- About this Journal ·
- Abstracting and Indexing ·
- Aims and Scope ·
- Article Processing Charges ·
- Articles in Press ·
- Author Guidelines ·
- Bibliographic Information ·
- Citations to this Journal ·
- Contact Information ·
- Editorial Board ·
- Editorial Workflow ·
- Free eTOC Alerts ·
- Publication Ethics ·
- Reviewers Acknowledgment ·
- Submit a Manuscript ·
- Subscription Information ·
- Table of Contents
Volume 2013 (2013), Article ID 614735, 14 pages
Ribonucleoproteins in Archaeal Pre-rRNA Processing and Modification
1Department of Molecular Biophysics and Biochemistry, Yale University School of Medicine, New Haven, CT 06510, USA
2Department of Microbial Pathogenesis, Yale University School of Medicine, New Haven, CT 06510, USA
3Department of Therapeutic Radiology, Yale University School of Medicine, New Haven, CT 06510, USA
4Department of Genetics, Yale University School of Medicine, New Haven, CT 06510, USA
Received 12 October 2012; Revised 9 January 2013; Accepted 15 January 2013
Academic Editor: Anita Marchfelder
Copyright © 2013 W. S. Vincent Yip et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.
Given that ribosomes are one of the most important cellular macromolecular machines, it is not surprising that there is intensive research in ribosome biogenesis. Ribosome biogenesis is a complex process. The maturation of ribosomal RNAs (rRNAs) requires not only the precise cleaving and folding of the pre-rRNA but also extensive nucleotide modifications. At the heart of the processing and modifications of pre-rRNAs in Archaea and Eukarya are ribonucleoprotein (RNP) machines. They are called small RNPs (sRNPs), in Archaea, and small nucleolar RNPs (snoRNPs), in Eukarya. Studies on ribosome biogenesis originally focused on eukaryotic systems. However, recent studies on archaeal sRNPs have provided important insights into the functions of these RNPs. This paper will introduce archaeal rRNA gene organization and pre-rRNA processing, with a particular focus on the discovery of the archaeal sRNP components, their functions in nucleotide modification, and their structures.
Without ribosomes, cells cannot grow and divide. Thus, it is not surprising that ribosomes have been selectively conserved through millennia and are one of the few macromolecular machines present in all three domains of life. Having been under such tight selective pressure, ribosomes have been and continue to be used in establishing phylogenetic relationships through one specific component, the 16S rRNA in Bactria and Archaea and the 18S rRNA in Eukarya [1–3]. This led scientists to uncover that instead of only “prokaryotes” and “eukaryotes,” there is an additional third domain that would become the Archaea [4, 5].
Ribosome biogenesis and processing begins with ribosomal gene organization. This paper will cover both the genome organization of various rRNA operons in Archaea as well as the small ribonucleoproteins (sRNPs) responsible for chemical modification of nucleotides on the rRNA. In particular, the two most abundant types of chemical modifications are mediated by box C/D and box H/ACA sRNPs. It is not yet well understood why these nucleotides are chemically modified. In considering these modifications of rRNA, it is first important to understand why ribosomes are essential, how Archaea are unique, and how their ribosomal RNA loci are organized in the genome.
2. Ribosomes and rRNA
Ribosomes are essential for the translation of mRNA into a polypeptide chain that is then folded into a functional protein . These cellular machines are not only comprised of rRNA (transcribed from ribosomal DNA, rDNA), but also a number of ribosomal proteins that are required for the correct structure and function of the ribosome . Ribosome biogenesis is a very energy-intensive process  and requires a host of proteins and RNA modifications. In an actively growing Saccharomyces cerevisiae cell, transcription of the rRNA genes can account for up to 60% of total cellular transcription; additionally, the processing of ribosomal proteins takes up to 90% of mRNA splicing activities within the actively growing cell . Considering that ribosomes are essential, it is not surprising that they are selectively conserved. As previously mentioned, rRNA has proven to be very helpful in establishing evolutionary relationships of almost all known organisms, both microscopic and macroscopic [1–3].
3. Ribosomal Architecture
All ribosomes are comprised of a large and small subunit; while the subunits differ in structure across the evolutionary domains, they share a common function. The small subunit (SSU) contains one rRNA in all organisms (16S in Bacteria and Archaea, 18S in Eukarya). Each also has a large subunit (LSU) that in eukaryotes is comprised of the 28S (25S in S. cerevisiae), 5.8S, and 5S rRNAs, while in Bacteria and Archaea is composed of the 23S and 5S rRNAs (Table 1). In addition to these rRNAs, ribosomal proteins account for part of the mass of each subunit. For example, the prokaryotic SSU has a 16S rRNA, but sediments at 30S in a sucrose gradient. While the 70S prokaryotic ribosome contains a 50S LSU and 30S SSU, the eukaryotic ribosome is 80S, with a 60S LSU and 40S SSU .
4. Archaea: An Independent Monophyletic Grouping
Relative to rRNA sequence, Archaea are phylogenetically distinct from Bacteria and Eukarya (Figure 1). Archaea have ribosomes that are structurally similar to bacterial ribosomes: the LSU contains a 23S and 5S rRNA while the SSU contains a 16S rRNA. While the domains Bacteria and Eukarya are well studied and understood, the members of Archaea remain more of a mystery, especially considering that organisms with extreme growth requirements are often contained within the domain. Hyperthermophilic, psychrophilic, halophilic, and even piezophilic organisms are all contained within the Archaea.
Considering the diversity of organisms that comprise the archaeal domain, it is not surprising that they represent strong candidates for biological research. It is essential that scientists continue to emphasize that the Archaea do in fact stand alone as a domain and contain phyla and biological divisions that are just as structured and inclusive as the other domains (Figure 1, Table 1). With biochemical and structural features that are so unique to Archaea (i.e., cell wall and lipid differences between Archaea and the other domains; see  for an early account of the differences) it is easy to understand that they represent a wealth of knowledge waiting to be uncovered. One particular area of interest lies in biotechnological applications of Archaea .
5. rRNA Operon Number and Organization across Archaea
5.1. rRNA Operon Number across Archaea
Within the Archaea, there is great variation in the number of rrn genes encoding the 23S, 16S, and 5S ribosomal RNAs. There are one to four copies of the 16S rrn gene in diverse archaeal species, with over half of the sequenced genomes having only one, which lies in contrast to the one to fifteen copies that can be found in bacterial species [14, 15]. Specifically, approximately 20% of sequenced bacterial genomes have one copy of the 16S rrn gene, while 11% have greater than eight [14, 15]. The fact that there is often more than one repeat of these genes in organisms that typically are monoallelic for other genes underlies the importance of the rrn genes and the essential requirement for an abundant supply of properly functioning ribosomes. Additionally, all sequenced Crenarchaeota, Nanoarchaeota, and Korarchaeota have only one copy of the 16S rRNA gene, so that any species with more than one copy of the 16S rRNA gene belongs to the Euryarchaeota . Although rDNA gene number and organization varies across archaeal species, the reason for such organization remains unknown.
5.2. Polycistronic Transcription of rRNA Genes in Archaea
In several species of Archaea, the 16S, 23S, and 5S rRNAs exist in a continuous polycistronic operon. In this organization, the 16S, 23S, and 5S rRNA genes are transcribed as a single transcript and then excised via an archaeal-specific splicing mechanism (Figure 2). An example of the polycistronic transcription of rRNA operons is in the model archaeon, Haloferax volcanii. Intriguingly, H. volcanii has two full copies of the rRNA operons that each contains a copy of the 16S, 23S, and 5S rRNAs . Another example of polycistronic transcription of rRNA genes is in Halobacterium cutirubrum, which has been reported to contain a single copy of rRNA genes encoded in one operon encoding the 16S, tRNAAla, 23S, 5S, tRNACys . This setup is typical of what is seen in the Euryarchaeota (Figure 2) . As in H. cutirubrum, the archaeal rRNA operons often contain tRNA genes interspersed between the rRNA genes. This represents a clear way to ensure that certain tRNA genes are transcribed. For information on the presence, number, and organization of tRNA genes, see [14, 15].
