RESEARCH ARTICLE
Host-Microbe Biology
Quantitative Proteome Analysis of Atg5-Deficient Mouse
Embryonic Fibroblasts Reveals the Range of the AutophagyModulated Basal Cellular Proteome
Kiran Bala Sharma,a Manish Sharma,a* Suruchi Aggarwal,a Amit Kumar Yadav,a Shinjini Bhatnagar,a Sudhanshu Vrati,a,b
Manjula Kaliaa,b
a
Translational Health Science and Technology Institute, NCR Biotech Science Cluster, Faridabad, Haryana, India
b
Regional Centre for Biotechnology, NCR Biotech Science Cluster, Faridabad, Haryana, India
Basal autophagy is crucial for maintenance of cellular homeostasis.
ATG5 is an essential protein for autophagosome formation, and its depletion has
been extensively used as a tool to disrupt autophagy. Here, we characterize the impact of Atg5 deficiency on the cellular proteome of mouse embryonic fibroblasts
(MEFs). Using a tandem mass tagging (TMT)-based quantitative proteomics analysis,
we observe that 14% of identified proteins show dysregulated levels in atg5⫺/⫺
MEFs. These proteins were distributed across diverse biological processes, such as
cell adhesion, development, differentiation, transport, metabolism, and immune responses. Several of the upregulated proteins were receptors involved in transforming growth factor  (TGF-) signaling, JAK-STAT signaling, junction adhesion, and
interferon/cytokine-receptor interactions and were validated as autophagy substrates. Nearly equal numbers of proteins, including several lysosomal proteins and
enzymes, were downregulated, suggesting a complex role of autophagy/ATG5 in
regulating their levels. The atg5⫺/⫺ MEFs had lower levels of key immune sensors
and effectors, including Toll-like receptor 2 (TLR2), interferon regulatory factor 3
(IRF3), IRF7, MLKL, and STAT1/3/5/6, which were restored by reexpression of ATG5.
While these cells could efficiently mount a type I interferon response to the doublestranded RNA (dsRNA) mimic poly(I·C), they were compromised in their inflammatory
response to the bacterial pathogen-associated molecular patterns (PAMPs) lipopolysaccharide (LPS) and Pam3CSK4. Transcriptional activation and secretion of
interleukin-6 (IL-6) in these cells could be recovered by ATG5 expression, supporting
the role of autophagy in the TLR2-induced inflammatory response. This study provides a key resource for understanding the effect of autophagy/ATG5 deficiency on
the fibroblast proteome.
ABSTRACT
Citation Sharma KB, Sharma M, Aggarwal S,
Yadav AK, Bhatnagar S, Vrati S, Kalia M. 2019.
Quantitative proteome analysis of Atg5deficient mouse embryonic fibroblasts reveals
the range of the autophagy-modulated basal
cellular proteome. mSystems 4:e00481-19.
https://doi.org/10.1128/mSystems.00481-19.
Editor Ileana M. Cristea, Princeton University
IMPORTANCE Autophagy performs housekeeping functions for cells and maintains a
functional mode by degrading damaged proteins and organelles and providing energy under starvation conditions. The process is tightly regulated by the evolutionarily conserved Atg genes, of which Atg5 is one such crucial mediator. Here, we have
done a comprehensive quantitative proteome analysis of mouse embryonic fibroblasts that lack a functional autophagy pathway (Atg5 knockout). We observe that
14% of the identified cellular proteome is remodeled, and several proteins distributed across diverse cellular processes with functions in signaling, cell adhesion, development, and immunity show either higher or lower levels under autophagydeficient conditions. These cells have lower levels of crucial immune proteins that
are required to mount a protective inflammatory response. This study will serve as a
valuable resource to determine the role of autophagy in modulating specific protein
levels in cells.
November/December 2019 Volume 4 Issue 6 e00481-19
Copyright © 2019 Sharma et al. This is an
open-access article distributed under the terms
of the Creative Commons Attribution 4.0
International license.
Address correspondence to Sudhanshu Vrati,
vrati@rcb.res.in, or Manjula Kalia,
manjula@rcb.res.in.
* Present address: Manish Sharma, Department
of Neuroscience, the Scripps Research Institute,
Jupiter, Florida, USA.
Autophagy deficit impact on the basal
fibroblast proteome
Received 7 August 2019
Accepted 8 October 2019
Published 5 November 2019
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Sharma et al.
KEYWORDS Atg5, IL-6, JAK-STAT, TLR2, TMT mass spectrometry, cell adhesion,
cytokine receptors, inflammation, innate immune response, interferon
M
acroautophagy (here autophagy) acts as a housekeeping module to keep the
cellular system clean by constitutively maintaining protein turnover and removing damaged organelles and aggregated proteins. During starvation, it turns into a
“lifeguard” to provide survival energy by degrading the nonessential components of
the cell. Autophagy targets a diverse range of substrates and hence is involved in the
regulation of several cellular pathways impacting development, metabolism, signal
transduction, aging, and immune function. Autophagy also plays critical roles under
diverse conditions such as pathogen infection, cancer, and neurodegeneration (1–3).
Autophagosome biogenesis is executed by the action of the evolutionarily conserved ATG genes (4). In response to signals such as mTOR inhibition, phagophore
formation is initiated by the ULK1-ATG3-FIP200 complex and the class III phosphatidylinositol 3-kinase (PI3-K)-Beclin1 complex (5, 6). Elongation of the phagophore involves two ubiquitin-like (UBL) conjugation systems. A series of enzymatic events leads
to the activation and formation of the ATG12-ATG5-ATG16L1 molecular complex that
binds to the phagophore and completes the loading of phosphatidylethanolamine (PE)
conjugated to microtubule-associated protein 1 light chain 3 (LC3) on the inner and
outer membranes of the autophagosome (7, 8). Given its central and crucial role in
autophagosome formation, ATG5 depletion has been widely used as a powerful tool to
understand autophagy and processes regulated by it, at both the cellular and organism
levels (9–21).
