specificity and regulation of the endoplasmic reticulum-associated degradation machinery
TRANSCRIPT
Specificity and Regulation of the Endoplasmic Reticulum-Associated Degradation Machinery
Jessica Merulla1,2, Elisa Fasana1, Tatiana Soldà1 and Maurizio Molinari1,3*
1Institute for Research in Biomedicine, Protein Folding and Quality Control,
CH-6500 Bellinzona, Switzerland 2Graduate School for Cellular and Biomedical Sciences, University of Bern, Switzerland
3Ecole Polytechnique Fédérale de Lausanne, School of Life Sciences, CH-1015 Lausanne,
Switzerland
Correspondence to: [email protected]
Keywords Chemical and pharmacological chaperones Conformational diseases Defective ribosomal products (DRiPS) Endoplasmic reticulum ER-associated degradation (ERAD) ERAD tuning ER stress Hijacking by pathogens Misfolded proteins Proteostasis Ubiquitin proteasome system Unfolded protein response (UPR)
This article has been accepted for publication and undergone full peer review but has not been through the copyediting, typesetting, pagination and proofreading process, which may lead to differences between this version and the Version of Record. Please cite this article as doi: 10.1111/tra.12068
© 2013 John Wiley & Sons A/S
Abstarct
The endoplasmic reticulum-associated degradation (ERAD) machinery selects native and misfolded polypeptides
for dislocation across the ER membrane and proteasomal degradation. Regulated degradation of native proteins
is an important aspect of cell physiology. For example, it contributes to the control of lipid biosynthesis, calcium
homeostasis and ERAD capacity by setting the turnover rate of crucial regulators of these pathways. In contrast,
degradation of native proteins has pathologic relevance when caused by viral or bacterial infections, or when it
occurs as a consequence of dysregulated ERAD activity. The efficient disposal of misfolded proteins prevents
toxic depositions and persistent sequestration of molecular chaperones that could induce cellular stress and
perturb maintenance of cellular proteostasis.
In the first section of this review, we survey the available literature on mechanisms of selection of native and non-
native proteins for degradation from the ER and on how pathogens hijack them. In the second section, we
highlight the mechanisms of ERAD activity adaptation to changes in the ER environment with a particular
emphasis on the post-translational regulatory mechanisms collectively defined as ERAD tuning.
Introduction The cellular proteome is mostly synthesized by
cytosolic ribosomes to operate in the cytosol and,
upon appropriate targeting, in various intracellular
organelles or in the extracellular space. Cellular
compartments where protein folding occurs (e.g.,
the cytosol, mitochondria, the endoplasmic
reticulum (ER)) contain two classes of non-native
polypeptides: i) newly synthesized polypeptide
chains that must be assisted by folding chaperones
and enzymes to attain the native mono- or
oligomeric structure; ii) terminally misfolded
conformers that must efficiently be degraded to
prevent the formation of toxic deposits and the
persistent sequestration of chaperones that could
eventually inhibit the cellular protein folding capacity
and elicit stress (1-3) (Fig. 1A). The distinction
between the two classes of non-native chains, one
to be preserved, the second to be cleared from the
folding compartment is not an easy task for the
cellular quality control machineries. Selection for
disposal might be a stochastic process: the longer
the persistency of structural defects in the ER, the
greater is the probability to be selected for
destruction. Therefore, mutations that delay folding
may channel the polypeptide into destructive
pathways, even if they do not compromise the
function of the mutated protein.
In the ER, non-native, but also native proteins are
selected for degradation by components of the
ERAD machinery that deliver them at dislocation
sites embedded in the ER membrane. Dislocation
sites consist of a multitude of luminal and
membrane-bound specialized ER-resident proteins
as well as a number of cytosolic factors insuring
dislocation across the ER membrane, poly-
ubiquitylation and disposal of ERAD substrates by
26S proteasomes (Section A, Specificity of the
ERAD machinery). Dysregulated ERAD activity
caused by excessive luminal content of ERAD
factors may result in premature interruption of
ongoing folding attempts where proteins that would
have attained functional structures are
inappropriately destroyed thus causing loss-of-
function phenotypes or disorders (Fig. 1B). All in all,
balanced activity of the degradation machinery
crucially contributes to maintenance of protein
homeostasis (proteostasis) (Section B, Regulation
of the ERAD activity).
A. Specificity of the ERAD machinery
ERAD of native proteins in healthy cells: select
examples
The regulated degradation of functional proteins is a
crucial aspect of cellular physiology and contributes,
for example, to set the level of lipid biosynthesis, to
adjust calcium homeostasis, to determine the
constitutive level of the ERAD activity and to adapt
it to variations in misfolded proteins load (4, 5).
The ERAD machinery controls the intracellular
content of the 3-hydroxy-3-methyl-glutaryl-CoA
reductase (HMG-CoA reductase), a rate-limiting
enzyme in the synthesis of sterols from acetyl-CoA.
The HMG-CoA reductase turnover is enhanced
when the cellular sterol level is high, a classical
example of feedback regulation (6-8). Likewise,
ERAD factors may select the lipid carrier ApoB (9,
10) or the IP3P receptor (11) for destruction when
lipid levels are low or when cytosolic levels of IP3
and calcium are high, respectively.
Poorly studied, but crucial to maintain cellular
proteostasis, are the constitutive and the regulated
degradation of ERAD factors (5). ERAD factors
turnover may directly be affected by the presence of
misfolded polypeptides in the ER lumen and
contributes in determining the rapid adaptation of
the overall ERAD activity to changes in the ER
folding environment as described in Section B.
Degradation of native proteins triggered by
pathogens: select examples
Viruses and bacteria may dysregulate ERAD
pathways of infected cells to enhance their chances
to survive in the host, to generate their progeny and
to escape immunosurveillance (12, 13). This
highlights the impact that ERAD modulation may
have on cellular physiology and on protein
production.
The human cytomegalovirus (HCMV): One of the
most revealing examples of manipulation of the
equilibrium existing in eukaryotic cells between
maturation and disposal of newly synthesized
polypeptides relates to cells infected with HCMV.
These cells produce the viral proteins US2 and
US11 that select for disposal newly synthesized
class I or class II MHC (14-16). The intervention of
US2 and US11 anticipates the assembly of
complexes that bind viral epitopes in the ER lumen
and transport them at the cell surface for activation
of the host immune response. In infected cells,
class I and class II molecules are cleared from the
ER with intervention of conventional ERAD factors
(thoroughly described below) such as SEL1L, derlin
1, VIMP, p97/VCP and the E3 ubiquitin ligase TRC8
(17-19). Infected cells may also express the viral
protein Pp65 to inhibit proteasomal activity (20), a
strategy that HMCV shares with several other
viruses (Epstein-Barr virus (21), human
immunodeficiency virus (HIV) (22), hepatitis B virus
(HBV) (23), Kaposi sarcoma herpes virus (24)) to
elude immunosurveillance.
HIV: Cells infected with HIV express the viral
protein Vpu causing the proteasome-mediated
degradation of the viral receptor CD4 thereby
preventing superinfection (25-28).
The murine γ-Herpes virus 68 and the rodent
herpes virus Peru (RHVP): The expression of viral
E3 ubiquitin ligases is yet another strategy used by
pathogens to specifically clear host cell proteins that
could activate the immune response. The viral E3
ligase mK3 expressed in cells infected with murine
γ-Herpes virus 68 binds to and uses the
TAP/Tapasin complex as an adaptor to specifically
polyubiquitylate and destroy the class I MHC heavy
chain (29-32). Interestingly, the ubiquitin ligase
activity of mK3 is directed to serine and threonine in
addition to the conventional lysine residues (33).
The viral pK3 expressed in cells infected with RHVP
promotes proteasome-mediated degradation of the
class I MHC heavy chain (34).
The hepatitis C (HCV) and HBV viruses: Another
example of manipulation of the host cell ERAD
activity during the viral life cycle is reported for cells
infected with HCV (35) or HBV (36). ERAD
enhancement resulting from the ER stress-induced
up-regulation of proteins of the EDEM family (37)
reduces the fraction of newly synthesized viral
glycoproteins able to attain the native structure in
due time. Consistent with data showing that ERAD
enhancement interferes with completion of ongoing
folding programs (38-41), folding and assembly of
viral spikes becomes inefficient. This is proposed to
maintain low production of viral particles thus
contributing to infection persistency.