5.3. Partial Uncoupling of Transcription of rRNA Genes in Archaea
While a polycistronic operon would seem to be an efficient way to transcribe archaeal rRNAs, other gene organizations exist as well. There is no shortage of examples that represent variations on a theme of rRNA gene organization in Archaea. For example, Thermoproteus tenax and Desulfurococcus mobilis, both members of the Crenarchaeota, have an operon containing the 16S, and 23S rRNA genes but not including the 5S genes, which are found under the control of a different promoter at an alternative locus in the genome [44, 45]. Sulfolobus solfataricus, a model archaeal organism, also has this operon architecture . Moreover, Thermus thermophilus processes the 23S and 5S rRNA genes together within an operon, with the 16S rRNA gene located elsewhere in the genome . Most interesting of the partially uncoupled operons is Methanococcus jannaschii, which contains two copies of the genes for the 16S, 23S, and 5S rRNAs. In this species, there is one 16S/23S/5S operon (Operon A) and a 16S/23S operon (Operon B) that is uncoupled from the second 5S gene .
5.4. Complete Uncoupling of Transcription of rRNA Genes in Archaea
Some archaeal species do not have any operon organization of their rRNA genes but instead have three separate genes at three separate locations under three separate promoters, each encoding the 23S, 16S, and 5S rRNAs. Examples of such species are Thermoplasma acidophilum, the first archaeal organism to be discovered with this rRNA genome organization , and Nanoarchaeum equitans . It should be noted that in N. equitans, there is also a dispersal of ribosomal proteins throughout the genome that are found in close proximity not only in other archaeal species of other phyla, but also in the Bacteria . In N. equitans, the uniqueness of this organism as the only known member of the Nanoarchaeota phylum can explain the unique genome organization, but this alone cannot be used as an umbrella explanation for the separate 23S, 16S, and 5S organization since it is also found in T. acidophilum.
Since all of the rRNA components (i.e., 23S, 16S, and 5S) are required to assemble a functioning ribosome, what are the reasons, if any, in uncoupling transcription in each component in the rRNA unit? Similarly, what are the reasons for partially uncoupling the operons as is seen in M. janaschii? Further research will be required to understand archaeal rRNA gene organization and why some organisms have polycistronic transcription, while others have transcriptional uncoupling of rRNA synthesis.
6. Introns within Archaeal rRNA Genes
In addition to variation in the number and organization of the rRNA genes throughout genomes, there is also variation amongst Archaea in terms of intronic sequences found within the rRNA sequences. While Bacteria do not contain introns within the genes for the 23S, 16S, and 5S RNAs, some archaeal species, in fact, do. Intronic sequences in the 23S ribosomal RNA gene were first described in Desulfurococcus mobilis with a mechanism of splicing unique to Archaea . Interestingly, there have even been reports of 23S rRNA genes containing two introns of approximately equal length in Staphylothermus marinus . Moreover, there have also been reports of introns found within the 16S rRNA gene. The presence of an intron in Pyrobaculum aerophilum, but not the closely related Pyrobaculum islandicum, was the first report of an intron found in a 16S rRNA gene .
Many of these archaeal rDNA introns contain putative open reading frames that often lack sequence similarity to known proteins [20–22]. There have, however, been reports of these sequences coding for proteins, such as the site-specific endonuclease I-DmoI found in the intron of the 23s rRNA of Desulfurococcus mobilis [23, 24]. More research will be required to see whether there are additional examples of functional proteins or noncoding RNAs produced from these introns or whether these are simply few isolated cases. Their origin is also interesting considering that Bacteria do not contain intronic sequences in these genes.
Excision of introns in Archaea takes part through an archaeal-specific splicing mechanism  via-archaeal specific endonucleases, which is unusual since Archaea do not contain Group I or Group II introns . The hallmark of this splicing reaction is the recognition of the bulge-helix-bulge motif that is found at the intron-exon junction [38, 53] (for more on archaeal splicing, see [11, 21, 53–55]). The presence of introns in archaeal rRNA genes suggests that, while the ribosomes and rRNAs are more similar to the Bacteria in structure, their processing and even, at times, gene organization (i.e., presence of introns in the rRNA genes) is more similar to Eukarya. This is one of many aspects of Archaea that truly identifies the domain as independent and part of neither the bacterial nor eukaryotic groupings.
7. RNA-Guided rRNA Modifications and Guide Small RNPs in Archaea
Certain rRNA processing events in Archaea are similar to those in Eukarya. Indeed, similar to eukaryotic rRNAs, archaeal rRNAs are heavily modified. rRNAs from eukaryotes such as S. cerevisiae contain ~100 modifications (Table 1) [34, 37–40]. Archaeal rRNAs contain a comparable number of modifications [36–38, 56]. For instance, S. solfataricus has ~70 modifications in the rRNAs . In direct contrast, bacterial rRNAs are modified to a much lesser extent, containing merely ~40 modifications (most of which are base modifications) [34, 37, 38, 40, 41].
The two major types of chemical modifications in rRNAs are the methylation of the 2′ hydroxyl group, known as 2′-O-methylations (Nms), and the isomerization of the uridine base into pseudouridine, known as pseudouridylation () (Figure 3). There are two mechanisms for chemically modifying rRNA: site-specific enzyme catalysis or RNA-guided catalysis [29–35]. While all of the rRNA chemical modifications in Bacteria are catalyzed by site-specific enzymes, most modifications in Archaea are achieved by RNA-guided RNP complexes [34, 35, 56–59].
In fact, these RNA-guided nucleotide modification machines are only present in the Archaea and Eukarya and absent in Bacteria [26–35, 56–60]. These machines, known as small ribonucleoproteins (sRNPs) in Archaea and small nucleolar ribonucleoproteins (snoRNPs) in Eukarya, are named after the small RNAs (sRNAs) in Archaea and small nucleolar RNAs (snoRNAs) in Eukarya. There are two types of s(no)RNPs: box C/D s(no)RNPs and box H/ACA s(no)RNPs, which carry out 2′-O-methylation and pseudouridylation, respectively [26–28, 30–33, 60]. Within a functional type of sRNP, the protein components are the same but the sRNAs differ. Thus, the sRNA provides the specificity of the nucleotide modification [26–28, 30–33, 60]. Hence, the sRNAs are often referred to as guide RNAs.
8. Discovery of Archaeal sno-Like RNAs
The discovery that archaeal rRNAs contain a comparable number of chemical modifications as eukaryotic rRNAs prompted a search for sno-like guide RNAs (sRNAs) in Archaea. Both computational and experimental approaches have been used to detect guide sRNAs in various archaeal species [42, 43, 61–67]. Computational approaches used to identify these sRNAs take advantage of the conserved length and sequence elements and homologies with known snoRNAs or sRNAs in other eukaryotes and Archaea [63, 65, 67]. However, the relatively small sizes of the conserved sequence features of the sRNAs and the low degree of conservation of the sequence outside these features have presented challenges to the identification of sRNAs in Archaea. Therefore, other algorithms have been developed to identify candidate sRNAs [62, 67].
Alternatively, experimental approaches can be used to search for archaeal sRNAs. Some approaches make use of Sanger sequencing of a size-selected cDNA library derived from total archaeal RNA [42, 64]. Others take advantage of the fact that the guide sRNAs form sRNP complexes and use immunoprecipitation methods to isolate the sRNAs [43, 61]. Recently, advances in nucleic acid sequencing technologies have allowed the direct sequencing of the selectively enriched stable RNA species from total RNA of N. equitans .
The combination of computational and experimental approaches presents a powerful means to identify putative guide sRNAs. These approaches have led to the discovery of over one hundred candidate guide sRNAs from various archaeal species in the Euryarchaeota, Crenarchaeota, and Nanoarchaeota phyla [42, 43, 61–67]. Interestingly, in approaches where both box C/D and H/ACA sRNAs were identified, the number of sRNAs of the H/ACA type is usually fewer than those of the C/D type [43, 64, 66]. This correlates with the finding that archaeal rRNAs usually have fewer pseudouridylations than 2′-O-methylations [35, 36, 38]. Alternatively, however, these may also be a result of the bias inherent in the approaches being used .