In recent years, several technical advances in mass spectrometry have enabled an
enhanced capacity for proteomic discovery (22). High-throughput quantitative proteomics is a highly sensitive approach to analyze global protein dynamics within a cell
(23). By directly focusing on the biological effector molecules, it provides several
advantages over mRNA expression analysis. Here, we present a tandem mass tagging
(TMT)-based mass spectrometry analysis of wild-type (WT) and atg5⫺/⫺ mouse embryonic fibroblasts (MEFs) and analyze the role of autophagy/ATG5 in remodeling the
cellular fibroblast proteome under basal conditions. We observe that 14% of the cellular
proteome is dysregulated due to ATG5 deficiency, and proteins implicated in diverse
biological functions, such as development, cell adhesion, signal transduction, metabolism, and immune and inflammatory processes, are impacted. Several of the upregulated proteins were receptors, indicating an important role of basal autophagy in the
constitutive turnover of receptors. Multilayered cellular regulation through ATG5 could
also be seen, as equal numbers of proteins were downregulated in these cells. Several
of the downregulated proteins were critical modulators of immune and inflammatory
responses. The atg5⫺/⫺ MEFs expressed low levels of Toll-like receptor 2 (TLR2) and
were inefficient in mounting a response to the bacterial pathogen-associated molecular
patterns (PAMPs) lipopolysaccharide (LPS) and Pam3CSK4, and this effect was reversed
by reexpression of ATG5. This study will serve as a useful proteomic resource for the
impact of autophagy deficiency in fibroblasts.
RESULTS
TMT-based mass spectrometry of WT and atg5ⴚ/ⴚ MEFs. To study the impact of
basal autophagy on the cellular proteome, we analyzed results of a TMT-based mass
spectrometry quantitative proteomics study for biological replicates of WT and atg5⫺/⫺
MEFs (see Fig. S1 in the supplemental material). A total of 8,745 proteins were
quantified from each sample (1% false discovery rate [FDR]). Proteins having fewer than
2 unique peptides were excluded, and the resulting 7,795 proteins were used for
further analysis. A hierarchical cluster heat map shows changes in relative protein
abundances across the WT and ATG5-deficient conditions (Fig. 1A). A comparison of the
replicates showed good correlation between the sample duplicates of WT and atg5⫺/⫺
cells (Fig. 1B). Replicates were combined based on their normalized percent relative
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FIG 1 TMT-based mass spectrometry analysis of WT and atg5⫺/⫺ MEFs. (A) Hierarchical cluster heat map showing the levels of 7,795 (ⱖ2 unique peptides and
⬍1% FDR) quantified proteins across the WT and atg5⫺/⫺ MEFs. The normalized raw intensities were used for creating the heat map using the Gene-E tool.
(B) Scatterplot displaying the relative protein abundances of 7,795 proteins in the sample duplicates of WT and atg5⫺/⫺ MEFs. Pearson’s correlation is indicative
of the reproducibility of the biological replicates. (C) Fold change (atg5⫺/⫺/WT) intensities of the 7,795 quantified proteins. The pie chart displays the numbers
of unchanged, upregulated (ⱖ1.5-fold), and downregulated (ⱕ1.5-fold) proteins. (D) Gene ontology (GO) enrichment analysis of upregulated and downregulated proteins in atg5⫺/⫺ MEFs was performed using GeneCodis to study biological processes (BP). (E and F) Bar graphs showing the normalized relative protein
abundances of several ATG proteins and autophagy substrates (E) and of different proteins involved in lysosomal organization and pH regulation (F) in atg5⫺/⫺
MEFs.
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FIG 2 GO enrichment analysis of up- and downregulated proteins found in atg5⫺/⫺ MEFs was performed using GeneCodis to identify molecular functions (MF)
(A) and cellular components (CC) (B).
abundances, and the protein intensity fold change (FC) between the two cell types was
calculated. We found that the absence of ATG5 affected ⬃14% (1,087 of 7,795) of the
identified proteome, with 538 (6.9%) proteins upregulated (ⱖ1.5-fold) and 549 (7.04%)
proteins downregulated (ⱕ1.5-fold) in atg5⫺/⫺ MEFs (Fig. 1C and Data Set S1).
Pathway enrichment analysis was performed to segregate the dysregulated proteins
based on biological processes, cellular components, and molecular functions (Fig. 1D,
Fig. 2, and Data Set S2). We observed that several proteins implicated in cell adhesion,
proteolysis, transport, metabolic processes, signal transduction, and immune and inflammatory responses were dysregulated in atg5⫺/⫺ MEFs (Fig. 1D and Data Set S2).
The proteins affected by autophagy modulation had diverse molecular functions, such
as protein, lipid, metal ion, nucleotide, ATP binding, hydrolase, transferase, kinase, and
peptidase activities, etc., and different subcellular localizations (Fig. 2 and Data Set S2).
The levels of ATG5, ATG12, and ATG16L1 were reduced by over 90% in atg5⫺/⫺
MEFs. Other autophagy proteins, ATG3, ATG7, GABARAP, and OPTN, displayed 20 to
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40% reductions in levels, while the levels of ATG2A, ATG4A, ATG4B, ATG13, and ATG14
were found to be unchanged (Fig. 1E). Consistent with the literature, we also observed
the accumulation of autophagy substrates such as SQSTM1, NBR1, and BNIP3 in
atg5⫺/⫺ MEFs (Fig. 1E). These cells also had lower levels of lysosomal proteins, enzymes,
and vacuolar ATPases, indicative of a reduced lysosomal compartment in these cells
(Fig. 1F, Fig. 2B, Fig. S2, and Fig. S3B).
Several proteins implicated in cell differentiation, transport, signal transduction,
cytoskeleton reorganization, endocytosis, apoptosis, and innate immune responses
were selectively upregulated in atg5⫺/⫺ MEFs (Fig. 1D). Molecular function and cellular
compartment analyses showed that many of these proteins were receptors with an
extracellular localization but diverse functions, such as the transforming growth factor
 (TGF-) receptor family; platelet-derived growth factor binding; collagen, ubiquitin,
and heparin binding; and the low-density lipoprotein (LDL) receptor (LDLR) and LDL
receptor-related protein families (Fig. S2A and B). Since all the proteins that have higher
levels in atg5⫺/⫺ MEFs are likely to be autophagy substrates, these were checked for
potential LC3-interacting region (LIR) motifs, and the position-specific scoring matrix
(PSSM) score was calculated (24). A total of 339 (63%) upregulated proteins had a PSSM
score of ⬎13, suggesting that these are potential autophagy substrates (Fig. S2 and
Data Set S3).
