RNA MISHMASH
RNA MODIFICATIONS
Sibbrrit et al, WIREsRNA 2013
FUNCTIONS
m A RNA-seq
Li at al, Nat Methods, 2017
m C RNA-seq
Li at al, Nat Methods, 2017
RNA MODIFICATION: mRNA m A
Dominissini at al, Nat.Rev.Genet., 2014
N 6 -methyladenosine:
• in eukaryotic mRNAs lncRNAs (discovered in 1970s)
• reversible, conserved
• methyltransferase METTL3 or METTL4-METTL14 complex with WTAP (yeast Mum2) in a [G/A/U][G>A]m6AC[U>A>C] context
• demethylases FTO and ALKBH5
• occurrence 0.1–0.4% of As in mammals (~3–5 m
6A sites per mRNA)
• Readers: YTHDF2 methyltransferases
demethylases
FUNCTIONS of mRNA m A
Dominissini at al, Nat.Rev.Genet., 2014
Readers (or anti-readers): YTHDF2 family preferentially recognize m
6A RNA m
6A can be also read by hnRNPs
• Regulation of mRNA stability and localization
• circadian clock
- inhibition of m6A leads to prolonged nuclear retention of circadian mRNAs and delays their nuclear exit
• cell cycle
- meiosis in yeast in nitrogen starvation
• development and differentiation
- in embryonic stem cells (mESCs)
FUNCTIONS of m A
Dominissini at al, Nat.Rev.Genet., 2014;
Pan, TiBS, 2013
Chen and Shyu, TiBS 2016
m A and mRNA STABILITY
promoting deadenylation
affecting local secondary structure
inhibiting deadenylation
Chen and Shyu, TiBS 2016
m A and mRNA STABILITY
promoting deadenylation
affecting local secondary structure
inhibiting deadenylation
FUNCTIONS of m A: pri-miRNA PROCESSING
• m
6A is present in pri-miRNA regions
• METTL3 modulates miRNA expression level
• METTL3 targets pri-miRNAs for m
6A methylation
• m
6A in pri-miRNA is required for normal processing by DGCR8
• HNRNPA2B1 RNA-binding protein recognizes m
6A sites
• HNRNPA2B1 nuclear reader recruits Microprocessor
Alarcon at al, Nature, 2015
FUNCTIONS of m A: mRNA SPLICING
Xiao et al, Mol. Cell, 2016
nuclear YTHDC1 m
6A reader
• interacts with SR proteins SRSF3 and SRSF10
• facilitates/blocks binding of SRSF3/SRSF10 to pre- mRNAs
• promotes exon inclusion
of targeted mRNAs
FUNCTIONS of m A: TRANSLATION
• m
6A in 5’ UTR promotes cap-independent translation
• m
6A in 5’ UTR upregulates translation
• cellular stresses increase m
6A in 5’ UTRs
• YTHDF2 in heat shock induces m
6A-dependent translation of HS mRNAs
• m
6A in mRNA body disrupts tRNA selection and translation elongation dynamics
Meyer et al, Cell, 2015;
Zhou et al, Nature, 2015;
Choi et al, Nat. Struct. Mol. Biol.’16
FUNCTIONS of m A: RNAPII and TRANSLATION
Slobodin et al, Cell, 2017
• mRNA transcription rates correlate with translation
• slow PolII results in higher level of m
6A in mRNAs
• high level m
6A reduces translation rate
• nuclear control on protein
abundance
OTHER FUNCTIONS of m A
X-chromosome inactivation
m
6A facilitates gene silencing via nuclear reader DC1 that binds to m
6A on Xist.