Whether the majority of archaeal guide sRNAs can assemble into catalytically active sRNPs is not known. The existence of many candidate sRNAs discovered using experimental approaches has been confirmed by either northern blots or by primer extension [42, 43, 61–65]. Some predicted sRNAs have been shown experimentally to be able to assemble into sRNPs which are catalytically active [26, 43, 65, 67–69]. In addition, the predicted target sites of some candidate guide sRNAs have been confirmed to be modified [42, 43, 61, 63–65, 67]. In contrast, many putative sRNAs are orphan sRNAs with no known predicted target sites [42, 43, 61–67], so it remains unclear whether they are bona fide guide sRNAs. Moreover, because current computational and experimental approaches rely heavily on previously known structures and sequence features of the sRNAs, many potential guide sRNAs may have been overlooked . Nevertheless, the identification of candidate sRNAs permits a general understanding of their sequence and structural features and is the first step in characterizing them and their sRNPs in Archaea.
9. Properties and Secondary Structures of Box C/D sRNA
Archaeal box C/D sRNAs are typically ~50–60 nt long [42, 43, 59, 61, 64, 66]. The sRNA is a critical component in the catalysis of 2′-O-methylation. It contains two consensus sequence elements, boxes C (RUGAUGA) and D (CUGA), located near the 5′ and 3′ termini of the RNA, respectively (Figure 4(a)) [42, 43, 56–59, 61–64, 66]. In addition, it also contains two similar sequence elements, C′ and D′, in its internal region [42, 43, 56–59, 61–64, 66]. Boxes C and D form noncanonical GA:AG sheared pairs . The 5′ region of box C is a 3 nt asymmetric bulge. The GA:AG sheared pairs and the 3 nt asymmetric bulge allow the formation of a kink between the noncanonical stem formed by the box C/D motif and the canonical stem formed between the 5′ and 3′ termini [70, 71]. This motif is known as the kink-turn motif and is a structural feature of the box C/D sRNA [70, 71]. Similarly, boxes C′ and D′ also form a kink-turn-like motif . However, instead of a stem-kink-stem structure, the boxes C′/D′ form a stem-kink-loop structure, known as the kink-loop motif .
The C/D and C′/D′ motifs are separated by two unpaired strands of RNA [42, 43, 61–67]. These regions contain the guide sequences. The guide sequences 5′ to box D and to box D′ are, respectively, known as the D and the D′ guides. They form Watson-Crick base-pairs with the substrate RNAs [26, 31–33, 37, 56, 58, 59]. Base-pairing between the guide RNA and its substrate(s) allows the substrate(s) to be specifically 2′-O-methylated at a site that is five nucleotides 5′ from box D or D′. Intriguingly, in the several archaeal species examined, the unpaired sequences separating the C/D and C′/D′ motifs have a conserved length of 10–12 nt . The maintenance of this length has been demonstrated to be essential for 2′-O-methylation .
10. Box C/D sRNPs
Box C/D s(no)RNPs carry out site-specific 2′-O-methylation of pre-rRNAs. The minimal components required to make a functional box C/D s(no)RNP were revealed when a catalytically active box C/D sRNP was reconstituted in vitro for the first time using recombinant S. solfataricus proteins and in vitro transcribed S. acidocaldarius sRNA by Omer et al. . The catalytically active sRNP is composed of three protein components, L7Ae, Nop5, and fibrillarin, and an sRNA component (Figure 5) . These three proteins and the sRNA constitute the core sRNP complex that is the minimal set of components necessary for catalytic activity in vitro . It is unclear whether other factors associate with the core complex for optimal assembly or catalytic activity in vivo .
Since the first in vitro reconstitution of the core box C/D sRNP, its structure and biochemistry have been extensively studied [16, 17, 26, 68, 70, 73–90]. The L7Ae protein, which is also a large ribosomal subunit protein in Archaea, binds the kink-turn or kink-loop motif of the sRNA formed by boxes C/D and by boxes C′/D′ [17, 26, 70, 75, 76, 78, 79, 86, 87]. Each individual kink-turn or kink-loop motif allows the binding of one L7Ae protein [78, 79]. Therefore, one single sRNA allows the binding of two copies of the protein. The binding of L7Ae is required for the assembly of Nop5, and fibrillarin [26, 78, 79]. Without the binding of L7Ae, Nop5 and fibrillarin have little to no binding affinity for the sRNA [26, 79]. Nop5 contains a coiled coil domain that allows homodimerization [77, 81, 84]. It also interacts with a fibrillarin in vitro to form a Nop5/fibrillarin heterodimer [77, 80, 81]. Two Nop5/fibrillarin heterodimers further dimerize to form a heterotetramer [77, 80, 84]. Therefore, Nop5 and fibrillarin may assemble onto the sRNP complex in a tetrameric form . Because fibrillarin contains an S-adenosylmethionine (SAM) binding pocket and has a conserved SAM-dependent methyltransferase fold [74, 77, 80, 84, 91], it is suggested to be the catalytic enzyme for 2′-O-methylation. Mutations in S. solfataricus and S. cerevisiae fibrillarin result in a loss of sRNP 2′-O-methylation activity [26, 92].
Structural studies of archaeal box C/D sRNP individual core proteins, protein-protein, and protein-RNA complexes have revealed important structural features that are essential for assembly and catalysis [16, 68, 70, 74, 77, 84, 86, 89]. A cocrystal structure of L7Ae and a minimal box C/D sRNA confirmed the formation of a kink-turn motif and the importance of this motif in the binding of the L7Ae protein . Crystal structures and biochemical studies of Nop5/fibrillarin complexes as well as a partial C/D sRNP complex assembled with L7Ae, Nop5, fibrillarin, and a half-mer box C/D sRNA revealed the importance of Nop5 protein as a protein bridge [77, 84, 86, 87]. The C-terminal domain (CTD) of the Nop5 protein contacts the composite surface formed by L7Ae and the sRNA while the N-terminal domain (NTD) of Nop5 interacts with fibrillarin [77, 84, 86, 87]. Furthermore, the coiled coil domain of Nop5 provides an interaction surface with another Nop5 protein, which serves as a mediator between the proteins assembled on two different box C/D motifs. Importantly, cocrystal structures of Nop5/fibrillarin complexes from different species as well as a partial C/D sRNP complex have suggested that there is a flexible hinge region in the Nop5 protein, around which the NTD moves [77, 84, 87]. This hinge region may also allow movement of the associated fibrillarin enzyme, allowing efficient catalysis upon substrate binding.
Recently, the structure of a complete, catalytically active box C/D sRNP was successfully reconstructed for M. jannaschii using negative staining electron microscopy (EM) [68, 89]. Unexpectedly, this structure is a dimeric sRNP structure (di-sRNP) (Figure 5(a)), which is further supported by extensive biochemical evidence [68, 93]. In the di-sRNP model, rather than having two sets of the three core proteins associated with a single sRNA, a complete box C/D sRNP is composed of four sets of the core proteins associated with two sRNAs (Figure 5(a)). Intriguingly, the docking of crystal structures of the core proteins into the di-sRNP volume also suggested that the Nop5 dimers act as a bridge between the L7Ae and fibrillarin proteins assembled on the box C/D motif of one sRNA with those assembled on the box C′/D′ motif of a different sRNA. Thus, the sRNA does not run parallel to the Nop5 dimer (Figure 5(a)). While the relatively low resolution of the EM reconstruction does not provide atomic details, it does present a novel model of how the box C/D sRNP may carry out catalysis.
The di-sRNP model has been challenged by the crystal structure of a fully assembled sRNP from S. solfataricus that contains a substrate RNA . In contrast to the di-sRNP structure, the crystal structure suggests that a complete sRNP complex is composed of two sets of the three core proteins assembled on a single sRNA (Figure 5(b)). This model, which is referred to as the mono-sRNP model, not only contrasts with the di-sRNP model in terms of oligomeric state of the complex but also suggests a different orientation of the proteins and sRNA in the complex. While the Nop5 dimer connects the box C/D (C′/D′) motifs from two sRNAs in the di-sRNP structure, the dimer connects the box C/D (C′/D′) motifs from the same sRNA in the mono-sRNP structure (Figure 5). The sRNA, therefore, runs parallel to the Nop5 dimer in the mono-sRNP model, which is distinct from the di-sRNP model.