In the atg5⫺/⫺ MEFs, several crucial transporters were also found to be dysregulated
(Fig. S3A and B). Of these, proteins that function in membrane trafficking (LDLR, STX6,
RAB39b, KDELR3, SYT11, and SNX17), the solute carrier (SLC) superfamily, the ABC
transporter superfamily, and lipid transporters were selectively upregulated (Fig. S3A
and B and Data Set S4), while other proteins, such as vacuolar ATPases, were downregulated (Fig. S3B and Data Set S4). In accordance with the role of autophagy in
regulating cellular homeostasis, proteins implicated in multiple metabolic pathways
(lipid, carbohydrate, sphingolipid, glutathione, ceramide, and amino sugar, etc.) were
dysregulated (Fig. S3C and D and Data Set S4).
Autophagy is a critical regulator of proteins involved in development. Sonic
Hedgehog, TGF-, fibroblast growth factor (FGF), Notch, and Wnt signaling proteins are
crucial for early patterning and organization in embryonic development and also
control cell proliferation and differentiation throughout life (25). The literature has
demonstrated the importance of autophagy in embryogenesis and development, as
deletion of autophagy genes in mice leads to lethality (embryonic and neonatal stages)
and defects in neuronal differentiation (26, 27). Several studies have shown the
interplay between autophagy/autophagy-related genes (ATGs) and developmental
pathways (Wnt, Notch, Shh, FGF, and TGF-) in different cell models (28–33). Autophagy balances the levels of various development-related signaling proteins. It is well
known to antagonize Wnt signaling by degrading disheveled protein in autolysosomes
in normal rat kidney epithelial cells and MEFs (28, 30) and by eliminating cytoplasmic
beta-catenin (31, 34), Notch signaling by degrading Notch receptor and controlling
neurogenesis and stem cell growth (33), and TGF- signaling by degrading TGF- (29)
and TGF- receptor 1 (TGF-R1) (35).
In accordance with published data, atg5⫺/⫺ MEFs showed enhanced levels of key
players involved in development and differentiation pathways such as TGF-, Wnt,
Hedgehog, and Notch (Fig. 3A and B and Data Set S4). We validated the higher
expression levels of some of the key molecules of the TGF- signaling pathway in
atg5⫺/⫺ MEFs by Western blotting. Significantly higher levels of TGF-R1, TGF-R2,
ACVR1A, ACVR2A (activin A receptors of the bone morphogenetic protein [BMP]
pathway), and SMAD6 were observed (Fig. 3C and D). SMAD6 is an inhibitory SMAD that
binds and inactivates phosphorylated receptor SMADs, preventing nuclear translocation and transcription of genes that promote osteoblast differentiation (36). SMAD6
also inhibits BMP signaling by complexing with the ubiquitin ligase SMURF1, leading to
the proteasomal degradation of BMP receptors and receptor SMADs (37).
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FIG 3 Autophagy is a critical regulator of proteins involved in development. (A) KEGG pathway analysis of the upregulated development-related proteins in
atg5⫺/⫺ MEFs was performed using GeneCodis. (B) A functional protein association network was generated using STRING 11.0. The line thickness indicates the
strength of data support. (C) WT and atg5⫺/⫺ MEFs were treated with the vehicle control (dimethyl sulfoxide [DMSO]) or 100 nM bafilomycin A1 (Baf A1) for
3 h. Protein lysates were analyzed by Western blotting with TGF-R1, TGF-R2, ACVR1A, ACVR2A, SMAD6, LC3, and actin (loading control) antibodies. (D) Bar
graph showing normalized protein levels in KO MEFs (atg5⫺/⫺/WT), Baf A1-treated WT MEFs [WT (Baf)/WT], and Baf A1-treated KO MEFs [atg5⫺/⫺(Baf)/atg5⫺/⫺].
An increase in the protein level upon Baf A1 treatment as seen for LC3-II is indicative of protein degradation through autophagy. Densitometry analysis of the
protein bands was performed using ImageJ software. Data are presented as means ⫾ SD of values obtained from 3 independent experiments. Student’s t test
was used to calculate P values (*, P ⬍ 0.05; **, P ⬍ 0.01; NS, not significant).
To distinguish the protein accumulations caused by ATG5 deficiency versus a block
in autophagosome degradation, we used the vacuolar ATPase inhibitor bafilomycin A1
(Baf A1), which inhibits vesicle acidification and thus prevents autophagosome maturation into autolysosomes and subsequent degradation of cargo. As expected, treatment of WT MEFs with Baf A1 increased levels of LC3-II significantly (Fig. 3C and D). A
similar increase in protein levels of TGF-R1, ACVR1A, and ACVR2A was observed in WT
MEFs upon Baf A1 treatment, validating that autophagy is involved in the turnover of
these receptors in the cell (Fig. 3C and D). The relative mRNA levels of a subset of TGF-
signaling pathway genes (Tgfr1, Tgfr2, Tgfr3, Acvr1a, Acvr2a, Smad6, and Bmpr2)
were also evaluated (Fig. S4A). While levels of some transcripts were unchanged,
significantly lower levels of Tgfr1 and higher levels of Tgfr2 and Tgfr3 were
observed in atg5⫺/⫺ MEFs. This was not unexpected since protein levels are influenced
by multiple factors and do not always correlate with mRNA levels. Collectively, our data
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confirm the involvement of autophagy in regulating the expression of key TGF-
receptor signaling components.
Autophagy regulates levels of several cell adhesion proteins. Cell adhesion
emerged as a major biological process whose proteins were dysregulated in atg5⫺/⫺
MEFs (Fig. 4A and B and Data Set S4). Several studies have documented an essential
role of autophagy in establishing tight junction permeability, cell adhesion, cell motility,
and tumor metastasis (38, 39). The turnover of cadherin (40, 41), Claudin2 (42),
internalized collagen and focal adhesion (FA) proteins (43, 44), VCAM1 in endothelial
cells (45), cytokine-induced ICAM1 levels in lung epithelial cells (46), and the actin
cytoskeleton and adherens junctions in human induced pluripotent stem cells (47) are
known to be regulated by autophagy.