Degradation of misfolded proteins: specificity of
the ERAD machinery
Genomic defects, transcriptional and translational
errors may alter the amino acid composition or the
length of the polypeptide sequence. This may
prevent attainment of the native structure or delay
the folding process such that selection for disposal
of the mutated chains precedes completion of the
folding program. Intra- or extracellular accumulation
of folding-defective polypeptides causes gain-of-
toxic-function diseases, for example hereditary lung
emphysema and liver disease caused by mutant
forms of α1-antitrypsin or many types of
neurodegenerative disorders. On the other hand,
clearance of the aberrant gene products can result
in loss-of-function diseases, for example cystic
fibrosis or lysosomal storage diseases (thoroughly
reviewed elsewhere (42)). The development of
appropriate therapeutic approaches to contrast the
onset and the course of conformational (or protein
misfolding) diseases is of great interest. Such
diseases can individually be treated with
pharmacologic chaperones that specifically
enhance the folding-efficiency of a mutated gene
product (43). Alternatively, loss-of-function defects
could be rescued by targeting with therapeutic
agents the ER quality control machinery so that, as
one example, mutated polypeptides are offered
wider time windows to eventually attain the native
structure. Such approaches would greatly benefit of
the capacity to predict for each disease-causing
polypeptide, which chaperones and pathways will
be engaged for ER-retention, quality control and/or
disposal.
The presence of N-linked oligosaccharides
The oligosaccharyl transferase complex located at
the entry site of the ER transfers pre-assembled
glucose3-mannose9-N-acetyl glucosamine2-
oligosaccharides onto nascent polypeptide chains
entering the ER lumen (44). Normally, two terminal
glucose residues are rapidly removed by the
sequential intervention of the α-glucosidases I and
II. This generates a mono-glucosylated protein-
bound oligosaccharide that engages the lectin
chaperones calnexin and calreticulin and exposes
newly synthesized polypeptides to a folding
environment comprising the oxidoreductase ERp57
and the peptidyl-prolyl isomerase CypB. ERp57
promotes formation of the native set of disulfide
bonds, CypB the appropriate structuring of peptidyl-
prolyl bonds in the cis or in the trans configuration
(44).
Some nascent polypeptides rapidly enter off-
pathways of the folding program. This may inhibit
the action of the α-glucosidase II and results in the
inappropriate persistence of the di-glucosylated
form of protein-bound oligosaccharides. Aberrantly
structured newly synthesized polypeptides
displaying di-glucosylated oligosaccharides are
sequestered by a recently characterized membrane
anchored ER lectin, malectin (45). Malectin plays a
crucial role in retention of folding-defective
glycoproteins in the ER and acts in concert with
ribophorin I, a subunit of the ER glycosylation
machinery with proposed molecular chaperone
function (46, 47).
Persistent ER retention of misfolded conformers
elicits intervention of ER-resident mannosidases of
the glycosyl hydrolase 47 family (48) comprising the
ERManI, EDEM1, EDEM2, EDEM3. These directly
or indirectly enhance removal of α1,2-bonded
mannose residues (49-57) to extract misfolded
polypeptides from the calnexin chaperone system
(58) and to generate disposal signals decoded by
mannose-binding ERAD lectins such as OS-9 and
XTP3-B variants (50, 51, 59-62). The ERAD lectins,
which are interchangeable in function at least for
soluble ERAD substrates (ERAD-LS) (63), shuttle
misfolded polypeptides from the ER lumen to
dislocation sites in the ER membrane (Fig. 2). Both
the mannose-cleaving and the mannose-binding
ERAD factors also bind non-glycosylated proteins
(60, 61, 64-66) possibly as components of
supramolecular complexes containing general
chaperones such as BiP and GRP94 that direct
their action towards terminally misfolded proteins
(67).
The position of the folding defect and the
topology of the misfolded protein
E3 ubiquitin ligases embedded in the ER membrane
participate in supramolecular complexes containing
membrane-anchored and peripherally associated
factors both at the luminal and at the cytosolic side
of the bilayer. These multimeric complexes, the
dislocons, deliver misfolded proteins from the ER
lumen into the cytosol for proteasome-mediated
degradation (Fig. 2).
In S. cerevisiae, dislocons are built around two E3
ubiquitin ligases, Hrd1p and Doa10p. The luminal
(ERAD-L), transmembrane (ERAD-M) or cytosolic
(ERAD-C) position of the folding defect may
determine the engagement of either one of them.
Hrd1p preferentially assists ERAD-L and ERAD-M
substrates (68-72); Doa10p assists ERAD-C
substrates (68, 69, 73). The two yeast E3 ligases
have redundant function in assisting polytopic,
folding-defective polypeptides such as the ΔF508
cystic fibrosis transmembrane regulator (CFTR)
(74).
The mammalian ER membrane contains at least 24
RING-finger E3 ubiquitin ligases (75), some of
which (e.g., HRD1, gp78, RNF5, TEB4, RFP2,
TRC8) have a documented role in ERAD (76). The
ERAD system in Metazoa is therefore much more
complex and redundant than in Fungi. Only very
few attempts have been performed to systematically
establish how changes in the biophysical features of
misfolded polypeptides determine the engagement
of specific dislocation factors. For example,
misfolded luminal modules (ERAD-LS substrates)
strongly depend on the supramolecular complex
built around HRD1, comprising the associated
adaptor SEL1L and the two interchangeable ERAD
lectins OS-9 and XTP3-B that deliver the misfolded
polypeptides from the ER lumen to the dislocation
site. The same misfolded modules tethered at the
ER membrane (ERAD-LM substrates) are efficiently
cleared from the ER even in cells with non-
functional HRD1 dislocons, possibly because lateral
diffusion in the lipid bilayer facilitates delivery to
alternative machineries (Fig. 2) (63, 77).
The disposal of orphan/misfolded membrane
proteins: select examples
The study of the fate of orphan subunits of
oligomeric complexes is of historical importance.
Klausner and colleagues crucially reported that
unassembled subunits of the T cell receptor (TCR)
are degraded in a pre-lysosomal compartment
being part or closely related to the ER (78). Since
then, several TCR subunits, namely TCRα, TCRβ
and CD3δ have become model substrates to
investigate the mechanisms of protein disposal from
the ER (79-86). More recently, CD147 a component
of several membrane transporters, has been
identified as an endogenous ERAD substrate
whose turnover may regulate expression of the
corresponding functional complexes (87). The
peculiarity of all these proteins is the presence of
charged residues in the intramembrane space.
These residues promote the assembly of functional
complexes by pairing with residues of opposite
charge present in the transmembrane domains of
partner polypeptides in oligomeric complexes.
When oligomerization fails, the intramembrane
domains displaying charged residues might
facilitate the rapid degradation of the orphan
subunits by maintaining them in a monomeric state
and by recruiting specific ERAD factors (86, 88-90).
They may also serve, in some specific case, as
intramembrane cleavage sites that may facilitate
extraction from the ER membrane of the orphan
subunit to be degraded (91). TCRα and CD3δ are
both type I glycopolypeptides with charged residues
in the intramembrane space. Yet, their requirements
for efficient degradation differ quite extensively, thus
showing how difficult it may be to predict factors
and pathways engaged during specific polypeptides
quality control. For instance, only degradation of
CD3δ requires extensive N-glycans de-
mannosylation and only the cytosolic dislocation of
CD3δ is coupled with proteasomal activity (82).
Significantly, the cytosolic domain of TCRα is poly-
ubiquitylated on serine residues (85), rather than on
the more conventional lysine residues. Serine,
cysteine and threonine residues as well as the
polypeptide N-terminus are alternative ubiquitin
acceptor sites (33, 92-94).
The evolution of transmembrane domains
displaying destabilizing charged residues is one of
the strategies developed by viruses to co-opt the
mammalian dislocation machinery during the
infection cycle. This has been reported for simian
virus 40, where a charged residue in the
membrane-inserted domain of the VP2 protein,
which is conserved in several other polyomaviruses,
engages the ERAD factor BAP31 to possibly
promote dislocation of the entire virion across the
ER membrane (90).
The multispanning CFTR protein has also
extensively been described. It is characterized by
low folding-efficiency, about 25%, which is further
decreased upon gene mutations (95-97). The
ΔF508CFTR mutant form was the first reported
example of involvement of cytosolic programs in the
clearance of folding-defective polypeptides from the
mammalian ER (98, 99). This cystic fibrosis-causing
defective gene product is a paradigm for all mutant
proteins that maintain their function (100), yet are
rapidly destroyed from the ER (98, 99) or from the
cell surface (101) because structurally unstable.
This inevitably results in a loss-of-function protein
folding disease. Such mutants, or the quality control
pathways that they engage, are or may become
targets of therapeutic intervention based on the use
of chemical or pharmacologic chaperones as well
as proteostasis modifiers (95, 102). This alone
justifies the importance of deciphering the
mechanisms regulating protein quality control at the
molecular level.
The needs for unfolding
Many models (and at least as many candidates for
a channel in the ER membrane (103-105)) have
been proposed to explain how misfolded
polypeptides, tightly folded domains, catalytic
subunits of AB toxins (e.g., ricin, cholera, Shiga-
like) and even entire viral particles are dislocated
across the ER membrane. This remains poorly
understood but it relies on the intervention of
several luminal, cytosolic and membrane bound
factors including BiP, BAP31 and BAP29 (90, 106),
EDEM1 (107, 108), SEL1L (109), derlins (110-112),
HRD1 (113, 114), gp78 (114), p97/VCP (115, 116)
and many others.