It was surprising that box C/D sRNPs from different archaeal species with very conserved protein components can adopt such diverse structures. One explanation may lie in the different sRNAs used. In the di-sRNP structure, a natural sRNA made of a single continuous strand containing both kink-turn and kink-loop motifs was used [68, 89]. In contrast, in the mono-sRNP structure, a nonnatural sRNA made of two strands of RNA, containing two kink-turn motifs and lacking an internal loop, was used . This seemingly slight difference in the presence of the loop of the sRNA induces different sRNP structures as demonstrated by native gel experiments . While the natural sRNA, with the internal loop, forms only the di-sRNP species, the use of a nonnatural sRNA, lacking an internal loop, leads to the formation of a mixed population of both mono- and di-sRNP species . Protein components from four different archaeal species assemble both mono- and di-sRNPs, depending on the sRNA .
Since the di-sRNP structure contains a physiological sRNA, it will be important to determine whether it changes conformation upon binding of substrate RNA. While the crystal structure of the mono-sRNP complex provides information about substrate RNA interactions, it remains unclear how the di-sRNP structure changes conformation upon substrate binding. Because the orientation of the proteins and sRNA is fundamentally different between the mono- and the di-sRNPs, different conformational changes might therefore be expected upon substrate binding. Further structural studies on the box C/D di-sRNP complex assembled using a natural sRNA in the presence of the substrate RNA need to be performed to understand the conformational changes associated with RNA methylation catalysis.
11. Properties and Secondary Structures of Box H/ACA sRNA
The box H/ACA sRNA is the sRNA component of the box H/ACA sRNP that catalyzes pseudouridylation. Most archaeal box H/ACA sRNAs consist of a ~65–75 nt single hairpin structure which is immediately followed by the consensus sequence ANANNA (box H) or ACA (box ACA) (Figure 4(b)) [37, 43, 59, 61, 64, 66]. However, box H/ACA sRNA containing two or three hairpins have also been reported in Archaea [64–66]. Similar to the archaeal box C/D sRNA, box H/ACA sRNA also contains a kink-turn or a kink-loop motif in the internal region of the RNA [64–66]. In the middle of the hairpin, there are two unpaired strands. These sequences can form two 4–8 nt duplexes with the substrate RNA where the site of modification remains unpaired and sandwiched between the two duplexes (Figure 4(b)) [27, 28, 30, 58–60, 94, 95]. This bipartite loop structure is known as the pseudouridylation pocket. The site of pseudouridylation is ~14–16 nt away from the box H or box ACA [27, 28, 30, 60].
12. Box H/ACA sRNPs
Box H/ACA s(no)RNPs direct site-specific pseudouridylations in pre-rRNAs. The first significant advance in our understanding of archaeal box H/ACA sRNP function came from in vitro reconstitution of catalytically active box H/ACA sRNPs from recombinant archaeal proteins and in vitro transcribed sRNAs [27, 28]. These studies provided insight into the minimal set of proteins necessary for the assembly of a functional box H/ACA sRNP.
The minimal box H/ACA sRNP contains a set of four core proteins: L7Ae, Nop10, Gar1, and Cbf5 [27, 28, 76]. Biochemical studies have provided information on core protein interaction and assembly with box H/ACA guide sRNAs [27, 28, 76]. L7Ae, an important component of archaeal box C/D sRNPs, also recognizes the kink-turn or kink-loop motif of the box H/ACA sRNA [76, 96]. In contrast to the box C/D sRNP where Nop5 and fibrillarin are unable to bind to the sRNA prior to L7Ae, the box H/ACA sRNP core protein, Cbf5, is able to bind to the sRNA independently of L7Ae [27, 28]. Cbf5, based on its homology to the TruB family of pseudouridine synthases, is likely the catalytic moiety of the box H/ACA sRNP [94, 95, 97, 98]. Indeed, genetic depletion of the yeast Cbf5 homolog results in the loss of pseudouridylation of pre-rRNA . Efficient binding of Cbf5 to the sRNA requires the box H or ACA motif, the pseudouridylation pocket, and a GAG sequence in the terminal loop [27, 28]. The binding of Cbf5 to the sRNA is necessary for the assembly of Nop10 and Gar1 with the sRNA [27, 28].
In addition to biochemical studies, various structures of partial or complete core box H/ACA sRNPs have been determined [52, 100–105]. These structures provide atomic details for box H/ACA sRNP assembly and catalysis. As predicted, L7Ae binds to the kink-turn or kink-loop motif in the terminal loop near the upper stem . Cbf5 can be divided into two domains, the catalytic domain and the PUA domain. The catalytic domain of Cbf5 interacts with the upper stem (P1) of the sRNA and the pseudouridylation pocket (Figure 6) [52, 101, 104, 105]. Nop10 wedges between L7Ae and Cbf5 and interacts with both proteins [52, 101, 104]. Therefore, Nop10 acts as an organizer that mediates the interaction between L7Ae and Cbf5. The PUA domain of Cbf5 interacts with the lower stem (P1) of the sRNA. In addition, it also sequence-specifically recognizes the box ACA motif [52, 101, 104, 105]. It has been suggested that the interactions of the PUA domain with the lower stem and the interaction of the catalytic domain with the upper stem positions the pseudouridylation pocket such that the target modification site is positioned correctly in the active site of Cbf5 .
Furthermore, the structure of a substrate-bound box H/ACA sRNP shows that the helix formed between the 3′ guide sequence and the 5′ segment of the substrate interacts with the catalytic domain of Cbf5 . An important structural element of the catalytic domain, known as the thumb loop, makes extensive contacts with the substrate RNA and has been proposed to be important to lock the substrate RNA into place (Figure 6) . These interactions, together with the interactions between the PUA domain of Cbf5 and the lower stem of the sRNA, allow the precise positioning of the target modification site in the active site of Cbf5, which may explain why the spacing between the target modification site and the box H or ACA motif is usually ~15 nt .
While the other core proteins interact with the guide sRNA and the substrate RNA, Gar1 does not make any contacts with either RNA (Figure 6) [52, 101, 104, 105]. Rather, Gar1 interacts only with Cbf5. This observation is consistent with the fact that the box H/ACA sRNP still has detectable activity even in the absence of Gar1 [27, 52]. Interestingly, Gar1 is only able to interact with the thumb loop of Cbf5 in the substrate-free state but not in the substrate-bound state (Figure 6) [52, 101]. The thumb loop, therefore, switches between a closed state, which makes contact with the substrate, and an open state, which makes contacts with Gar1. This switching between the two states has led to the hypothesis that while Gar1 may not have a direct role in the chemistry of the catalytic reaction, it may have a role in facilitating the release of the product .
13. Other Functions of Box C/D and Box H/ACA sRNPs
While the function of archaeal box C/D and box H/ACA sRNPs for RNP-guided modification is relatively well understood, these sRNPs may also perform other functions. Some eukaryotic box C/D and box H/ACA snoRNPs perform functions other than RNA modification [106, 107]. One example is the eukaryotic U3 box C/D snoRNP. Using the guide snoRNA base-pairing capacity, U3 snoRNP helps cleave the 35S rRNA and may act as a chaperone in RNA folding [107–113]. Furthermore, there are other eukaryotic box C/D and box H/ACA snoRNPs that have evolved pre-rRNA processing functions [95, 106, 107].
While it is apparent that U3-like sRNAs are absent in Archaea , the ability of archaeal box C/D and box H/ACA sRNPs to perform functions other than nucleotide modifications remains a possibility. This may explain why the targets of nucleotide modification of some of the candidate box C/D sRNAs and box H/ACA sRNAs cannot be identified [42, 43, 61–66]. Therefore, some archaeal sRNPs may function in pre-rRNA cleaving or folding [69, 107, 115]. The hypothesis that sRNPs act as chaperones is consistent with the box C/D sRNP di-sRNP model. A dimeric sRNP can potentially allow base-pairing with four segments of pre-rRNAs using the four guide sequences, trapping nearby pre-rRNA sequences and avoiding the formation of premature RNA tertiary structures [16, 69]. The nonmodification functions of archaeal sRNPs are speculative. It will be interesting to see if these functions can be demonstrated for the archaeal sRNPs.