In our data, we found that the absence of autophagy/ATG5 altered the expression
levels of numerous cell adhesion molecules that are essential for focal adhesion,
adherens junctions, tight junctions, extracellular matrix-receptor interactions, and leukocyte transendothelial migration in the cells (Fig. 4A and B). Levels of adhesion
proteins, including members of the immunoglobulin superfamily (JAM1, JAM3, VCAM1,
and NCAM1), cadherins (CDH3, PCDHB22, PCDH19, PCDH18, and PCDH16), integrins
(ITGA5 and ITGA11), syndecans (SDC2 and SDC4), laminins (LAMA4 and LAMB1), and
collagens (COL6a1, COL5a1, COL12a1, and COL18a1), were found to be increased,
whereas levels of proteins such as CDH13, LAMA5, ICAM1, integrins (ITGAV, ITGA2,
ITGA1, ITGB5, and ITGA7), and collagens (COL8a1 and COL11a1) were found to be
decreased in ATG5-deficient MEFs (Fig. 4C and Data Set S4).
We validated the expression levels of some of these proteins by Western blotting
and observed significantly higher levels of JAM1, JAM3, P-cadherin, E-cadherin, and
SDC2 in autophagy-defective cells than in WT cells (Fig. 4D and E). WT and atg5⫺/⫺
MEFs were also treated with Baf A1, and cell lysates were further analyzed by Western
blotting. In WT MEFs, Baf A1 treatment led to a rapid accumulation of LC3-II, indicating
that autophagosomes are not being turned over by lysosomal proteolysis, whereas, as
expected, atg5⫺/⫺ MEFs did not show LC3-II (Fig. 3C and D). WT MEFs showed an
enhancement of JAM1, E-cadherin, and SDC2 levels in Baf A1-treated samples, while the
intensity of JAM3 and P-cadherin remain unchanged (Fig. 4D and E). Several of these
proteins were also transcriptionally upregulated in atg5⫺/⫺ MEFs (Fig. S4B). Our data
thus indicate that ATG5/autophagy plays a major role in modulating levels of proteins
involved in cell adhesion, motility, and cell communication.
Absence of ATG5 alters levels of several immune effectors. Our proteome
analysis showed differential expression patterns for various immune-related proteins,
suggesting that autophagy/ATG5 may be crucial in regulating interferon (IFN) and
inflammatory and adaptive immune responses. We observed elevated levels of several
cytokine receptors, interferon receptors, tumor necrosis factor (TNF) receptors, TGF
receptors, and complement system proteins in atg5⫺/⫺ MEFs (Fig. 5A to C and Data Set
S4). Studies have shown that the IFNAR1 and IFNGR1 receptors undergo ubiquitindependent lysosomal degradation (48–50). Similarly, plasma membrane levels of TNFR1
and LIFR are maintained via endocytosis and degradation in lysosomes (51, 52). The
complement protein C3 directly interacts with ATG16L1 and is involved in autophagydependent bacterial growth restriction and recycling in diabetogenic stress (53, 54).
Several of these proteins also have LIR motifs (Fig. S2 and Data Set S3), suggesting that
autophagy might be engaged in maintaining the basal turnover of these immune
signaling receptors by degradation in lysosomes. Furthermore, atg5⫺/⫺ MEFs also have
higher protein levels of JAK1, a protein noncovalently associated with the cytoplasmic
tail of several cytokine receptors, including IFNAR and IFNGR (55).
On the other hand, many proteins known to play a fundamental role in pathogen
recognition (TLR2, TLR3, and ZBP1) and the activation of innate (OAS1, OAS2, IFIT1,
IFIT2, TRIM25, ISG20, and the GBP family) and adaptive (HLA-A, TAP1, TAP2, TAPBP,
PSMB8, and PSMB9) immunity were suppressed in autophagy-deficient cells (Fig. 5B
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FIG 4 ATG5 deficiency dysregulates several cell adhesion proteins. (A and B) KEGG analysis of cell adhesion proteins found to be up- and downregulated upon
autophagy deficiency. (C) Bar graph showing the differential expression of integrin and collagen proteins due to autophagy deficiency. (D) WT and atg5⫺/⫺ MEFs
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and C and Data Set S4). This is indicative of a strong link between basal autophagy/
ATG5 and levels of immune proteins in resting cells.
Using Western blotting, we validated the expression levels of some crucial innate
immune-related and STAT family proteins in atg5⫺/⫺ MEFs (Fig. 6). Significant reductions in the levels of TLR2, interferon regulatory factor 3 (IRF3), IRF7, MLKL, STAT1,
STAT3, STAT5, and STAT6 was observed in these cells (Fig. 6A and B). The transcriptional
levels of these genes in both cell lines showed significant downregulation of Irf7, Mlkl,
Stat1, and Stat5 in atg5⫺/⫺ MEFs (Fig. 6C). We further treated WT and atg5⫺/⫺ MEFs
with Baf A1 to distinguish innate immune effector suppression caused by autophagy
degradation impairment versus ATG5 absence. No change in TLR2, MLKL, and STAT1
levels upon Baf A1 treatment in WT MEFs was observed. However, levels of the primary
innate immune effector IRF3 showed an increase, implying that its basal levels are
maintained through autophagy (Fig. 6C and D). To validate that the lower protein levels
of these key immune sensors and adaptors was a direct effect of ATG5 deficiency, we
overexpressed ATG5 in the atg5⫺/⫺ MEFs (Fig. 6E and F). Expression of ATG5 and
conversion of LC3-I to LC3-II were seen in these cells, confirming restoration of
autophagy function. The levels of all the key immune-related proteins were restored to
nearly wild-type levels in these cells, confirming that their amounts in resting cells are
maintained through ATG5/autophagy.
Effect of ATG5 deficiency on immune responses to viral and bacterial PAMPs.