Seemingly contrasting data are available on the
requirement for polypeptides unfolding to facilitate
transport across the lipid bilayer. For example, it
has been shown that the tightly folded DHFR
protein does not affect dislocation when appended
to class I MHC in US2 and US11-expressing cells
(117, 118). Moreover, compelling data do exist
showing that virions can dislocate across the ER
membrane and that misfolded glycopolypeptides,
which display bulky, highly hydrophilic
oligosaccharides bound to the polypeptide
backbone can efficiently pass the lipid bilayer to be
exported into the cytosol. However, other data imply
that a certain degree of unfolding is required for
efficient dislocation. For example, in contrast to
reference (117), DHFR appended to ERAD
substrates in non-infected cells may substantially
impair dislocation (119). Moreover, several
evidence highlight the involvement of members of
the protein disulfide isomerase (PDI) family in the
preparation of misfolded polypeptides for dislocation
across the ER membrane and in transport across
the bilayer of virions and of catalytic subunits of
toxins. For example, intra- (120) and inter-molecular
disulfide bonds (121) in ERAD substrates as well as
interchain disulfides linking the regulatory and
catalytic subunits of bacterial toxins are reduced
with the intervention of PDI (122-126) and/or PDI
family members (e.g., ERdj5 (127-129), ERp57
(106), ERp72, ERp29 (130), TMX1 (131), ERFAD-
ERp90 (132) and ERO1 (133)).
Recent work from our lab showed that the
conversion of cis into trans peptidyl-prolyl bonds by
the peptidyl-prolyl cis/trans isomerase CyPB may
facilitate transport of misfolded polypeptides
through the elusive transmembrane dislocation
channel by unfolding the polypeptide chain (134).
Finally, a role of rhomboid proteases and
pseudoproteases in ERAD substrates extraction
from the ER has been proposed and relates to their
capacity to cleave intramembrane anchors or to
cause bilayer thinning, respectively (91, 135, 136).
B. Regulation of the ERAD activity
Physiologic and pathologic destruction of
nascent chains
Contrasting data are available on the overall
fraction of nascent chains degraded before
attainment of the native structure, i.e., of defective
ribosomal products (DRiPS). Values range from
more than 30% (137) to substantially less (138).
DRiPs include polypeptides that have failed the
folding program. In this context, individual
mammalian polypeptides are characterized by
specific folding efficiencies (as low as 25% for the
CFTR, approaching the 90% for α1AT (60)). DRiPs
may also derive from defective mRNA or may be
characterized by errors in the primary sequence
that occur when the genetic information is
converted into proteins and most frequently result
from tRNA-aminoacid mis-acylation. If strictly
monitored by quality control programs, the relative
inefficiency of the protein biogenesis pathways is
fully compatible with life as it warrants production of
sufficient amount of functional proteins that keep
cells, tissues and organisms running. It probably
offers evolutionary advantages; DRiPs have been
proposed to provide ligands for class I MHC
presentation, thus enabling the immune system to
rapidly detect alterations in cellular gene expression
possibly caused by pathogen infection or
tumorogenic deviance (139).
A dysregulated ERAD activity may substantially
contribute to shift the physiological inefficiency of
protein folding to a pathological condition. A
constitutive ERAD activity surveys the normal
production of by-products of protein biogenesis
thereby contrasting their toxic accumulation. If the
constitutive ERAD activity is insufficient, folding-
defective polypeptides may remain in the ER lumen
thereby eventually interfering with protein
biogenesis and secretion upon, as one example,
persistent sequestration of folding chaperones (41,
140, 141). In contrast, excessive ERAD activity
would drastically reduce the time allocated to
nascent chains for maturation, thus causing loss-of-
function phenotypes and diseases (19, 34, 35, 38-
40, 142-149).
Understanding ERAD activity regulation is one of
the fascinating questions addressed in several
laboratories working on cellular proteostasis. The
transcriptional/translational induction of ERAD
factors upon activation of unfolded protein response
(UPR) programs is the best studied mechanism
operating in eukaryotic cells to adapt ERAD (and
folding) activity to changes in cellular needs (150).
UPR activation may optimally respond to long-
lasting (chronic) ER stresses. It seems however
inappropriate to respond to transient, acute and/or
periodic fluctuations in ER cargo load. In fact, onset
of these programs has a latency of several hours (2,
151). Moreover, the recovery from a stress requires
activation of elusive mechanisms that must reduce
the size of the ER after the UPR-triggered
expansion and must remove the excess of
chaperones produced during the ER stress phase.
These might be very slow processes because ER
stress-induced chaperones and enzymes such as
PDI family members, calnexin, calreticulin, BiP have
half-lives above the 24 h (152).
We propose that in healthy eukaryotic cells, the
constitutive ERAD that must cope with the
physiological production of by-products of protein
biogenesis without interfering with ongoing folding
programs is controlled by mechanisms collectively
defined as ERAD tuning. These mechanisms
survey the turn-over, the segregation from the ER
and the engagement of ERAD factors in
supramolecular functional complexes (5).
The concept of ERAD tuning
The concept of ERAD tuning is based on three
observations: i) unlike conventional ER-resident
chaperones and enzymes, several ERAD factors
(e.g., ERManI (153, 154), EDEM1 (38, 155-157),
OS-9 (149), XTP3-B (59), HERP (158, 159), SEL1L
(160, 161), the E3 ligases SMURF1 (162, 163) and
gp78 (164, 165), JAMP (166), ataxin-3 (167, 168))
are subjected to fast turnover, which may involve
the ubiquitin proteasome system, autophagy or
autophagy-like pathways; ii) select ERAD factors
are constitutively segregated from the ER (149,
169); iii) luminal expression of misfolded
polypeptides may delay the turnover of ERAD
factors, may retain them in the ER by interfering
with their vesicle-mediated segregation from the
compartment and may directly affect the
composition of supramolecular ERAD complexes
thereby setting their activity (149, 170, 171) (Fig. 3).
The concept of ERAD tuning proposes that
interactions with misfolded proteins synthesized in
the ER directly regulate (tune) the abundance, the
localization and the activity of components of the
ERAD machinery. Misfolded polypeptides may
support the assembly (or inhibit the disassembly) of
active supramolecular ERAD complexes as
reported, for example, for the association of the
adaptor protein SEL1L with the ER membrane-
embedded HRD1 dislocation machinery (149).
Moreover, since E3 ligases may ubiquitylate
themselves (164, 165, 172-174) and other
components of the ERAD machinery that are
engaged with them in supramolecular complexes
(158-160, 164, 165, 168), a possible scenario is that
folding-defective polypeptides serve as preferred
acceptors for the ubiquitylating activity of the E3
ligases thereby protecting the ERAD machinery
from self-destruction (Fig. 3).
The concept of ERAD tuning implies that misfolded
proteins may directly enhance the activity of the
ERAD machinery by a sort of autocrine regulatory
mechanism(s) that controls turnover, localization
and assembly of ERAD components (Fig. 3). In this
scenario, rapid adaptation, i.e., enhancement and
inhibition of ERAD activity, does not require signal
transduction from the ER to the nucleus, as it is the
case when the UPR must be activated. All in all, the
ERAD tuning pathways may offer rapid and readily
reversible adaptation responses to deal with
transient problems that may arise in the folding
compartment.
Interestingly, pathogens such as the mouse
hepatitis virus have been shown to hijack ERAD
tuning pathways to co-opt ER-derived vesicles
containing segregated ERAD factors as platforms
for replication of the viral genome (149, 156).
Conclusion The capacity to distinguish between non-native
polypeptides to be retained in the folding
compartment to complete the maturation program
and non-native polypeptides that must be removed
from the ER to prevent their toxic accumulation is
crucial to maintain cellular proteostasis.
Dysregulated ERAD may lead to inappropriate,
premature selection of folding-competent
conformers for destruction (too high activity) or to
an equally inappropriate and harmful tolerance of
misfolded conformers in the folding-compartment
(too weak activity). As these conditions inevitably
affect maintenance of cellular and organisms
proteostasis, the molecular characterization of the
processes covered by this review is of daunting
importance. What are the mechanisms that
maintain the fragile equilibrium between the activity
of the folding and the degradation machineries
operating in the ER and in other cellular
compartments such as the cytosol and the
mitochondria where not-yet-native proteins must
attain their functional conformations, yet misfolded
conformers must efficiently be cleared? How is this
equilibrium maintained upon the frequent
modifications of the environmental conditions cells
are subjected to? How do cells revert situations of
disequilibrium that may intervene upon pathogen
attack, nutrient deprivation, variations in protein
synthesis levels, transient failure of folding
programs? How do pathogens actually exploit the
host protein folding and degradation machineries to
enhance their survival and replication chances?
How can we intervene to contrast their infection
cycles? These are few of the challenging questions
remaining for future research.
Acknowledgments Members of the Molinari’s lab are acknowledged for
discussions and suggestions. M.M. is supported by
grants from the Foundation for Research on
Neurodegenerative Diseases, the Swiss National
Science Foundation, the Association Française
contre les Myopathies, the Gabriele Foundation.