14. Functions of Nucleotide Modification
The locations of the pseudouridylations and 2′-O-methylations have been mapped onto the ribosomes of certain Eukaryotes, Bacteria, and Archaea  and are located in functionally important regions of the ribosome. Therefore, chemical modification has been proposed to have important functions in protein translation. While the removal of individual modifications does not have significant effects on the growth of an organism, studies in S. cerevisiae have shown that global removal of all modifications led to severe growth defects [35, 92, 116, 117]. Moreover, mutations that led to the removal of certain targeted nucleotide modifications also resulted in severe growth and protein synthesis defects [116, 118, 119]. Furthermore, depleting or mistargeting certain modifications in the S. cerevisiae rRNA, particularly in regions that are predicted to be important for ribosomal activity and/or ribosome biogenesis, also resulted in defects in ribosome synthesis and in mRNA translation [116, 118–120]. These studies have only been performed in eukaryotes. However, since nucleotide modifications are also located in important regions of archaeal ribosomes, they are likely to have important functions for archaeal ribosomes as well.
Accumulating evidence suggests that nucleotide modification is important in archaeal ribosome function. In S. solfataricus there is an increase in the number of nucleotide modifications when the growth temperature is increased, indicating nucleotide modification may have a stabilizing effect on the structure of the ribosome . This is especially important for many Archaea that live in extreme conditions. Indeed, NMR studies on a small segment of the 23S rRNA that contains a 2′-O-methylated nucleotide suggested that the modification enforces a certain local conformation of nearby nucleotides, thereby reducing the conformational dynamics of the nearby structures in a varying range of pH . Taken together, these studies suggest that rRNA modifications influence the stability of ribosomes. However, since current functional studies on rRNA modification in Archaea are very limited, the precise function of most modifications is still unknown.
A more thorough understanding of how Archaea regulate the process of modification of the 23S, 16S, and 5S rRNAs will come from further studies of the sRNPs that catalyze modifications. In these roles, further studies on the box C/D and box H/ACA sRNPs will yield a more complete elucidation of their structure, enzymatic activities, and conformational changes. There is still much to learn in terms of the chemical modification of nucleotides on the rRNA. Because the Archaea represent an untapped resource of knowledge, further research will yield many interesting and surprising results from this independent domain that is neither Bacteria nor Eukarya.
W. S. V. Yip and N. G. Vincent contributed equally to this paper.
The authors would like to thank the members of the Baserga Lab for their careful and thoughtful reading of this paper.
- W. F. Doolittle, “Phylogenetic classification and the universal tree,” Science, vol. 284, no. 5423, pp. 2124–2128, 1999.
- P. Yarza, M. Richter, J. Peplies et al., “The All-Species Living Tree project: a 16S rRNA-based phylogenetic tree of all sequenced type strains,” Systematic and Applied Microbiology, vol. 31, no. 4, pp. 241–250, 2008.
- G. E. Fox, L. J. Magrum, W. E. Balch, R. S. Wolfe, and C. R. Woese, “Classification of methanogenic bacteria by 16S ribosomal RNA characterization,” Proceedings of the National Academy of Sciences of the United States of America, vol. 74, no. 10, pp. 4537–4541, 1977.
- C. R. Woese and G. E. Fox, “Phylogenetic structure of the prokaryotic domain: the primary kingdoms,” Proceedings of the National Academy of Sciences of the United States of America, vol. 74, pp. 5088–5090, 1977.
- C. R. Woese, O. Kandler, and M. L. Wheelis, “Towards a natural system of organisms: proposal for the domains Archaea, Bacteria, and Eucarya,” Proceedings of the National Academy of Sciences of the United States of America, vol. 87, no. 12, pp. 4576–4579, 1990.
- R. Green and H. F. Noller, “Ribosomes and translation,” Annual Review of Biochemistry, vol. 66, pp. 679–716, 1997.
- P. J. Shaw and E. G. Jordan, “The nucleolus,” Annual Review of Cell and Developmental Biology, vol. 11, pp. 93–121, 1995.
- J. R. Warner, “The economics of ribosome biosynthesis in yeast,” Trends in Biochemical Sciences, vol. 24, no. 11, pp. 437–440, 1999.
- T. Allers and M. Mevarech, “Archaeal genetics—the third way,” Nature Reviews Genetics, vol. 6, no. 1, pp. 58–73, 2005.
- A. E. Hage and D. Tollervey, “A surfeit of factors: why is ribosome assembly so much more complicated in eukaryotes than bacteria?” RNA Biology, vol. 1, no. 1, pp. 10–15, 2004.
- G. Klug, E. Evguenieva-Hackenberg, A. D. Omer, et al., RNA Processing, American Society for Microbiology, Washington, DC, USA, 2007.
- C. R. Woese, L. J. Magrum, and G. E. Fox, “Archaebacteria,” Journal of Molecular Evolution, vol. 11, no. 3, pp. 245–252, 1978.
- R. P. Anitori, Ed., Extremophiles: Microbiology and Biotechnology, Caister Academic Press, Norfolk, UK, 2012.
- Z. M. P. Lee, C. Bussema III, and T. M. Schmidt, “rrnDB: documenting the number of rRNA and tRNA genes in bacteria and archaea,” Nucleic Acids Research, vol. 37, no. 1, pp. D489–D493, 2009.
- J. A. Klappenbach, P. R. Saxman, J. R. Cole, and T. M. Schmidt, “rrndb: the ribosomal RNA operon copy number database,” Nucleic Acids Research, vol. 29, no. 1, pp. 181–184, 2001.
- K. R. Bower-Phipps, D. W. Taylor, H. Wang, and S. J. Baserga, “The box C/D sRNP dimeric architecture is conserved across domain Archaea,” RNA, vol. 18, no. 8, pp. 1527–1540, 2012.
- J. Lin, S. Lai, R. Jia et al., “Structural basis for site-specific ribose methylation by box C/D RNA protein complexes,” Nature, vol. 469, no. 7331, pp. 559–563, 2011.
- A. L. Hartman, C. Norais, J. H. Badger et al., “The complete genome sequence of Haloferax volcanii DS2, a model archaeon,” PloS One, vol. 5, no. 3, article e9605, 2010.
- J. Chant and P. Dennis, “Archaebacteria: transcription and processing of ribosomal RNA sequences in Halobacterium cutirubrum,” The EMBO Journal, vol. 5, no. 5, pp. 1091–1097, 1986.
- J. Kjems and R. A. Garrett, “An intron in the 23S ribosomal RNA gene of the archaebacterium Desulfurococcus mobilis,” Nature, vol. 318, no. 6047, pp. 675–677, 1985.
- J. Kjems and R. A. Garrett, “Ribosomal RNA introns in archaea and evidence for RNA conformational changes associated with splicing,” Proceedings of the National Academy of Sciences of the United States of America, vol. 88, no. 2, pp. 439–443, 1991.
- S. Burggraf, N. Larsen, C. R. Woese, and K. O. Stetter, “An intron within the 16S ribosomal RNA gene of the archaeon Pyrobaculum aerophilum,” Proceedings of the National Academy of Sciences of the United States of America, vol. 90, no. 6, pp. 2547–2550, 1993.
- J. Z. Dalgaard, R. A. Garrett, and M. Belfort, “Purification and characterization of two forms of I-DmoI, a thermophilic site-specific endonuclease encoded by an archaeal intron,” Journal of Biological Chemistry, vol. 269, no. 46, pp. 28885–28892, 1994.
- J. Z. Dalgaard, R. A. Garrett, and M. Belfort, “A site-specific endonuclease encoded by a typical archaeal intron,” Proceedings of the National Academy of Sciences of the United States of America, vol. 90, no. 12, pp. 5414–5417, 1993.
- V. Salman, R. Amann, D. A. Shub, et al., “Multiple self-splicing introns in the 16S rRNA genes of giant sulfur bacteria,” Proceedings of the National Academy of Sciences of the United States of America, vol. 109, pp. 4203–4208, 2012.
- A. D. Omer, S. Ziesche, H. Ebhardt, and P. P. Dennis, “In vitro reconstitution and activity of a C/D box methylation guide ribonucleoprotein complex,” Proceedings of the National Academy of Sciences of the United States of America, vol. 99, no. 8, pp. 5289–5294, 2002.
