukla AK, Westfield GH, Xiao K, Reis RI, Huang L-Y, Tripathi-Shukla P, Qian J, Li S, Blanc A, Oleskie AN, Dosey AM, Su M, Liang C-R, Gu L-L, Shan J-M, Chen X, Hanna R, Choi M, Yao XJ, Klink BU, Kahsai AW, Sidhu SS, Koide S, Penczek PA, Kossiakoff AA, Woods VL, Kobilka BK, Skiniotis G, Lefkowitz RJ (2014) Visualization of arrestin recruitment by a G-protein-coupled receptor. Nature 512:218–222. https://doi.org/10.1038/nature13430
Kramm K, Schröder T, Gouge J, Vera AM, Gupta K, Heiss FB, Liedl T, Engel C, Berger I, Vannini A, Tinnefeld P, Grohmann D (2020) DNA origami-based single-molecule force spectroscopy elucidates RNA polymerase III pre-initiation complex stability. Nat Commun 11:2828. https://doi.org/10.1038/s41467-020-16702-x
Leitner A, Faini M, Stengel F, Aebersold R (2016) Crosslinking and mass spectrometry: an integrated technology to understand the structure and function of molecular machines. Trends Biochem Sci 41:20–32. https://doi.org/10.1016/j.tibs.2015.10.008
Schmidt C, Urlaub H (2017) Combining cryo-electron microscopy (cryo-EM) and cross-linking mass spectrometry (CX-MS) for structural elucidation of large protein assemblies. Curr Opin Struct Biol 46:157–168. https://doi.org/10.1016/j.sbi.2017.10.005
Acknowledgements
The authors thank all members of the Structural Biochemistry group and Biochemistry I/III departments of the University of Regensburg for help and discussions. This work was supported by the Emmy-Noether-Programme (DFG grant no. EN 1204/1-1 to CE) and SFB 960 TP-A8.
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Pilsl, M., Engel, C. (2022). Structural Studies of Eukaryotic RNA Polymerase I Using Cryo-Electron Microscopy. In: Entian, KD. (eds) Ribosome Biogenesis. Methods in Molecular Biology, vol 2533. Humana, New York, NY. https://doi.org/10.1007/978-1-0716-2501-9_5
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DOI: https://doi.org/10.1007/978-1-0716-2501-9_5
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Publisher Name: Humana, New York, NY
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