1. Balch WE, Morimoto RI, Dillin A, Kelly JW. Adapting proteostasis for disease intervention. Science 2008;319(5865):916‐919. 2. Walter P, Ron D. The unfolded protein response: from stress pathway to homeostatic regulation. Science 2011;334(6059):1081‐1086. 3. Molinari M. N‐glycan structure dictates extension of protein folding or onset of disposal. Nat Chem Biol 2007;3(6):313‐320. 4. Hampton RY, Garza RM. Protein quality control as a strategy for cellular regulation: lessons from ubiquitin‐mediated regulation of the sterol pathway. Chem Rev 2009;109(4):1561‐1574. 5. Bernasconi R, Molinari M. ERAD and ERAD tuning: disposal of cargo and of ERAD regulators from the mammalian ER. Curr Opin Cell Biol 2011;23(2):176‐183. 6. Gardner RG, Hampton RY. A highly conserved signal controls degradation of 3‐hydroxy‐3‐methylglutaryl‐coenzyme A (HMG‐CoA) reductase in eukaryotes. The Journal of biological chemistry 1999;274(44):31671‐31678. 7. Hampton RY, Gardner RG, Rine J. Role of 26S proteasome and HRD genes in the degradation of 3‐hydroxy‐3‐ methylglutaryl‐CoA reductase, an integral endoplasmic reticulum membrane protein. Mol Biol Cell 1996;7(12):2029‐2044.
8. Sever N, Song BL, Yabe D, Goldstein JL, Brown MS, DeBose‐Boyd RA. Insig‐dependent ubiquitination and degradation of mammalian 3‐hydroxy‐3‐methylglutaryl‐CoA reductase stimulated by sterols and geranylgeraniol. The Journal of biological chemistry 2003;278(52):52479‐52490. 9. Dixon JL, Furukawa S, Ginsberg HN. Oleate stimulates secretion of apolipoprotein B‐containing lipoproteins from Hep G2 cells by inhibiting early intracellular degradation of apolipoprotein B. The Journal of biological chemistry 1991;266(8):5080‐5086. 10. Zhou M, Fisher EA, Ginsberg HN. Regulated Co‐translational ubiquitination of apolipoprotein B100. A new paradigm for proteasomal degradation of a secretory protein. The Journal of biological chemistry 1998;273(38):24649‐24653. 11. Alzayady KJ, Panning MM, Kelley GG, Wojcikiewicz RJ. Involvement of the p97‐Ufd1‐Npl4 complex in the regulated endoplasmic reticulum‐associated degradation of inositol 1,4,5‐trisphosphate receptors. The Journal of biological chemistry 2005;280(41):34530‐34537. 12. Loureiro J, Ploegh HL. Antigen presentation and the ubiquitin‐proteasome system in host‐pathogen interactions. Adv Immunol 2006;92:225‐305. 13. Randow F, Lehner PJ. Viral avoidance and exploitation of the ubiquitin system. Nat Cell Biol 2009;11(5):527‐534. 14. Wiertz EJ, Jones TR, Sun L, Bogyo M, Geuze HJ, Ploegh HL. The human cytomegalovirus US11 gene product dislocates MHC class I heavy chains from the endoplasmic reticulum to the cytosol. Cell 1996;84(5):769‐779. 15. Wiertz EJ, Tortorella D, Bogyo M, Yu J, Mothes W, Jones TR, Rapoport TA,
Ploegh HL. Sec61‐mediated transfer of a membrane protein from the endoplasmic reticulum to the proteasome for destruction. Nature 1996;384(6608):432‐438. 16. Tomazin R, Boname J, Hegde NR, Lewinsohn DM, Altschuler Y, Jones TR, Cresswell P, Nelson JA, Riddell SR, Johnson DC. Cytomegalovirus US2 destroys two components of the MHC class II pathway, preventing recognition by CD4+ T cells. Nat Med 1999;5(9):1039‐1043. 17. Lilley BN, Ploegh HL. A membrane protein required for dislocation of misfolded proteins from the ER. Nature 2004;429(6994):834‐840. 18. Ye Y, Shibata Y, Yun C, Ron D, Rapoport TA. A membrane protein complex mediates retro‐translocation from the ER lumen into the cytosol. Nature 2004;429(6994):841‐847. 19. Stagg HR, Thomas M, van den Boomen D, Wiertz EJ, Drabkin HA, Gemmill RM, Lehner PJ. The TRC8 E3 ligase ubiquitinates MHC class I molecules before dislocation from the ER. J Cell Biol 2009;186(5):685‐692. 20. Gilbert MJ, Riddell SR, Plachter B, Greenberg PD. Cytomegalovirus selectively blocks antigen processing and presentation of its immediate‐early gene product. Nature 1996;383(6602):720‐722. 21. Masucci MG. Epstein‐Barr virus oncogenesis and the ubiquitin‐proteasome system. Oncogene 2004;23(11):2107‐2115. 22. Remoli AL, Marsili G, Perrotti E, Gallerani E, Ilari R, Nappi F, Cafaro A, Ensoli B, Gavioli R, Battistini A. Intracellular HIV‐1 Tat protein represses constitutive LMP2 transcription increasing proteasome activity by interfering with the binding of IRF‐1 to STAT1. Biochem J 2006;396(2):371‐380.
23. Zhang Z, Protzer U, Hu Z, Jacob J, Liang TJ. Inhibition of cellular proteasome activities enhances hepadnavirus replication in an HBX‐dependent manner. J Virol 2004;78(9):4566‐4572. 24. Zaldumbide A, Ossevoort M, Wiertz EJ, Hoeben RC. In cis inhibition of antigen processing by the latency‐associated nuclear antigen I of Kaposi sarcoma herpes virus. Mol Immunol 2007;44(6):1352‐1360. 25. Schubert U, Anton LC, Bacik I, Cox JH, Bour S, Bennink JR, Orlowski M, Strebel K, Yewdell JW. CD4 glycoprotein degradation induced by human immunodeficiency virus type 1 Vpu protein requires the function of proteasomes and the ubiquitin‐conjugating pathway. J Virol 1998;72(3):2280‐2288. 26. Willey RL, Maldarelli F, Martin MA, Strebel K. Human immunodeficiency virus type 1 Vpu protein induces rapid degradation of CD4. J Virol 1992;66(12):7193‐7200. 27. Fujita K, Omura S, Silver J. Rapid degradation of CD4 in cells expressing human immunodeficiency virus type 1 Env and Vpu is blocked by proteasome inhibitors. J Gen Virol 1997;78 ( Pt 3):619‐625. 28. Margottin F, Bour SP, Durand H, Selig L, Benichou S, Richard V, Thomas D, Strebel K, Benarous R. A novel human WD protein, h‐beta TrCp, that interacts with HIV‐1 Vpu connects CD4 to the ER degradation pathway through an F‐box motif. Mol Cell 1998;1(4):565‐574. 29. Lybarger L, Wang X, Harris MR, Virgin HWt, Hansen TH. Virus subversion of the MHC class I peptide‐loading complex. Immunity 2003;18(1):121‐130. 30. Boname JM, Stevenson PG. MHC class I ubiquitination by a viral PHD/LAP finger protein. Immunity 2001;15(4):627‐636.