- B. Charpentier, S. Muller, and C. Branlant, “Reconstitution of archaeal H/ACA small ribonucleoprotein complexes active in pseudouridylation,” Nucleic Acids Research, vol. 33, no. 10, pp. 3133–3144, 2005.
- D. L. Baker, O. A. Youssef, M. I. R. Chastkofsky, D. A. Dy, R. M. Terns, and M. P. Terns, “RNA-guided RNA modification: functional organization of the archaeal H/ACA RNP,” Genes & Development, vol. 19, no. 10, pp. 1238–1248, 2005.
- D. Tollervey, “Small nucleolar RNAs guide ribosomal RNA methylation,” Science, vol. 273, no. 5278, pp. 1056–1057, 1996.
- P. Ganot, M. L. Bortolin, and T. Kiss, “Site-specific pseudouridine formation in preribosomal RNA is guided by small nucleolar RNAs,” Cell, vol. 89, no. 5, pp. 799–809, 1997.
- Z. Kiss-László, Y. Henry, J. P. Bachellerie, M. Caizergues-Ferrer, and T. Kiss, “Site-specific ribose methylation of preribosomal RNA: a novel function for small nucleolar RNAs,” Cell, vol. 85, no. 7, pp. 1077–1088, 1996.
- M. Nicoloso, L. H. Qu, B. Michot, and J. P. Bachellerie, “Intron-encoded, antisense small nucleolar RNAs: the characterization of nine novel species points to their direct role as guides for the 2′-O-ribose methylation of rRNAs,” Journal of Molecular Biology, vol. 260, no. 2, pp. 178–195, 1996.
- J. Cavaillé, M. Nicoloso, and J. P. Bachellerie, “Targeted ribose methylation of RNA in vivo directed by tailored antisense RNA guides,” Nature, vol. 383, no. 6602, pp. 732–735, 1996.
- B. Lapeyre, “Conserved ribosomal RNA modification and their putative roles in ribosome biogenesis and translation,” in Fine-Tuning of RNA Functions by Modification and Editing, vol. 12, pp. 263–284, Springer, New York, NY, USA, 2005.
- W. A. Decatur and M. J. Fournier, “rRNA modifications and ribosome function,” Trends in Biochemical Sciences, vol. 27, no. 7, pp. 344–351, 2002.
- K. R. Noon, E. Bruenger, and J. A. McCloskey, “Posttranscriptional modifications in 16S and 23S rRNAs of the archaeal hyperthermophile Sulfolobus solfataricus,” Journal of Bacteriology, vol. 180, no. 11, pp. 2883–2888, 1998.
- W. A. Decatur and M. J. Fournier, “RNA-guided nucleotide modification of ribosomal and other RNAs,” Journal of Biological Chemistry, vol. 278, no. 2, pp. 695–698, 2003.
- J. Ofengand and A. Bakin, “Mapping to nucleotide resolution of pseudouridine residues in large subunit ribosomal RNAs from representative eukaryotes, prokaryotes, archaebacteria, mitochondria and chloroplasts,” Journal of Molecular Biology, vol. 266, no. 2, pp. 246–268, 1997.
- B. E. H. Maden, “The numerous modified nucleotides in eukaryotic ribosomal RNA,” Progress in Nucleic Acid Research and Molecular Biology, vol. 39, pp. 241–303, 1990.
- D. D. Piekna-Przybylska, W. A. Decatur, and M. J. Fournier, “The 3D rRNA modification maps database: with interactive tools for ribosome analysis,” Nucleic Acids Research, vol. 36, no. 1, pp. D178–D183, 2008.
- M. Del Campo, Y. Kaya, and J. Ofengand, “Identification and site of action of the remaining four putative pseudouridine synthases in Escherichia coli,” RNA, vol. 7, no. 11, pp. 1603–1615, 2001.
- T. H. Tang, N. Polacek, M. Zywicki et al., “Identification of novel non-coding RNAs as potential antisense regulators in the archaeon Sulfolobus solfataricus,” Molecular Microbiology, vol. 55, no. 2, pp. 469–481, 2005.
- M. A. Zago, P. P. Dennis, and A. D. Omer, “The expanding world of small RNAs in the hyperthermophilic archaeon Sulfolobus solfataricus,” Molecular Microbiology, vol. 55, no. 6, pp. 1812–1828, 2005.
- J. Kjems and R. A. Garrett, “Novel expression of the ribosomal RNA genes in the extreme thermophile and archaebacterium Desulfurococcus mobilis,” The EMBO Journal, vol. 6, pp. 3521–3530, 1987.
- J. Kjems, H. Leffers, R. A. Garrett, G. Wich, W. Leinfelder, and A. Böck, “Gene organization, transcription signals and processing of the single ribosomal RNA operon of the archaebacterium Thermoproteus tenax,” Nucleic Acids Research, vol. 15, no. 12, pp. 4821–4835, 1987.
- Q. She, R. K. Singh, F. Confalonieri, et al., “The complete genome of the crenarchaeon Sulfolobus solfataricus P2,” Proceedings of the National Academy of Sciences of the United States of America, vol. 98, no. 14, pp. 7835–7840, 2001.
- R. K. Hartmann, N. Ulbrich, and V. A. Erdmann, “An unusual rRNA operon constellation: in Thermus thermophilus HB8 the 23S/5S rRNA operon is a separate entity from the 16S rRNA operon,” Biochimie, vol. 69, no. 10, pp. 1097–1104, 1987.
- C. J. Bult, O. White, G. J. Olsen, et al., “Complete genome sequence of the methanogenic archaeon, Methanococcus jannaschii,” Science, vol. 273, no. 5278, pp. 1058–1073, 1996.
- H. K. Ree and R. A. Zimmermann, “Organization and expression of the 16S, 23S and 5S ribosomal RNA genes from the archaebacterium Thermoplasma acidophilum,” Nucleic Acids Research, vol. 18, no. 15, pp. 4471–4478, 1990.
- E. Waters, M. J. Hohn, I. Ahel, et al., “The genome of Nanoarchaeum equitans: insights into early archaeal evolution and derived parasitism,” Proceedings of the National Academy of Sciences of the United States of America, vol. 100, no. 22, pp. 12984–12988, 2003.
- G. Wachtershauser, “Towards a reconstruction of ancestral genomes by gene cluster alignment,” Systematic and Applied Microbiology, vol. 21, no. 4, pp. 473–477, 1998.
- J. Duan, L. Li, J. Lu, W. Wang, and K. Ye, “Structural mechanism of substrate RNA recruitment in H/ACA RNA-guided pseudouridine synthase,” Molecular Cell, vol. 34, no. 4, pp. 427–439, 2009.
- J. Lykke-Andersen, C. Aagaard, M. Semionenkov, and R. A. Garrett, “Archaeal introns: splicing, intercellular mobility and evolution,” Trends in Biochemical Sciences, vol. 22, no. 9, pp. 326–331, 1997.
- M. Belfort, M. E. Reaban, T. Coetzee, and J. Z. Dalgaard, “Prokaryotic introns and inteins: a panoply of form and function,” Journal of Bacteriology, vol. 177, no. 14, pp. 3897–3903, 1995.
- T. H. Tang, T. S. Rozhdestvensky, B. C. d'Orval et al., “RNomics in Archaea reveals a further link between splicing of archaeal introns and rRNA processing,” Nucleic Acids Research, vol. 30, no. 4, pp. 921–930, 2002.
- P. P. Dennis, A. Omer, and T. Lowe, “A guided tour: small RNA function in Aarchaea,” Molecular Microbiology, vol. 40, no. 3, pp. 509–519, 2001.
- S. M. Ziesche, A. D. Omer, and P. P. Dennis, “RNA-guided nucleotide modification of ribosomal and non-ribosomal RNAs in Archaea,” Molecular Microbiology, vol. 54, no. 4, pp. 980–993, 2004.
- A. D. Omer, S. Ziesche, W. A. Decatur, M. J. Fournier, and P. P. Dennis, “RNA-modifying machines in archaea,” Molecular Microbiology, vol. 48, no. 3, pp. 617–629, 2003.
- P. P. Dennis and A. Omer, “Small non-coding RNAs in Archaea,” Current Opinion in Microbiology, vol. 8, no. 6, pp. 685–694, 2005.