DC1 may recruit Polycomb and/or other silencing factors (SHARP, LBR, hnRNPU, hnRNPK)
Huisman et al, 2017, TiBS
Epitranscriptomics, Meiosis, Sex determination, Cellular differentiation,
Development, Pluripotency and Reprogramming, Disease, Cancer
m A
MULTIPLE FUNCTIONS
Patil et al, 2017, TiCB
RNA MODIFICATION: mRNA m A
N 1 -methyladenosine m 1 A:
• in eukaryotic mRNAs (from yeasts to mammals)
• modified by TRMT6/TRMT61A (nuclear) or TRMT61B, TRMT10C (mitochondrial)
• at mRNA cap and 5’ UTR increases translation
• prevalent in mitochondrial-encoded transcripts inhibits translation
• in different mRNA regions differentially impacts translation
Li at al, Mol Cell 2017
Dominissini et al, Nature 2017
• widespread (20% in humans)
• enriched around the start codon upstream of the first splice site
• preferentially in more structured regions around translation initiation sites
• is dynamic in response to different conditions
• promotes translation
• in cytosol low in few mRNAs
• in tRNA T-loop like structures
• present also in mitochondria
• leads to translational repression
• is disruptive to W-C basepairing
• generally avoided by cells
Safra et al, Nature 2017
FUNCTIONS of m C
• synthesized by TRM4B methyltransferase
• enriched in the CG context and in downstream of translation initiation sites
• present in mRNAs and ncRNAs, also tRNAs
• tissue specific, acts as a epitranscriptome marker
• mRNA export: NSUN2 as the methyltransferase and ALYREF as an m
5C reader
Yang et al, 2017, Cell Res
Simms and Zaher, CellMolLifeSci 2016
damaged nucleobases exhibit altered base pairing
RNA REPAIR
oxidative and alkylative
damage on RNA
Simms and Zaher, CellMolLifeSci 2016
RNA REPAIR
R-LOOPs = DNA::RNA hybrid
Aguilera and Garcıa-Muse, Mol Cell, 2012
R-LOOPs in TRANSCRIPTION
Aguilera and Garcıa-Muse, Mol Cell, 2012
Yeast
Metazoans
Preventing R-loops
• DNA::RNA hybrids forming during
transcription before RNP packaging into RNP
• negative effect, may result in
- polymerase stalling, termination defects - replication fork stalling
- DNA damage
- genetic instability
R-LOOPs
DIP:
DNA IP
Le and Manley, Gene Dev, 2005
R-LOOPs
Aguilera and Garcıa-Muse Mol Cell, 2012
collision with: DNA lesions RNA::DNA hybrid
RNAP fork reversal by torsional stress
by template switching
homologous recombination
R-LOOPs accumulate in RNP biogenesis mutants
elongation impairment replication blockage DNA damage
genotoxic agents nucleases
tho and export mutants
WT with PolII stalled on damage Transcription-Coupled Repair (TCR) activated or PolII degraded
mut with PolII stalled on damage TCR not activated, only PolII degradation and global genome repair (GGR)
ssDNA
Sen1 and R-loop degradation by RNaseH prevent genome instability
R-loop accumulate in sen1 mut and may result in homologous recombination via:
- nicks in ssDNA
- ssDNA recognition by proteins
- collapse of colliding replication forks
sen1 mutant
Huertas and Aguillera, Mol Cell, 2004; Gaillard et al, NAR, 2007; Mischo et al., Mol Cell, 2011
ChIP
DIP= IP with DNA/RNA Abs
The level of R-loops and Pol I pileups depend on topoisomerase I and RNase H
Topoisomerases release positive supercoiling built in front of Pol I by rotating DNA during transcripton
This pauses Pol I (pileups) but opens DNA behind, stimulates
R-loops which slow down Pol I
RNase H cleave DNA/RNA hybrids releasing truncated pre-rRNA fragments degraded by TRAMP/exosome
Lack of Top1/2 and RNaseH massive R-loops cause severe Pol I arrest and pileups
El Hage et al., Gene Dev, 2011
R-LOOPs block rRNA transcription
ALTERNATIVE POLYMERASES
Scheer et al, TiG., 2016
OLIGO-URIDYLATION
PUP Poly(U) Polymerases
TUTase Terminal Uridylyl Transferase 3’ oligouridylation 1. Histone mRNA degradation (metazoans)
Mullen and Marzluff, Genes Dev., 2008
DIS3L2
Scheer et al, TiG., 2016
1. Histone mRNA degradation (metazoans)
2. miRNA degradation
precursors C. elegans
Krol et al., Nat Rev Genet, 2010; Kim et al., Cell, 2010
OLIGO-URIDYLATION
mature
Arabidopsis
Chlamydomonas
3. mRNA degradation? (plants)
Lsm1-7
DIS3L2
OLIGO-URIDYLATION
3. mRNA degradation
Scheer et al, TiG., 2016
OLIGO-URIDYLATION
Scheer et al, TiG., 2016
3. other
HISTONE mRNA 3’ end FORMATION
(nonpolyadenylated, metazoa, unique)
Dominski and Marzluff, Gene, 2007
U7 snRNP unique
Sm/Lsm10/11 SL
structure
endonuclease
• Histone pre-mRNA contains conserved stem-loop (SL) structure, recognized by the SLBP (SL-binding protein)
• SLBP, ZFP100 and HDE (histone downstream element) stabilize the binding of U7
• U7 snRNP, specificaly Lsm11, recruits cleavage factors and the cleavage by
endonuclease CPSF-73 generates mature 3’ end of histone mRNA
URIDYLATION
Lee et al, Cell, 2014
Uridylation-dependet mRNA decay
Uridylation of pre-miRNAs and miRNAs
Degradation of histone mRNAs
TUTases
Wethmar WIREsRNA, 2014
uORFs = upstream ORFs
Puyeo et al, TiBS, 2016
small ORFs = sORFs, sPEPs, smORF
Methods to identify sORFs and sPEPs
Plaza et al, Annu Rev Cell Dev Biol, 2017
sORFs
Couso and Patraquim Nat Rev Mol Cell Biol, 2017
Functions of sPEPs
Couso and Patraquim Nat Rev Mol Cell Biol, 2017
Andrews and Rothnagel, Nat Rev Genet, 2014
Functional sPEPs
POLYMERASE BACKTRACKING
Nudlerr, Cell, 2013