31. Yu YY, Harris MR, Lybarger L, Kimpler LA, Myers NB, Virgin HWt, Hansen TH. Physical association of the K3 protein of gamma‐2 herpesvirus 68 with major histocompatibility complex class I molecules with impaired peptide and beta(2)‐microglobulin assembly. J Virol 2002;76(6):2796‐2803. 32. Boname JM, de Lima BD, Lehner PJ, Stevenson PG. Viral degradation of the MHC class I peptide loading complex. Immunity 2004;20(3):305‐317. 33. Wang X, Herr RA, Chua WJ, Lybarger L, Wiertz EJ, Hansen TH. Ubiquitination of serine, threonine, or lysine residues on the cytoplasmic tail can induce ERAD of MHC‐I by viral E3 ligase mK3. The Journal of cell biology 2007;177(4):613‐624. 34. Herr RA, Wang X, Loh J, Virgin HW, Hansen TH. Newly Discovered Viral E3 Ligase pK3 Induces Endoplasmic Reticulum‐associated Degradation of Class I Major Histocompatibility Proteins and Their Membrane‐bound Chaperones. The Journal of biological chemistry 2012;287(18):14467‐14479. 35. Saeed M, Suzuki R, Watanabe N, Masaki T, Tomonaga M, Muhammad A, Kato T, Matsuura Y, Watanabe H, Wakita T, Suzuki T. Role of the endoplasmic reticulum‐associated degradation (ERAD) pathway in degradation of hepatitis C virus envelope proteins and production of virus particles. The Journal of biological chemistry 2011;286(43):37264‐37273. 36. Lazar C, Macovei A, Petrescu S, Branza‐Nichita N. Activation of ERAD pathway by human hepatitis B virus modulates viral and subviral particle production. PLoS One 2012;7(3):e34169. 37. Olivari S, Molinari M. Glycoprotein folding and the role of EDEM1, EDEM2 and EDEM3 in degradation of folding‐defective
glycoproteins. FEBS Lett 2007;581(19):3658‐3664. 38. Cali T, Galli C, Olivari S, Molinari M. Segregation and rapid turnover of EDEM1 by an autophagy‐like mechanism modulates standard ERAD and folding activities. Biochem Biophys Res Commun 2008;371(3):405‐410. 39. Wu Y, Swulius MT, Moremen KW, Sifers RN. Elucidation of the molecular logic by which misfolded alpha 1‐antitrypsin is preferentially selected for degradation. Proc Natl Acad Sci U S A 2003;100(14):8229‐8234. 40. Younger JM, Chen L, Ren HY, Rosser MF, Turnbull EL, Fan CY, Patterson C, Cyr DM. Sequential quality‐control checkpoints triage misfolded cystic fibrosis transmembrane conductance regulator. Cell 2006;126(3):571‐582. 41. Eriksson KK, Vago R, Calanca V, Galli C, Paganetti P, Molinari M. EDEM contributes to maintenance of protein folding efficiency and secretory capacity. J Biol Chem 2004;279(43):44600‐44605. 42. Powers ET, Morimoto RI, Dillin A, Kelly JW, Balch WE. Biological and chemical approaches to diseases of proteostasis deficiency. Annu Rev Biochem 2009;78:959‐991. 43. Bernier V, Lagace M, Bichet DG, Bouvier M. Pharmacological chaperones: potential treatment for conformational diseases. Trends Endocrinol Metab 2004;15(5):222‐228. 44. Aebi M, Bernasconi R, Clerc S, Molinari M. N‐glycan structures: recognition and processing in the ER. Trends Biochem Sci 2010;35(2):74‐82. 45. Galli C, Bernasconi R, Solda T, Calanca V, Molinari M. Malectin participates in a backup glycoprotein quality control pathway in the mammalian ER. PLoS One 2011;6(1):e16304. 46. Qin SY, Hu D, Matsumoto K, Takeda K, Matsumoto N, Yamaguchi Y,
Yamamoto K. Malectin forms a complex with ribophorin I for enhanced association with misfolded glycoproteins. The Journal of biological chemistry 2012;287(45):38080‐38089. 47. Wilson CM, Kraft C, Duggan C, Ismail N, Crawshaw SG, High S. Ribophorin I associates with a subset of membrane proteins after their integration at the sec61 translocon. J Biol Chem 2005;280(6):4195‐4206. 48. Moremen KW, Molinari M. N‐linked glycan recognition and processing: the molecular basis of endoplasmic reticulum quality control. Curr Opin Struct Biol 2006(16):592‐599. 49. Olivari S, Cali T, Salo KE, Paganetti P, Ruddock LW, Molinari M. EDEM1 regulates ER‐associated degradation by accelerating de‐mannosylation of folding‐defective polypeptides and by inhibiting their covalent aggregation. Biochem Biophys Res Commun 2006;349(4):1278‐1284. 50. Clerc S, Hirsch C, Oggier DM, Deprez P, Jakob C, Sommer T, Aebi M. Htm1 protein generates the N‐glycan signal for glycoprotein degradation in the endoplasmic reticulum. J Cell Biol 2009;184:159‐172. 51. Quan EM, Kamiya Y, Kamiya D, Denic V, Weibezahn J, Kato K, Weissman JS. Defining the glycan destruction signal for endoplasmic reticulum‐associated degradation. Mol Cell 2008;32(6):870‐877. 52. Kitzmuller C, Caprini A, Moore SE, Frenoy JP, Schwaiger E, Kellermann O, Ivessa NE, Ermonval M. Processing of N‐linked glycans during endoplasmic‐reticulum‐associated degradation of a short‐lived variant of ribophorin I. Biochem J 2003;376(Pt 3):687‐696. 53. Hosokawa N, Tremblay LO, You Z, Herscovics A, Wada I, Nagata K. Enhancement of endoplasmic reticulum (ER) degradation of misfolded Null Hong Kong alpha1‐antitrypsin by
human ER mannosidase I. J Biol Chem 2003;278(28):26287‐26294. 54. Frenkel Z, Gregory W, Kornfeld S, Lederkremer GZ. Endoplasmic reticulum‐associated degradation of mammalian glycoproteins involves sugar chain trimming to Man6‐5GlcNAc2. J Biol Chem 2003;278(36):34119‐34124. 55. Foulquier F, Duvet S, Klein A, Mir AM, Chirat F, Cacan R. Endoplasmic reticulum‐associated degradation of glycoproteins bearing Man5GlcNAc2 and Man9GlcNAc2 species in the MI8‐5 CHO cell line. Eur J Biochem 2004;271(2):398‐404. 56. Foulquier F, Harduin‐Lepers A, Duvet S, Marchal I, Mir AM, Delannoy P, Chirat F, Cacan R. The unfolded protein response in a dolichyl phosphate mannose‐deficient Chinese hamster ovary cell line points out the key role of a demannosylation step in the quality‐control mechanism of N‐glycoproteins. Biochem J 2002;362(Pt 2):491‐498. 57. Ermonval M, Kitzmuller C, Mir AM, Cacan R, Ivessa NE. N‐glycan structure of a short‐lived variant of ribophorin I expressed in the MadIA214 glycosylation‐defective cell line reveals the role of a mannosidase that is not ER mannosidase I in the process of glycoprotein degradation. Glycobiology 2001;11(7):565‐576. 58. Molinari M, Calanca V, Galli C, Lucca P, Paganetti P. Role of EDEM in the release of misfolded glycoproteins from the calnexin cycle. Science 2003;299(5611):1397‐1400. 59. Hosokawa N, Wada I, Nagasawa K, Moriyama T, Okawa K, Nagata K. Human XTP3‐B forms an endoplasmic reticulum quality control scaffold with the HRD1‐SEL1L ubiquitin ligase complex and BiP. J Biol Chem 2008;283(30):20914‐20924. 60. Bernasconi R, Pertel T, Luban J, Molinari M. A Dual Task for the Xbp1‐responsive OS‐9 Variants in the
Mammalian Endoplasmic Reticulum: Inhibiting Secretion of Misfolded Protein Conformers and Enhancing their Disposal. J Biol Chem 2008;283(24):16446‐16454. 61. Christianson JC, Shaler TA, Tyler RE, Kopito RR. OS‐9 and GRP94 deliver mutant alpha1‐antitrypsin to the Hrd1/SEL1L ubiquitin ligase complex for ERAD. Nat Cell Biol 2008;10(3):272‐282. 62. Alcock F, Swanton E. Mammalian OS‐9 is upregulated in response to endoplasmic reticulum stress and facilitates ubiquitination of misfolded glycoproteins. J Mol Biol 2009;385(4):1032‐1042. 63. Bernasconi R, Galli C, Calanca V, Nakajima T, Molinari M. Stringent requirement for HRD1, SEL1L, and OS‐9/XTP3‐B for disposal of ERAD‐LS substrates. J Cell Biol 2010;188(2):223‐235. 64. Cormier JH, Tamura T, Sunryd JC, Hebert DN. EDEM1 recognition and delivery of misfolded proteins to the SEL1L‐containing ERAD complex. Mol Cell 2009;34(5):627‐633. 65. Ron E, Shenkman M, Groisman B, Izenshtein Y, Leitman J, Lederkremer GZ. Bypass of glycan‐dependent glycoprotein delivery to ERAD by up‐regulated EDEM1. Mol Biol Cell 2011;22(21):3945‐3954. 66. Shenkman M, Groisman B, Ron E, Avezov E, Hendershot LM, Lederkremer GZ. A Shared Endoplasmic Reticulum‐associated Degradation Pathway Involving the EDEM1 Protein for Glycosylated and Nonglycosylated Proteins. The Journal of biological chemistry 2013;288(4):2167‐2178. 67. Hebert DN, Molinari M. Flagging and docking: dual roles for N‐glycans in protein quality control and cellular proteostasis. Trends Biochem Sci 2012;37(10):404‐410. 68. Vashist S, Ng DT. Misfolded proteins are sorted by a sequential
checkpoint mechanism of ER quality control. J Cell Biol 2004;165(1):41‐52. 69. Huyer G, Piluek WF, Fansler Z, Kreft SG, Hochstrasser M, Brodsky JL, Michaelis S. Distinct machinery is required in Saccharomyces cerevisiae for the endoplasmic reticulum‐associated degradation of a multispanning membrane protein and a soluble luminal protein. J Biol Chem 2004;279(37):38369‐38378. 70. Taxis C, Hitt R, Park SH, Deak PM, Kostova Z, Wolf DH. Use of modular substrates demonstrates mechanistic diversity and reveals differences in chaperone requirement of ERAD. J Biol Chem 2003;278(38):35903‐35913. 71. Willer M, Forte GM, Stirling CJ. Sec61p is required for ERAD‐L: genetic dissection of the translocation and ERAD‐L functions of Sec61P using novel derivatives of CPY. J Biol Chem 2008;283(49):33883‐33888. 72. Carvalho P, Goder V, Rapoport TA. Distinct ubiquitin‐ligase complexes define convergent pathways for the degradation of ER proteins. Cell 2006;126(2):361‐373. 73. Metzger MB, Michaelis S. Analysis of quality control substrates in distinct cellular compartments reveals a unique role for Rpn4p in tolerating misfolded membrane proteins. Mol Biol Cell 2009;20(3):1006‐1019. 74. Gnann A, Riordan JR, Wolf DH. Cystic fibrosis transmembrane conductance regulator degradation depends on the lectins Htm1p/EDEM and the Cdc48 protein complex in yeast. Mol Biol Cell 2004;15(9):4125‐4135. 75. Neutzner A, Neutzner M, Benischke AS, Ryu SW, Frank S, Youle RJ, Karbowski M. A systematic search for endoplasmic reticulum (ER) membrane‐associated RING finger proteins identifies Nixin/ZNRF4 as a regulator of calnexin stability and ER homeostasis. The Journal of biological chemistry 2011;286(10):8633‐8643.