- J. Ni, A. L. Tien, and M. J. Fournier, “Small nucleolar RNAs direct site-specific synthesis of pseudouridine in ribosomal RNA,” Cell, vol. 89, no. 4, pp. 565–573, 1997.
- A. D. Omer, T. M. Lowe, A. G. Russell, H. Ebhardt, S. R. Eddy, and P. P. Dennis, “Homologs of small nucleolar RNAs in Archaea,” Science, vol. 288, no. 5465, pp. 517–522, 2000.
- R. J. Klein, Z. Misulovin, and S. R. Eddy, “Noncoding RNA genes identified in AT-rich hyperthermophiles,” Proceedings of the National Academy of Sciences of the United States of America, vol. 99, no. 11, pp. 7542–7547, 2002.
- C. Gaspin, J. Cavaillé, G. Erauso, et al., “Archaeal homologs of eukaryotic methylation guide small nucleolar RNAs: lessons from the Pyrococcus genomes,” Journal of Molecular Biology, vol. 297, no. 4, pp. 895–906, 2000.
- T. H. Tang, J. P. Bachellerie, T. Rozhdestvensky et al., “Identification of 86 candidates for small non-messenger RNAs from the archaeon Archaeoglobus fulgidus,” Proceedings of the National Academy of Sciences of the United States of America, vol. 99, no. 11, pp. 7536–7541, 2002.
- S. Muller, F. Leclerc, I. Behm-Ansmant, J. B. Fourmann, B. Charpentier, and C. Branlant, “Combined in silico and experimental identification of the Pyrococcus abyssi H/ACA sRNAs and their target sites in ribosomal RNAs,” Nucleic Acids Research, vol. 36, no. 8, pp. 2459–2475, 2008.
- L. Randau, “RNA processing in the minimal organism Nanoarchaeum equitans,” Genome Biology, vol. 13, article R63, 2012.
- D. L. Bernick, P. P. Dennis, M. Höchsmann, et al., “Discovery of Pyrobaculum small RNA families with atypical pseudouridine guide RNA features,” RNA, vol. 18, pp. 402–411, 2012.
- F. Bleichert, K. T. Gagnon, B. Brown, et al., “A dimeric structure for archaeal box C/D small ribonucleoproteins,” Science, vol. 325, pp. 1384–1387, 2009.
- F. Bleichert and S. J. Baserga, “Ribonucleoprotein multimers and their functions,” Critical Reviews in Biochemistry and Molecular Biology, vol. 45, no. 5, pp. 331–350, 2010.
- T. Moore, Y. Zhang, M. O. Fenley, and H. Li, “Molecular basis of box C/D RNA-protein interactions: cocrystal structure of archaeal L7Ae and a box C/D RNA,” Structure, vol. 12, no. 5, pp. 807–818, 2004.
- D. J. Klein, T. M. Schmeing, P. B. Moore, and T. A. Steitz, “The kink-turn: a new RNA secondary structure motif,” The EMBO Journal, vol. 20, no. 15, pp. 4214–4221, 2001.
- S. Nolivos, A. J. Carpousis, and B. Clouet-d'Orval, “The K-loop, a general feature of the Pyrococcus C/D guide RNAs, is an RNA structural motif related to the K-turn,” Nucleic Acids Research, vol. 33, no. 20, pp. 6507–6514, 2005.
- E. Tran, X. Zhang, L. Lackey, and E. S. Maxwell, “Conserved spacing between the box C/D and C′/D′ RNPs of the archaeal box C/D sRNP complex is required for efficient 2′-O-methylation of target RNAs,” RNA, vol. 11, no. 3, pp. 285–293, 2005.
- H. Wang, D. Boisvert, K. K. Kim, R. Kim, and S. H. Kim, “Crystal structure of a fibrillarin homologue from Methanococcus jannaschii, a hyperthermophile, at 1.6 Å resolution,” The EMBO Journal, vol. 19, no. 3, pp. 317–323, 2000.
- J. F. Kuhn, E. J. Tran, and E. S. Maxwell, “Archaeal ribosomal protein L7 is a functional homolog of the eukaryotic 15.5kD/Snu13p snoRNP core protein,” Nucleic Acids Research, vol. 30, no. 4, pp. 931–941, 2002.
- T. S. Rozhdestvensky, T. H. Tang, I. V. Tchirkova, J. Brosius, J. P. Bachellerie, and A. Hüttenhofer, “Binding of L7Ae protein to the K-turn of archaeal snoRNAs: a shared RNA binding motif for C/D and H/ACA box snoRNAs in Archaea,” Nucleic Acids Research, vol. 31, no. 3, pp. 869–877, 2003.
- M. Aittaleb, R. Rashid, Q. Chen, J. R. Palmer, C. J. Daniels, and H. Li, “Structure and function of archaeal box C/D sRNP core proteins,” Nature Structural Biology, vol. 10, no. 4, pp. 256–263, 2003.
- R. Rashid, M. Aittaleb, Q. Chen, K. Spiegel, B. Demeler, and H. Li, “Functional requirement for symmetric assembly of archaeal box C/D small ribonucleoprotein particles,” Journal of Molecular Biology, vol. 333, no. 2, pp. 295–306, 2003.
- E. J. Tran, X. Zhang, and E. S. Maxwell, “Efficient RNA 2′-O-methylation requires juxtaposed and symmetrically assembled archaeal box C/D and C′/D′ RNPs,” The EMBO Journal, vol. 22, no. 15, pp. 3930–3940, 2003.
- M. Aittaleb, T. Visone, M. O. Fenley, and H. Li, “Structural and thermodynamic evidence for a stabilizing role of Nop5p in S-adenosyl-L-methionine binding to fibrillarin,” Journal of Biological Chemistry, vol. 279, no. 40, pp. 41822–41829, 2004.
- X. Zhang, E. A. Champion, E. J. Tran, B. A. Brown, S. J. Baserga, and E. Stuart Maxwell, “The coiled-coil domain of the Nop56/58 core protein is dispensable for sRNP assembly but is critical for archaeal box C/D sRNP-guided nucleotide methylation,” RNA, vol. 12, no. 6, pp. 1092–1103, 2006.
- J. W. Hardin and R. T. Batey, “The bipartite architecture of the sRNA in an archaeal box C/D complex is a primary determinant of specificity,” Nucleic Acids Research, vol. 34, no. 18, pp. 5039–5051, 2006.
- A. D. Omer, M. Zago, A. Chang, and P. P. Dennis, “Probing the structure and function of an archaeal C/D-box methylation guide sRNA,” RNA, vol. 12, no. 9, pp. 1708–1720, 2006.
- S. Oruganti, Y. Zhang, H. Li et al., “Alternative conformations of the archaeal Nop56/58-fibrillarin complex imply flexibility in box C/D RNPs,” Journal of Molecular Biology, vol. 371, no. 5, pp. 1141–1150, 2007.
- C. D. Appel and E. S. Maxwell, “Structural features of the guide:target RNA duplex required for archaeal box C/D sRNA-guided nucleotide 2′-O-methylation,” RNA, vol. 13, no. 6, pp. 899–911, 2007.
- K. Ye, R. Jia, J. Lin et al., “Structural organization of box C/D RNA-guided RNA methyltransferase,” Proceedings of the National Academy of Sciences of the United States of America, vol. 106, no. 33, pp. 13808–13813, 2009.
- S. Xue, R. Wang, F. Yang et al., “Structural basis for substrate placement by an archaeal box C/D ribonucleoprotein particle,” Molecular Cell, vol. 39, no. 6, pp. 939–949, 2010.
- K. T. Gagnon, X. Zhang, G. Qu et al., “Signature amino acids enable the archaeal L7Ae box C/D RNP core protein to recognize and bind the K-loop RNA motif,” RNA, vol. 16, no. 1, pp. 79–90, 2010.
- F. Bleichert and S. J. Baserga, “Dissecting the role of conserved box C/D sRNA sequences in di-sRNP assembly and function,” Nucleic Acids Research, vol. 38, no. 22, pp. 8295–8305, 2010.
- K. T. Gagnon, S. Biswas, X. Zhang, et al., “Structurally conserved Nop56/58 N-terminal domain facilitates archaeal box C/D ribonucleoprotein-guided methyltransferase activity,” The Journal of Biological Chemistry, vol. 287, no. 23, pp. 19418–19428, 2012.