We next assessed the activation of immune effectors in both WT and atg5⫺/⫺ MEFs in
response to stimulation with poly(I·C) (synthetic double-stranded RNA [dsRNA] virus
analog). Recognition of dsRNA activates IRF3-dependent expression of antiviral factors.
By 6 h posttreatment, poly(I·C) significantly upregulated the levels of IRF3, IRF7, STAT1,
STAT2, and MLKL in both cell types (Fig. 7A and B). Despite similar activation, the
protein levels of these effectors were still lower under autophagy-deficient conditions
than for the control (Fig. 6A and B). Since atg5⫺/⫺MEFs have lower STAT1 levels, the
level of STAT1 phosphorylation in these cells was also lower (Fig. 7A). However,
significant transcriptional activation of all these genes and IFN was observed in these
cells, with Irf7 and IFN showing severalfold-higher levels of upregulation in atg5⫺/
⫺MEFs than in WT MEFs (Fig. 7C). In accordance with higher RNA levels, the level of
secretion of IFN- in these cells was also higher (Fig. 7D). Enhanced IFN and cytokine
production in atg5⫺/⫺ MEFs in response to vesicular stomatitis virus (VSV) infection and
poly(I·C) has been reported in previous studies, based on association of the ATG5ATG12 complex with RIG-1, MDA-5, and IPS-1 (56), and by enhanced reactive oxygen
species (ROS) production mediated by dysfunctional mitochondria (57). Another recent
study demonstrated that in response to influenza A virus infection, ATG5-deficient cells
had higher IFN- expression levels than autophagy-competent cells (17).
We further checked for the capacity of the atg5⫺/⫺ MEFs to mount an immune
response against the common bacterial PAMP LPS. A 24-h treatment with LPS resulted
in significant increases in levels of TLR2 and IRF3 in both cell types (Fig. 8A and B). A
comparison of the transcriptional levels of Tlr2 and Il-6 revealed that the atg5⫺/⫺ MEFs
were suppressed for activation at early times (3 and 6 h) after LPS treatment (Fig. 8C).
To check if the transcriptional activation and secretion of the major proinflammatory
cytokine interleukin-6 (IL-6) were dependent on ATG5, we expressed ATG5 in
autophagy-deficient cells. After 3 h of LPS treatment, we observed significant recovery
of Il-6 mRNA levels and IL-6 secretion in ATG5-rescued cells (Fig. 8D and E).
A striking feature of atg5⫺/⫺ MEFs was lower levels of TLR2, a member of the
Toll-like receptor signaling family. TLR2 forms heterodimeric complexes with either
FIG 4 Legend (Continued)
were treated with DMSO (control) and 100 nM Baf A1 for 3 h, and protein extracts were analyzed by Western blotting with JAMA, JAMC, P-cadherin, E-cadherin,
syndecan 2, and actin (loading control) antibodies. (E) Bar graph showing the normalized protein levels in KO MEFs (atg5⫺/⫺/WT), Baf A1-treated WT MEFs [WT
(Baf)/WT], and Baf A1-treated KO MEFs [atg5⫺/⫺(Baf)/atg5⫺/⫺]. An increase in the protein level upon Baf A1 treatment is indicative of protein degradation
through autophagy. Densitometry analysis was performed using ImageJ software. Presented are means ⫾ standard deviations of values obtained from 3
independent experiments. Student’s t test was used to calculate P values (*, P ⬍ 0.05; **, P ⬍ 0.01; ***, P ⬍ 0.001).
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FIG 5 ATG5-deficient MEFs show dysregulation of several immune-related proteins. (A and B) KEGG analysis of immune-related proteins found to be upand downregulated due to autophagy deficiency. (C) Radar plot representing the expression values of the listed immune proteins in WT and atg5⫺/⫺ MEFs.
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FIG 6 ATG5-deficient MEFs have lower levels of immune signaling proteins and STATs, which can be rescued by ATG5 reexpression. (A and B)
Western blots and bar graphs showing levels of TLR2, DHX58, IRF3, IRF7, MLKL, STAT1, STAT2, STAT3, STAT5, STAT6, and actin (loading control) in
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FIG 7 ATG5-deficient MEFs show an enhanced type I interferon response to the dsRNA mimic poly(I·C). WT and atg5⫺/⫺ MEFs were transfected
with 1 g/ml poly(I·C) for 6 h or mock transfected. (A) Western blot showing the levels of DHX58, IRF3, IRF7, STAT1, pSTAT1, STAT2, MLKL, and
actin (loading control). (B) Bar graph showing normalized protein expression [poly(I·C)/control] of the indicated proteins in WT and atg5⫺/⫺ MEFs.
Densitometry analysis was performed using ImageJ software. (C) mRNA levels of various immune effector genes, including Dhx58, Irf3, Irf7, Stat1,
Stat2, Mlkl, and Ifn, were quantitated by qRT-PCR. (D) The supernatant collected from treated cells was used to perform an ELISA for IFN-. For
panels B to D, data presented are means ⫾ standard deviations of values obtained from 3 independent experiments. Student’s t test was used
to calculate P values (*, P ⬍ 0.05; **, P ⬍ 0.01; ***, P ⬍ 0.001).
TLR1 or TLR6 and binds to diacylated and triacylated lipopeptides (58). The TLR2/1
heterodimer recognizes the triacylated lipopeptide Pam3CSK4 (59). We further characterized the effect of ATG5/autophagy on TLR2 and its downstream signaling by using
its specific agonist Pam3CSK4 (Fig. 9). Samples prepared from mock- and Pam3CSK4treated WT and atg5⫺/⫺ MEFs were treated with brefeldin A to block protein secretion
and analyzed by Western blotting (Fig. 9A). We observed that the absence of autophagy reduced IL-1 synthesis and secretion and Il-6 activation in response to TLR2
activation (Fig. 9A and C). We further checked if restoration of ATG5 expression in the
FIG 6 Legend (Continued)
WT and atg5⫺/⫺ MEFs. (C and D) WT and atg5⫺/⫺ MEFs were treated with DMSO (control) or 100 nM Baf A1 for 3 h, and protein extracts were
analyzed by Western blotting. The Western blots and bar graphs show the levels of the indicated proteins. (E and F) ATG5 expression in atg5⫺/⫺
MEFs was performed by transfection with a vector backbone or pCI-neo-mApg5. For panels B and D, data in bar graphs showing normalized protein
levels (atg5⫺/⫺/WT [B] and Baf A1/mock [D]) are presented as means ⫾ SD of values obtained from 3 independent experiments. (F) Bar graphs
showing normalized protein levels (atg5⫺/⫺/WT and ATG5 rescue/WT) presented as mean values obtained from 2 independent experiments.