76. Claessen JH, Kundrat L, Ploegh HL. Protein quality control in the ER: balancing the ubiquitin checkbook. Trends Cell Biol 2012;22(1):22‐32. 77. Ninagawa S, Okada T, Takeda S, Mori K. SEL1L is required for endoplasmic reticulum‐associated degradation of misfolded luminal proteins but not transmembrane proteins in chicken DT40 cell line. Cell Struct Funct 2011;36(2):187‐195. 78. Lippincott‐Schwartz J, Bonifacino JS, Yuan LC, Klausner RD. Degradation from the endoplasmic reticulum: disposing of newly synthesized proteins. Cell 1988;54(2):209‐220. 79. Huppa JB, Ploegh HL. The alpha chain of the T cell antigen receptor is degraded in the cytosol. Immunity 1997;7(1):113‐122. 80. DeLaBarre B, Christianson JC, Kopito RR, Brunger AT. Central pore residues mediate the p97/VCP activity required for ERAD. Mol Cell 2006;22(4):451‐462. 81. Wang Q, Li L, Ye Y. Regulation of retrotranslocation by p97‐associated deubiquitinating enzyme ataxin‐3. J Cell Biol 2006;174(7):963‐971. 82. Yang M, Omura S, Bonifacino JS, Weissman AM. Novel aspects of degradation of T cell receptor subunits from the ER in T cells: importance of oligosaccharide processing, ubiquitination, and proteasome‐dependent removal from ER membranes. J Exp Med 1998;187(6):835‐846. 83. Yu H, Kaung G, Kobayashi S, Kopito RR. Cytosolic degradation of T‐cell receptor alpha chains by the proteasome. J Biol Chem 1997;272(33):20800‐20804. 84. Young J, Kane LP, Exley M, Wileman T. Regulation of selective protein degradation in the endoplasmic reticulum by redox potential. J Biol Chem 1993;268(26):19810‐19818.
85. Ishikura S, Weissman AM, Bonifacino JS. Serine residues in the cytosolic tail of the T‐cell antigen receptor alpha‐chain mediate ubiquitination and endoplasmic reticulum‐associated degradation of the unassembled protein. The Journal of biological chemistry 2010;285(31):23916‐23924. 86. Soetandyo N, Wang Q, Ye Y, Li L. Role of intramembrane charged residues in the quality control of unassembled T‐cell receptor alpha‐chains at the endoplasmic reticulum. J Cell Sci 2010;123(Pt 7):1031‐1038. 87. Tyler RE, Pearce MM, Shaler TA, Olzmann JA, Greenblatt EJ, Kopito RR. Unassembled CD147 is an endogenous ER‐associated degradation (ERAD) substrate. Mol Biol Cell 2012;23(24):4668‐4678. 88. Bonifacino JS, Cosson P, Klausner RD. Colocalized transmembrane determinants for ER degradation and subunit assembly explain the intracellular fate of TCR chains. Cell 1990;63(3):503‐513. 89. Bonifacino JS, Cosson P, Shah N, Klausner RD. Role of potentially charged transmembrane residues in targeting proteins for retention and degradation within the endoplasmic reticulum. Embo J 1991;10(10):2783‐2793. 90. Geiger R, Andritschke D, Friebe S, Herzog F, Luisoni S, Heger T, Helenius A. BAP31 and BiP are essential for dislocation of SV40 from the endoplasmic reticulum to the cytosol. Nat Cell Biol 2011;13(11):1305‐1314. 91. Fleig L, Bergbold N, Sahasrabudhe P, Geiger B, Kaltak L, Lemberg MK. Ubiquitin‐dependent intramembrane rhomboid protease promotes ERAD of membrane proteins. Mol Cell 2012;47(4):558‐569. 92. Cadwell K, Coscoy L. Ubiquitination on nonlysine residues by a viral E3 ubiquitin ligase. Science 2005;309(5731):127‐130.
93. Wang X, Herr RA, Rabelink M, Hoeben RC, Wiertz EJ, Hansen TH. Ube2j2 ubiquitinates hydroxylated amino acids on ER‐associated degradation substrates. The Journal of cell biology 2009;187(5):655‐668. 94. Shimizu Y, Okuda‐Shimizu Y, Hendershot LM. Ubiquitylation of an ERAD substrate occurs on multiple types of amino acids. Mol Cell 2010;40(6):917‐926. 95. Ledford H. Drug bests cystic‐fibrosis mutation. Nature 2012;482(7384):145. 96. Kopito RR. Biosynthesis and degradation of CFTR. Physiol Rev 1999;79(1 Suppl):S167‐173. 97. Ward CL, Kopito RR. Intracellular turnover of cystic fibrosis transmembrane conductance regulator. Inefficient processing and rapid degradation of wild‐type and mutant proteins. J Biol Chem 1994;269(41):25710‐25718. 98. Ward CL, Omura S, Kopito RR. Degradation of CFTR by the ubiquitin‐proteasome pathway. Cell 1995;83(1):121‐127. 99. Jensen TJ, Loo MA, Pind S, Williams DB, Goldberg AL, Riordan JR. Multiple proteolytic systems, including the proteasome, contribute to CFTR processing. Cell 1995;83(1):129‐135. 100. Drumm ML, Wilkinson DJ, Smit LS, Worrell RT, Strong TV, Frizzell RA, Dawson DC, Collins FS. Chloride conductance expressed by delta F508 and other mutant CFTRs in Xenopus oocytes. Science 1991;254(5039):1797‐1799. 101. Okiyoneda T, Barriere H, Bagdany M, Rabeh WM, Du K, Hohfeld J, Young JC, Lukacs GL. Peripheral Protein Quality Control Removes Unfolded CFTR from the Plasma Membrane. Science 2010. 102. Silva MC, Fox S, Beam M, Thakkar H, Amaral MD, Morimoto RI. A genetic screening strategy identifies novel
regulators of the proteostasis network. PLoS Genet 2011;7(12):e1002438. 103. Hebert DN, Bernasconi R, Molinari M. ERAD substrates: which way out? Semin Cell Dev Biol 2010;21(5):526‐532. 104. Hampton RY, Sommer T. Finding the will and the way of ERAD substrate retrotranslocation. Curr Opin Cell Biol 2012;24(4):460‐466. 105. Smith MH, Ploegh HL, Weissman JS. Road to ruin: targeting proteins for degradation in the endoplasmic reticulum. Science 2011;334(6059):1086‐1090. 106. Schelhaas M, Malmstrom J, Pelkmans L, Haugstetter J, Ellgaard L, Grunewald K, Helenius A. Simian Virus 40 depends on ER protein folding and quality control factors for entry into host cells. Cell 2007;131(3):516‐529. 107. Slominska‐Wojewodzka M, Gregers TF, Walchli S, Sandvig K. EDEM is involved in retrotranslocation of ricin from the endoplasmic reticulum to the cytosol. Mol Biol Cell 2006;17(4):1664‐1675. 108. Sokolowska I, Walchli S, Wegrzyn G, Sandvig K, Slominska‐Wojewodzka M. A single point mutation in ricin A‐chain increases toxin degradation and inhibits EDEM1‐dependent ER retrotranslocation. Biochem J 2011;436(2):371‐385. 109. Redmann V, Oresic K, Tortorella LL, Cook JP, Lord M, Tortorella D. Dislocation of ricin toxin A chains in human cells utilizes selective cellular factors. The Journal of biological chemistry 2011;286(24):21231‐21238. 110. Bernardi KM, Forster ML, Lencer WI, Tsai B. Derlin‐1 facilitates the retro‐translocation of cholera toxin. Mol Biol Cell 2008;19(3):877‐884. 111. Dixit G, Mikoryak C, Hayslett T, Bhat A, Draper RK. Cholera toxin up‐regulates endoplasmic reticulum proteins that correlate with sensitivity