- J. L. Martin and F. M. McMillan, “SAM (dependent) I AM: the S-adenosylmethionine-dependent methyltransferase fold,” Current Opinion in Structural Biology, vol. 12, no. 6, pp. 783–793, 2002.
- D. Tollervey, H. Lehtonen, R. Jansen, H. Kern, and E. C. Hurt, “Temperature-sensitive mutations demonstrate roles for yeast fibrillarin in pre-rRNA processing, pre-rRNA methylation, and ribosome assembly,” Cell, vol. 72, no. 3, pp. 443–457, 1993.
- H. Ghalei, H. H. Hsiao, H. Urlaub, M. C. Wahl, and N. J. Watkins, “A novel Nop5-sRNA interaction that is required for efficient archaeal box C/D sRNP formation,” RNA, vol. 16, no. 12, pp. 2341–2348, 2010.
- M. Terns and R. Terns, “Noncoding RNAs of the H/ACA family,” Cold Spring Harbor Symposia on Quantitative Biology, vol. 71, pp. 395–405, 2006.
- N. J. Watkins and M. T. Bohnsack, “The box C/D and H/ACA snoRNPs: key players in the modification, processing and the dynamic folding of ribosomal RNA,” Wiley Interdisciplinary Reviews. RNA, vol. 3, no. 3, pp. 397–414, 2012.
- T. Hamma and A. R. Ferré-D'Amaré, “Structure of protein L7Ae bound to a K-turn derived from an archaeal box H/ACA sRNA at 1.8 Å resolution,” Structure, vol. 12, no. 5, pp. 893–903, 2004.
- E. V. Koonin, “Pseudouridine syntheses: four families of enzymes containing a putative uridine-binding motif also conserved in dUTPases and dCTP deaminases,” Nucleic Acids Research, vol. 24, no. 12, pp. 2411–2415, 1996.
- I. K. Blaby, M. Majumder, K. Chatterjee et al., “Pseudouridine formation in archaeal RNAs: the case of Haloferax volcanii,” RNA, vol. 17, no. 7, pp. 1367–1380, 2011.
- D. L. J. Lafontaine, C. Bousquet-Antonelli, Y. Henry, M. Caizergues-Ferrer, and D. Tollervey, “The box H + ACA snoRNAs carry Cbf5p, the putative rRNA pseudouridine synthase,” Genes & Development, vol. 12, no. 4, pp. 527–537, 1998.
- T. Hamma, S. L. Reichow, G. Varani, and A. R. Ferré-D'Amaré, “The Cbf5-Nop10 complex is a molecular bracket that organizes box H/ACA RNPs,” Nature Structural and Molecular Biology, vol. 12, no. 12, pp. 1101–1107, 2005.
- L. Li and K. Ye, “Crystal structure of an H/ACA box ribonucleoprotein particle,” Nature, vol. 443, no. 7109, pp. 302–307, 2006.
- X. Manival, C. Charron, J. B. Fourmann, F. Godard, B. Charpentier, and C. Branlant, “Crystal structure determination and site-directed mutagenesis of the Pyrococcus abyssi aCBF5-aNOP10 complex reveal crucial roles of the C-terminal domains of both proteins in H/ACA sRNP activity,” Nucleic Acids Research, vol. 34, no. 3, pp. 826–839, 2006.
- R. Rashid, B. Liang, D. L. Baker et al., “Crystal structure of a Cbf5-Nop10-Gar1 complex and implications in RNA-guided pseudouridylation and dyskeratosis congenita,” Molecular Cell, vol. 21, no. 2, pp. 249–260, 2006.
- B. Liang, J. Zhou, E. Kahen, R. M. Terns, M. P. Terns, and H. Li, “Structure of a functional ribonucleoprotein pseudouridine synthase bound to a substrate RNA,” Nature Structural and Molecular Biology, vol. 16, no. 7, pp. 740–746, 2009.
- B. Liang, S. Xue, R. M. Terns, M. P. Terns, and H. Li, “Substrate RNA positioning in the archaeal H/ACA ribonucleoprotein complex,” Nature Structural and Molecular Biology, vol. 14, no. 12, pp. 1189–1195, 2007.
- A. K. Henras, J. Soudet, M. Gérus et al., “The post-transcriptional steps of eukaryotic ribosome biogenesis,” Cellular and Molecular Life Sciences, vol. 65, no. 15, pp. 2334–2359, 2008.
- K. R. Phipps, J. M. Charette, and S. J. Baserga, “The small subunit processome in ribosome biogenesis—progress and prospects,” WIREs RNA, vol. 2, no. 1, pp. 1–21, 2011.
- M. Beltrame and D. Tollervey, “Identification and functional analysis of two U3 binding sites on yeast pre-ribosomal RNA,” The EMBO Journal, vol. 11, no. 4, pp. 1531–1542, 1992.
- M. Beltrame and D. Tollervey, “Base pairing between U3 and the pre-ribosomal RNA is required for 18S rRNA synthesis,” The EMBO Journal, vol. 14, no. 17, pp. 4350–4356, 1995.
- A. Méreau, R. Fournier, A. Grégoire et al., “An in vivo and in vitro structure-function analysis of the Saccharomyces cerevisiae U3A snoRNP: protein-RNA contacts and base-pair interaction with the pre-ribosomal RNA,” Journal of Molecular Biology, vol. 273, no. 3, pp. 552–571, 1997.
- A. V. Borovjagin and S. A. Gerbi, “The spacing between functional Cis-elements of U3 snoRNA is critical for rRNA processing,” Journal of Molecular Biology, vol. 300, no. 1, pp. 57–74, 2000.
- A. V. Borovjagin and S. A. Gerbi, “Xenopus U3 snoRNA GAC-box A′ and box A sequences play distinct functional roles in rRNA processing,” Molecular and Cellular Biology, vol. 21, no. 18, pp. 6210–6221, 2001.
- D. A. Samarsky and M. J. Fournier, “Functional mapping of the U3 small nucleolar RNA from the yeast Saccharomyces cerevisiae,” Molecular and Cellular Biology, vol. 18, no. 6, pp. 3431–3444, 1998.
- P. P. Dennis, A. G. Russell, and M. Moniz De Sá, “Formation of the 5′ end pseudoknot in small subunit ribosomal RNA: involvement of U3-like sequences,” RNA, vol. 3, no. 4, pp. 337–343, 1997.
- R. J. W. Schoemaker and A. P. Gultyaev, “Computer simulation of chaperone effects of Archaeal C/D box sRNA binding on rRNA folding,” Nucleic Acids Research, vol. 34, no. 7, pp. 2015–2026, 2006.
- X. H. Liang, Q. Liu, and M. J. Fournier, “Loss of rRNA modifications in the decoding center of the ribosome impairs translation and strongly delays pre-rRNA processing,” RNA, vol. 15, no. 9, pp. 1716–1728, 2009.
- Y. Zebarjadian, T. King, M. J. Fournier, L. Clarke, and J. Carbon, “Point mutations in yeast CBF5 can abolish in vivo pseudouridylation of rRNA,” Molecular and Cellular Biology, vol. 19, no. 11, pp. 7461–7472, 1999.
- S. Higa-Nakamine, T. Suzuki, T. Uechi, et al., “Loss of ribosomal RNA modification causes developmental defects in zebrafish,” Nucleic Acids Research, pp. 1–8, 2011.
- X. H. Liang, Q. Liu, and M. J. Fournier, “rRNA modifications in an intersubunit bridge of the ribosome strongly affect both ribosome biogenesis and activity,” Molecular Cell, vol. 28, no. 6, pp. 965–977, 2007.
- B. Liu, X. H. Liang, D. Piekna-Przybylska, Q. Liu, and M. J. Fournier, “Mis-targeted methylation in rRNA can severely impair ribosome synthesis and activity,” RNA Biology, vol. 5, no. 4, pp. 249–254, 2008.
- S. C. Blanchard and J. D. Puglisi, “Solution structure of the A loop of 23S ribosomal RNA,” Proceedings of the National Academy of Sciences of the United States of America, vol. 98, no. 7, pp. 3720–3725, 2001.