Densitometry analysis was done using ImageJ software. Student’s t test was used to calculate P values (*, P ⬍ 0.05; **, P ⬍ 0.01; ***, P ⬍ 0.001).
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FIG 8 ATG5-deficient MEFs show reduced immune responses to the bacterial PAMP LPS. WT and atg5⫺/⫺ MEFs were treated with 100 ng/ml LPS.
(A) Western blot showing the levels of TLR2, IRF3, IRF7, STAT1, STAT2, MLKL, and actin (loading control) 24 h after LPS treatment. (B) Bar graph
showing normalized protein expression (LPS/control) of the indicated proteins in WT and atg5⫺/⫺ MEFs. Densitometry analysis was performed
using ImageJ software. (C) Normalized mRNA levels of Tlr2 and Il-6 3, 6, and 24 h after LPS treatment. (D and E) LPS treatment was given for 3 h
to WT MEFs (vector transfected), atg5⫺/⫺ MEFs (vector transfected), and atg5⫺/⫺ MEFs (pCI-neo-mApg5 transfected). Transcript levels of Il-6 (D)
and secreted IL-6 in the culture supernatant (E) were estimated. Data presented are means ⫾ standard deviations of values obtained from 3
independent experiments. Student’s t test (B and C) or ANOVA followed by Dunnett’s post hoc comparison test (D and E) was used to calculate
P values (*, P ⬍ 0.05; **, P ⬍ 0.01; ***, P ⬍ 0.001; ****, P ⬍ 0.0001).
knockout (KO) MEFs would have any effect on Pam3CSK4-induced signaling through
TLR2 (Fig. 9B, D, and E). The protein levels of TLR2 (Fig. 9B), Il-6 activation (Fig. 9D), and
IL-6 secretion (Fig. 9E) were recovered by ATG5 expression in the autophagy-deficient
cells. Collectively, out data indicate a crucial role of functional autophagy/ATG5 for
activation of TLR2 signaling and IL-6 production.
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Sharma et al.
FIG 9 ATG5-deficient MEFs show reduced responses to the TLR2 agonist Pam3CSK4, which is rescued by ATG5 reexpression. (A) WT and atg5⫺/⫺ MEFs were
treated with 100 ng/ml Pam3CSK4 for 6 h. A total of 1 g/ml brefeldin A (BFA) was added 4 h before harvest to block protein secretion. Western blots show
the levels of TLR2, IL-1, and actin (loading control). (B) WT and atg5⫺/⫺ MEFs were transfected with an empty vector or pCI-neo-mApg5 and treated with
Pam3CSK4 for 3 h. Cell lysates were blotted for TLR2, ATG5, LC3, and actin (loading control). (C) Transcript levels of Tlr2 and Il-6 3, 6, and 24 h after Pam3CSK4
treatment. (D and E) Pam3CSK4 treatment was given for 3 h to WT MEFs (vector transfected), atg5⫺/⫺ MEFs (vector transfected), and atg5⫺/⫺ MEFs
(pCI-neo-mApg5 transfected). Transcript levels of Il-6 (D) and secreted IL-6 in the culture supernatant (E) were estimated. Data presented are means ⫾ standard
deviations of values obtained from 3 independent experiments. Student’s t test (B and C) or ANOVA followed by Dunnett’s post hoc comparison test (D and
E) was used to calculate P values (*, P ⬍ 0.05; **, P ⬍ 0.01; ***, P ⬍ 0.001).
DISCUSSION
This study serves as a resource for understanding the impact of autophagy deficiency on the basal fibroblast proteome. Our data show that autophagy modulates
nearly 14% of the cellular proteome, indicating its role in a plethora of cellular functions
and in maintaining intracellular homeostasis.
While autophagy plays a critical role under stress conditions, such as starvation and
pathogen infection, basal autophagy is also essential for constitutive turnover of
cellular contents. The role of autophagy in protein turnover was recently quantified in
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Autophagy-Deficient Basal Fibroblast Proteome
a study by comparing protein half-lives in autophagy-deficient primary human fibroblasts, using time-resolved isotopic labeling and mass spectrometry. This study showed
that the proteasome and the CCT/TriC chaperonin are autophagy substrates and are
stabilized under autophagy-deficient conditions (60). This highlighted how autophagy
can impact protein degradation through the ubiquitin proteasomal pathway. A subsequent study by the same group showed enhanced degradation of long-lived proteins
in quiescent fibroblasts via upregulation of autophagy (61). Autophagy has also been
shown to be a critical player in the balance between senescence and apoptosis (62).
Studies in Arabidopsis have shown that atg5 mutants accumulate proteins but also have
higher activities of the proteasome and papain-like cysteine protease, which could
contribute to enhanced cell death (63). These studies have given mechanistic insights
into how autophagy modulates basal protein levels in different experimental systems.
Our study with MEFs demonstrates that autophagy regulates proteins of diverse
biological processes, ranging from development, metabolism, cell adhesion, and transport to innate and adaptive immunity. Changes in the basal levels of these proteins can
potentially rewire entire cellular pathways and influence biological outcomes. Significantly, the lysosomal compartment was impacted by ATG5 loss, as seen by reduced
levels of several lysosomal proteins (LAMP1 and LAMP2), enzymes, and vacuolar
ATPases. Several upregulated proteins in the autophagy-deficient cells were receptors
with an extensive range of functions (TGF- signaling, JAK-STAT signaling, and cytokine
and interferon receptors). Several of these receptors signal at the plasma membrane by
binding to their ligands and are internalized into endosomes for recycling or are
degraded by targeting to the late endosome/lysosome. Higher levels of these receptors
are indicative of the role of autophagy in their turnover and the potential to impact the
strength of the signal emanating from them. Some of these receptors are known to be
modulated by autophagy, while others (ACVR1A, AVCR2A, JAMA, JAMC, and SDC2)
have been described for the first time in this study. We have analyzed all the upregulated proteins for potential LIR motifs (24) and observed that 63% of these were
potential autophagy substrates. A recent study described a new class of ATG8interacting proteins that utilize a ubiquitin-interacting motif-like sequence for highaffinity binding (64).