to the toxin. Exp Biol Med (Maywood) 2008;233(2):163‐175. 112. Lilley BN, Gilbert JM, Ploegh HL, Benjamin TL. Murine polyomavirus requires the endoplasmic reticulum protein Derlin‐2 to initiate infection. J Virol 2006;80(17):8739‐8744. 113. Li S, Spooner RA, Hampton RY, Lord JM, Roberts LM. Cytosolic entry of Shiga‐like toxin a chain from the yeast endoplasmic reticulum requires catalytically active Hrd1p. PLoS One 2012;7(7):e41119. 114. Bernardi KM, Williams JM, Kikkert M, van Voorden S, Wiertz EJ, Ye Y, Tsai B. The E3 ubiquitin ligases Hrd1 and gp78 bind to and promote cholera toxin retro‐translocation. Mol Biol Cell 2010;21(1):140‐151. 115. Kothe M, Ye Y, Wagner JS, De Luca HE, Kern E, Rapoport TA, Lencer WI. Role of p97 AAA‐ATPase in the retrotranslocation of the cholera toxin A1 chain, a non‐ubiquitinated substrate. The Journal of biological chemistry 2005;280(30):28127‐28132. 116. Wolf DH, Stolz A. The Cdc48 machine in endoplasmic reticulum associated protein degradation. Biochim Biophys Acta 2012;1823(1):117‐124. 117. Tirosh B, Furman MH, Tortorella D, Ploegh HL. Protein unfolding is not a prerequisite for endoplasmic reticulum‐to‐cytosol dislocation. J Biol Chem 2003;278(9):6664‐6672. 118. Fiebiger E, Story C, Ploegh HL, Tortorella D. Visualization of the ER‐to‐cytosol dislocation reaction of a type I membrane protein. Embo J 2002;21(5):1041‐1053. 119. Bhamidipati A, Denic V, Quan EM, Weissman JS. Exploration of the topological requirements of ERAD identifies Yos9p as a lectin sensor of misfolded glycoproteins in the ER lumen. Mol Cell 2005;19(6):741‐751. 120. Fagioli C, Mezghrani A, Sitia R. Reduction of interchain disulfide bonds precedes the dislocation of Ig‐mu chains
from the endoplasmic reticulum to the cytosol for proteasomal degradation. J Biol Chem 2001;276(44):40962‐40967. 121. Molinari M, Galli C, Piccaluga V, Pieren M, Paganetti P. Sequential assistance of molecular chaperones and transient formation of covalent complexes during protein degradation from the ER. J Cell Biol 2002;158(2):247‐257. 122. Majoul I, Ferrari D, Soling HD. Reduction of protein disulfide bonds in an oxidizing environment. The disulfide bridge of cholera toxin A‐subunit is reduced in the endoplasmic reticulum. FEBS Lett 1997;401(2‐3):104‐108. 123. Tsai B, Rodighiero C, Lencer WI, Rapoport TA. Protein disulfide isomerase acts as a redox‐dependent chaperone to unfold cholera toxin. Cell 2001;104(6):937‐948. 124. Spooner RA, Watson PD, Marsden CJ, Smith DC, Moore KA, Cook JP, Lord JM, Roberts LM. Protein disulphide‐isomerase reduces ricin to its A and B chains in the endoplasmic reticulum. Biochem J 2004;383(Pt 2):285‐293. 125. Forster ML, Sivick K, Park YN, Arvan P, Lencer WI, Tsai B. Protein disulfide isomerase‐like proteins play opposing roles during retrotranslocation. J Cell Biol 2006;173(6):853‐859. 126. Moore MS. Protein translocation: Nuclear export‐out of the dark. Current Biol 1996;6:137‐140. 127. Ushioda R, Hoseki J, Araki K, Jansen G, Thomas DY, Nagata K. ERdj5 is required as a disulfide reductase for degradation of misfolded proteins in the ER. Science 2008;321(5888):569‐572. 128. Hosoda A, Kimata Y, Tsuru A, Kohno K. JPDI, a novel endoplasmic reticulum‐resident protein containing both a BiP‐interacting J‐domain and thioredoxin‐like motifs. J Biol Chem 2003;278(4):2669‐2676.
129. Dong M, Bridges JP, Apsley K, Xu Y, Weaver TE. ERdj4 and ERdj5 are required for endoplasmic reticulum‐associated protein degradation of misfolded surfactant protein C. Mol Biol Cell 2008;19(6):2620‐2630. 130. Walczak CP, Tsai B. A PDI family network acts distinctly and coordinately with ERp29 to facilitate polyomavirus infection. J Virol 2011;85(5):2386‐2396. 131. Pasetto M, Barison E, Castagna M, Della Cristina P, Anselmi C, Colombatti M. Reductive activation of type 2 ribosome‐inactivating proteins is promoted by transmembrane thioredoxin‐related protein. The Journal of biological chemistry 2012;287(10):7367‐7373. 132. Riemer J, Hansen HG, Appenzeller‐Herzog C, Johansson L, Ellgaard L. Identification of the PDI‐family member ERp90 as an interaction partner of ERFAD. PLoS One 2011;6(2):e17037. 133. Moore P, Bernardi KM, Tsai B. The Ero1alpha‐PDI redox cycle regulates retro‐translocation of cholera toxin. Mol Biol Cell 2010;21(7):1305‐1313. 134. Bernasconi R, Soldà T, Galli C, Pertel T, Luban J, Molinari M. CyclosporineA‐sensitive, cyclophillinB‐dependent endoplasmic reticulum‐associated protein degradation. PLoS One 2010;5(9):e13008. 135. Greenblatt EJ, Olzmann JA, Kopito RR. Derlin‐1 is a rhomboid pseudoprotease required for the dislocation of mutant alpha‐1 antitrypsin from the endoplasmic reticulum. Nat Struct Mol Biol 2011;18(10):1147‐1152. 136. Zettl M, Adrain C, Strisovsky K, Lastun V, Freeman M. Rhomboid family pseudoproteases use the ER quality control machinery to regulate intercellular signaling. Cell 2011;145(1):79‐91.
137. Schubert U, Anton LC, Gibbs J, Norbury CC, Yewdell JW, Bennink JR. Rapid degradation of a large fraction of newly synthesized proteins by proteasomes. Nature 2000;404(6779):770‐774. 138. Vabulas RM, Hartl FU. Protein synthesis upon acute nutrient restriction relies on proteasome function. Science 2005;310(5756):1960‐1963. 139. Yewdell JW. DRiPs solidify: progress in understanding endogenous MHC class I antigen processing. Trends Immunol 2011;32(11):548‐558. 140. Gidalevitz T, Ben‐Zvi A, Ho KH, Brignull HR, Morimoto RI. Progressive disruption of cellular protein folding in models of polyglutamine diseases. Science 2006;311(5766):1471‐1474. 141. Gidalevitz T, Krupinski T, Garcia S, Morimoto RI. Destabilizing protein polymorphisms in the genetic background direct phenotypic expression of mutant SOD1 toxicity. PLoS Genet 2009;5(3):e1000399. 142. Tsai YC, Mendoza A, Mariano JM, Zhou M, Kostova Z, Chen B, Veenstra T, Hewitt SM, Helman LJ, Khanna C, Weissman AM. The ubiquitin ligase gp78 promotes sarcoma metastasis by targeting KAI1 for degradation. Nat Med 2007;13(12):1504‐1509. 143. Liang JS, Kim T, Fang S, Yamaguchi J, Weissman AM, Fisher EA, Ginsberg HN. Overexpression of the tumor autocrine motility factor receptor Gp78, a ubiquitin protein ligase, results in increased ubiquitinylation and decreased secretion of apolipoprotein B100 in HepG2 cells. J Biol Chem 2003;278(26):23984‐23988. 144. Chen X, Tukachinsky H, Huang CH, Jao C, Chu YR, Tang HY, Mueller B, Schulman S, Rapoport TA, Salic A. Processing and turnover of the Hedgehog protein in the endoplasmic reticulum. J Cell Biol 2011;192(5):825‐838.