Immune-related proteins formed a major subgroup that was dysregulated upon
ATG5 deficiency. While several cytokine and interferon receptors were upregulated in
these cells, key immune sensors (TLR2) and effectors (IRF3, IRF7, MLKL, and STAT1/3/
5/6) had lower levels. Their expression in the KO MEFs was restored by the expression
of ATG5, validating the essential role of ATG5/autophagy in modulating their levels in
resting cells.
We observed that protein levels of IRF3 were low, while its transcript level was
upregulated in atg5⫺/⫺ MEFs. However, Baf A1 treatment of WT MEFs confirmed that
basal levels of IRF3 were directly modulated by autophagy. This suggests that in
ATG5-deficient cells, either IRF3 stabilization factors are lacking or there is enhanced
proteasomal degradation of IRF3. The E3 ubiquitin ligase c-Cbl has been shown to be
a negative regulator of IRF3 stability, promoting its polyubiquitination and proteasomal
degradation (65). Studies have also shown that IRF3 is constitutively associated with
IFITM3, which regulates IRF3 homeostasis by mediating its autophagic degradation
(66).
Several studies have dissected the role of autophagy in the context of diverse
infections in different cell types. Autophagy has been shown to modulate different
steps of immune signaling during bacterial and viral infections (1). It can either enhance
the immune response by facilitating PAMP recognition by TLRs present on autophagosomes or suppress signaling by degrading various immune-related proteins in
autolysosomes (67–69). Autophagy is involved in limiting the type I IFN response by (i)
clearing the RIG-I pathway proteins in autophagy-deficient Ras-driven cancer cells
(70), (ii) degrading NF-B signaling components (71) and IRF3 by TRIM21-mediated
selective degradation, and (iii) interfering with RLR-IPS1 interaction-driven downstream signaling.
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Sharma et al.
Our study demonstrates dysregulation of critical immune receptors, signaling proteins, and effectors under ATG5 deficiency. The role of autophagy in determining the
outcome of the immune response is likely to be highly complex and context dependent, as immune responses are likely to have multilayered regulation, at the receptor,
adaptor, transcriptional, translational, and/or posttranslational level. Consistent with
previous studies (56, 57), we observed that Atg5 KO cells can mount a higher type I IFN
response to the dsRNA mimic poly(I·C).
Significantly lower levels of TLR2 were seen in the atg5⫺/⫺ MEFs, which were
rescued by ATG5 reexpression. IL-6 activation and secretion in response to LPS and the
TLR2 ligand Pam3CSK4 were also directly modulated by autophagy, as reexpression of
ATG5 was able to rescue the stunted inflammatory response under autophagy-deficient
conditions. TLR2 signaling is closely related to autophagy induction and flux (72) and
plays important roles in innate immune responses to several bacterial infections,
including Staphylococcus aureus, Pseudomonas aeruginosa, Klebsiella pneumoniae, and
Mycobacterium tuberculosis infections (73, 74), and in the regulation of inflammation
(75).
Our data and analyses provide a global profile of how autophagy modulates the
fibroblast cellular proteome and can potentially impact key cellular processes. We also
validate the crucial role of autophagy in modulation of innate immune responses. This
study should serve as a useful resource for the molecular and cellular machinery that
is regulated by autophagy/ATG5.
MATERIALS AND METHODS
Cells and reagents. WT and Atg5-deficient (atg5⫺/⫺) mouse embryonic fibroblasts were a kind gift
from Noboru Mizushima and obtained through the RIKEN Bio-Resource Cell Bank (catalog numbers
RCB2710 and RCB2711). MEFs were grown in Dulbecco’s modified Eagle’s medium (DMEM) (catalog
number AL007A; HiMedia) supplemented with 10% fetal bovine serum (FBS) (catalog number RM10432;
HiMedia). All media were additionally supplemented with 100 g/ml penicillin-streptomycin and 2 mM
L-glutamine. Antibodies and reagents used in this study are listed in Table S1 in the supplemental
material.
TMT-based mass spectrometry. (i) Sample preparation. The experimental system was designed
for 8-plex TMT-based mass spectrometry analysis (Fig. S1A). For this study, we analyzed four samples,
which were two biological replicates each of WT and atg5⫺/⫺ MEFs. Cells grown in conditioned DMEM
were lysed in a buffer consisting of 50 mM Tris (pH 8.5), 8 M urea, 1% SDS, and protease and phosphatase
inhibitors (catalog number 05056489001; Roche). Protein quantification was done using a microbicinchoninic acid (BCA) assay (catalog number 23225; Pierce). One milligram of protein for each sample
was precipitated using a methanol-chloroform precipitation method and sent for TMT-based mass
spectrometry to the Thermo Fisher Center for Multiplexed Proteomics (TCMP) facility at Harvard Medical
School. Sample digestion, TMT labeling, TMT-based mass spectrometry, and data searches were performed at the TCMP facility. After protein recovery, samples were quantitated, immediately reduced with
dithiothreitol (DTT), and alkylated with iodoacetamide (IAM). Protein from each sample was digested
using endoproteinase-LysC and trypsin, and 75 g of the peptides of each sample was labeled with TMT
reagent. Peptides thus generated were fractionated using basic-pH reverse-phase (bRP) columns.
(ii) Mass spectrometry data acquisition. Peptide fractions from HPRP (high-pH reverse-phase)
separation were analyzed on an Orbitrap fusion mass spectrometer. Peptides were separated using a
gradient of 3% to 25% acetonitrile in 0.125% formic acid over 180 min. Peptides were detected (MS1) and
quantified (MS3) in the Orbitrap, and peptides were sequenced (MS2) in the ion trap.