145. Nunziante M, Ackermann K, Dietrich K, Wolf H, Gadtke L, Gilch S, Vorberg I, Groschup M, Schatzl HM. Proteasomal dysfunction and endoplasmic reticulum stress enhance trafficking of prion protein aggregates through the secretory pathway and increase accumulation of pathologic prion protein. The Journal of biological chemistry 2011;286(39):33942‐33953. 146. Yamasaki S, Yagishita N, Tsuchimochi K, Nishioka K, Nakajima T. Rheumatoid arthritis as a hyper‐endoplasmic‐reticulum‐associated degradation disease. Arthritis Res Ther 2005;7(5):181‐186. 147. Joshi B, Li L, Nabi IR. A role for KAI1 in promotion of cell proliferation and mammary gland hyperplasia by the gp78 ubiquitin ligase. The Journal of biological chemistry 2010;285(12):8830‐8839. 148. Wang F, Song W, Brancati G, Segatori L. Inhibition of ER‐associated degradation rescues native folding in loss of function protein misfolding diseases. The Journal of biological chemistry 2011;286(50):43454‐43464. 149. Bernasconi R, Galli C, Noack J, Bianchi S, de Haan CA, Reggiori F, Molinari M. Role of the SEL1L:LC3‐I Complex as an ERAD Tuning Receptor in the Mammalian ER. Mol Cell 2012;46(6):809‐819. 150. Kincaid MM, Cooper AA. ERADicate ER stress or die trying. Antioxid Redox Signal 2007;9(12):2373‐2387. 151. Pincus D, Walter P. A first line of defense against ER stress. The Journal of cell biology 2012;198(3):277‐279. 152. Cambridge SB, Gnad F, Nguyen C, Bermejo JL, Kruger M, Mann M. Systems‐wide proteomic analysis in mammalian cells reveals conserved, functional protein turnover. J Proteome Res 2011;10(12):5275‐5284. 153. Wu Y, Termine DJ, Swulius MT, Moremen KW, Sifers RN. Human
endoplasmic reticulum mannosidase I is subject to regulated proteolysis. J Biol Chem 2007;282(7):4841‐4849. 154. Termine DJ, Moremen KW, Sifers RN. The mammalian UPR boosts glycoprotein ERAD by suppressing the proteolytic downregulation of ER mannosidase I. J Cell Sci 2009;122(Pt 7):976‐984. 155. Le Fourn V, Gaplovska‐Kysela K, Guhl B, Santimaria R, Zuber C, Roth J. Basal autophagy is involved in the degradation of the ERAD component EDEM1. Cell Mol Life Sci 2009;66(8):1434‐1445. 156. Reggiori F, Monastyrska I, Verheije MH, Cali T, Ulasli M, Bianchi S, Bernasconi R, de Haan CA, Molinari M. Coronaviruses Hijack the LC3‐I‐positive EDEMosomes, ER‐derived vesicles exporting short‐lived ERAD regulators, for replication. Cell Host Microbe 2010;7(6):500‐508. 157. Gauss R, Kanehara K, Carvalho P, Ng DT, Aebi M. A complex of Pdi1p and the mannosidase Htm1p initiates clearance of unfolded glycoproteins from the endoplasmic reticulum. Mol Cell 2011;42(6):782‐793. 158. Hori O, Ichinoda F, Yamaguchi A, Tamatani T, Taniguchi M, Koyama Y, Katayama T, Tohyama M, Stern DM, Ozawa K, Kitao Y, Ogawa S. Role of Herp in the endoplasmic reticulum stress response. Genes Cells 2004;9(5):457‐469. 159. Miura H, Hashida K, Sudo H, Awa Y, Takarada‐Iemata M, Kokame K, Takahashi T, Matsumoto M, Kitao Y, Hori O. Deletion of Herp facilitates degradation of cytosolic proteins. Genes Cells 2010;15(8):843‐853. 160. Mueller B, Lilley BN, Ploegh HL. SEL1L, the homologue of yeast Hrd3p, is involved in protein dislocation from the mammalian ER. J Cell Biol 2006;175(2):261‐270. 161. Cattaneo M, Lotti LV, Martino S, Alessio M, Conti A, Bachi A, Mariani‐
Costantini R, Biunno I. Secretion of novel SEL1L endogenous variants is promoted by ER stress/UPR via endosomes and shed vesicles in human cancer cells. PLoS One 2011;6(2):e17206. 162. Xie Y, Avello M, Schirle M, Whinnie EM, Feng Y, Bric‐Furlong E, Wilson C, Nathans R, Zhang J, Kirschner MW, Huang SM, Cong F. Deubiquitinase FAM/USP9X interacts with the E3 ubiquitin ligase SMURF1 and protects it from ligase activity‐dependent self‐degradation. The Journal of biological chemistry 2012;288:2976‐2985. 163. Guo X, Shen S, Song S, He S, Cui Y, Xing G, Wang J, Yin Y, Fan L, He F, Zhang L. The E3 ligase Smurf1 regulates Wolfram syndrome protein stability at the endoplasmic reticulum. The Journal of biological chemistry 2011;286(20):18037‐18047. 164. Shmueli A, Tsai YC, Yang M, Braun MA, Weissman AM. Targeting of gp78 for ubiquitin‐mediated proteasomal degradation by Hrd1: cross‐talk between E3s in the endoplasmic reticulum. Biochem Biophys Res Commun 2009;390(3):758‐762. 165. Ballar P, Ors AU, Yang H, Fang S. Differential regulation of CFTRDeltaF508 degradation by ubiquitin ligases gp78 and Hrd1. Int J Biochem Cell Biol 2010;42(1):167‐173. 166. Tcherpakov M, Broday L, Delaunay A, Kadoya T, Khurana A, Erdjument‐Bromage H, Tempst P, Qiu XB, DeMartino GN, Ronai Z. JAMP optimizes ERAD to protect cells from unfolded proteins. Mol Biol Cell 2008;19(11):5019‐5028. 167. Ying Z, Wang H, Fan H, Zhu X, Zhou J, Fei E, Wang G. Gp78, an ER associated E3, promotes SOD1 and ataxin‐3 degradation. Hum Mol Genet 2009;18(22):4268‐4281. 168. Durcan TM, Kontogiannea M, Bedard N, Wing SS, Fon EA. Ataxin‐3
Deubiquitination Is Coupled to Parkin Ubiquitination via E2 Ubiquitin‐conjugating Enzyme. The Journal of biological chemistry 2012;287(1):531‐541. 169. Leitman J, Ron E, Ogen‐Shtern N, Lederkremer GZ. Compartmentalization of Endoplasmic Reticulum Quality Control and ER‐Associated Degradation Factors. DNA Cell Biol 2013;32(1):2‐7. 170. Olzmann JA, Kopito RR, Christianson JC. The Mammalian Endoplasmic Reticulum‐Associated Degradation System. Cold Spring Harb Perspect Biol 2012. 171. Kny M, Standera S, Hartmann‐Petersen R, Kloetzel PM, Seeger M. Herp regulates Hrd1‐mediated ubiquitylation in a ubiquitin‐like domain‐dependent manner. The Journal of biological chemistry 2011;286(7):5151‐5156. 172. Laney JD, Hochstrasser M. Analysis of protein ubiquitination. Curr Protoc Protein Sci 2002;Chapter 14:Unit 14 15. 173. Morito D, Hirao K, Oda Y, Hosokawa N, Tokunaga F, Cyr DM, Tanaka K, Iwai K, Nagata K. Gp78 cooperates with RMA1 in endoplasmic reticulum‐associated degradation of CFTRDeltaF508. Mol Biol Cell 2008;19(4):1328‐1336. 174. Jo Y, Lee PC, Sguigna PV, DeBose‐Boyd RA. Sterol‐induced degradation of HMG CoA reductase depends on interplay of two Insigs and two ubiquitin ligases, gp78 and Trc8. Proceedings of the National Academy of Sciences of the United States of America 2011;108(51):20503‐20508.
Figure Legends
Fig. 1 Role of ERAD in cellular proteostasis. A Nascent polypeptide chains are co-translationally translocated
into the ER. Most nascent chains attain the native structure (step 1) and are exported from the folding
compartment (step 2). A variable percentage of the newly synthesized polypeptides enter off pathways of the
folding programs (step 3) and is removed from the ER by constitutive ERAD (step 4). In healthy cells, folding
intermediates are protected from recognition by ERAD factors and have sufficient time to complete the folding
process. B Dysregulated ERAD as a consequence of elevated luminal levels of ERAD factors may cause
inappropriate disposal of intermediates of ongoing folding programs (step 5) thereby reducing production of
native polypeptides (steps 1 and 2).
Fig. 2 Substrate-specific ERAD pathways. The same misfolded module shows different requirements for
efficient clearance from the ER when anchored to (ERAD-LM substrate) and when detached from the membrane
(ERAD-LS substrate), the latter showing stronger dependency on ERAD lectins and HRD1 dislocons.
Consistently, OS-9 and XTP3-B are depicted in lighter colors for ERAD-LM substrates and red arrows show that
ERAD-LM substrates can diffuse in the lipid bilayer to enter HRD1 or alternative dislocation machineries.
Fig. 3 ERAD regulation by misfolded proteins. A In healthy cells, unused dislocation machineries are
disassembled. E3 ubiquitin ligases may for example poly-ubiquitylate themselves or components of the
supramolecular complexes thereby resulting in their degradation. Orphan components may also be segregated
from the ER lumen as shown by the vesicle-mediated release of SEL1L, EDEM1 and OS-9 (149). B Misfolded
proteins engage ERAD factors thereby preserving ERAD complexes, delaying ERAD factors turnover and
segregation from the ER.