(iii) Database search and quantification. The raw files were searched using the Sequest algorithm
against the UniProt Mus musculus proteome FASTA database. The FASTA database also contained the
reversed sequences as decoys and known contaminants. TMT tags and carbamidomethylation were used
as fixed modifications, and methionine oxidation was used as a variable modification. The peptide
identifications were filtered at a false discovery rate (FDR) of 1% using the concatenated target-decoy
strategy combined with linear discriminant analysis. An FDR of 1% was applied to the proteins from 4
fractions, and quantitation was carried out from peptides with a summed signal-to-noise (S/N) threshold
of ⱖ200 and an isolation specificity of 0.5.
At a 1% FDR, 151,284 peptides were identified, corresponding to 10,032 proteins. Of these, 8,745
proteins were quantified using TMT reporter tags. The TMT intensities obtained were normalized, and the
replicate intensities were averaged, to calculate the combined areas. These combined replicate areas
were used to calculate the relative ratios. Proteins identified with fewer than two unique peptides were
excluded. Further analysis was performed with 7,795 proteins that were identified with more than two
unique peptides. The fold change was calculated for atg5⫺/⫺ cells versus the WT as follows: FC ⫽ Atg5
KO/WT. Three different stringency threshold conditions were applied to the data: low (FC of ⱖ1.5 and FC
of ⱕ0.666), medium (FC of ⱖ2 and FC of ⱕ0.5) and high (FC of ⱖ3 and FC of ⱕ0.33). The numbers and
identities of over- or underexpressed proteins observed under each condition are provided in Data Set
S1. To ensure maximum coverage and to avoid the loss of information for proteins that might show
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Autophagy-Deficient Basal Fibroblast Proteome
smaller variations in their levels under autophagy deficiency, we utilized differentially expressed proteins
under low-stringency conditions for detailed analysis.
Gene ontology (GO) analysis. The proteins observed to be underexpressed or overexpressed were
used separately for a functional enrichment analysis for biological processes, molecular functions, and
cellular components using GeneCodis 3.0 (76). KEGG pathways were analyzed using GeneCodis, and
Reactome pathway enrichment was carried out using MetaScape (77). All the functional enrichment
categories were filtered at a corrected P value of ⬍0.05 (hypergeometric test in GeneCodis). For pathway
analysis, the filtered list based on the P value from MetaScape and GeneCodis is unified based on the
proteins present in each category for a combined analysis.
Protein-protein interaction network analysis. For protein-protein interaction (PPI) network enrichment analysis, the lists of differentially expressed proteins under the two conditions were studied using
the STRING Web server. The interaction network was made at a medium confidence of 0.400, with
evidence present via experiments, databases, and coexpression only. The network was analyzed based
on KEGG pathway enrichment analysis done with the STRING functional enrichment tool.
Western blotting. Mock-treated and treated WT and atg5⫺/⫺ MEFs were washed using phosphatebuffered saline (PBS) and lysed by adding cell lysis buffer (50 mM Tris-HCl [pH 7.5], 150 mM NaCl, 1%
Triton X-100, a protease inhibitor cocktail [catalog number P8340; Sigma], and phenylmethylsulfonyl
fluoride [PMSF] [CAS number 329-98-6; Sigma]). Protein estimation was done using the micro-BCA assay
(catalog number 23225; Pierce). The lysate was mixed with 4⫻ Laemmli buffer (6% SDS, 40% glycerol,
0.04% bromophenol blue, 20% -mercaptoethanol, 0.25 M Tris [pH 6.8], and water) and further boiled for
10 min at 95°C. Equal amounts of cellular protein were loaded onto and separated on polyacrylamide
gels and later transferred to a polyvinylidene difluoride (PVDF) membrane (Immobilon-P, catalog number
IPVH00010; Merck Millipore) for immunoblotting. Band intensities were quantitated by using ImageJ
software. Data are presented as mean values ⫾ standard deviations (SD) obtained from 3 independent
experiments.
Expression of ATG5 in atg5ⴚ/ⴚ MEFs. The vector backbone or plasmid pCI-neo-mApg5 (Addgene
plasmid 22956) (14) was transfected into WT and atg5⫺/⫺ MEFs, respectively, using Amaxa cell line
Nucleofector kit V according to the manufacturer’s manual (catalog number VCA-1003; Lonza). At 24 h
posttransfection, cells were treated with 100 ng/ml of LPS (catalog number L2630; Sigma) or Pam3CSK4
(catalog number tlrl-pms; InvivoGen) for 3 h. Cells were lysed for Western blotting, cellular RNA was
extracted for real-time reverse transcription-quantitative PCR (qRT-PCR), and the culture supernatant was
used for an IL-6 enzyme-linked immunosorbent assay (ELISA).
Real-time reverse transcription-quantitative PCR. Total RNA from cells was extracted by lysis in
RNAiso Plus reagent (TaKaRa), and 500 ng of total RNA was used for cDNA preparation using random
hexamers and the ImProm-II reverse transcription system (Promega). Primers for all the genes were
designed based on sequences available in the Harvard quantitative PCR (qPCR) primer bank. All qPCRs
were performed using 2⫻ SYBR green reagent (TaKaRa) in a QuantStudio 6 flex RT-PCR machine. Gapdh
levels were used as the internal housekeeping control. The PCR conditions were as follows: 94°C for 2 min
(1 cycle) and 94°C for 15 s, 55°C for 30 s, and 72°C for 1 min (40 cycles). All experiments had biological
duplicates and were performed independently three or more times. The fold changes in the expression
levels of genes are presented as means ⫾ SD of data from three or more independent experiments.
Primer sequences used for quantification of various genes are provided in Table S2.
Interferon/IL-6 ELISA. The culture supernatant was collected from the cells that were mock
transfected or poly(I·C) (catalog number P1530; Sigma) transfected for 6 h, mock/LPS/Pam3CSK4 treated
for 3 h, and centrifuged to remove any debris. An ELISA was performed according to the manufacturers’
protocols for IFN- (catalog number 42400; PBL Assay Science) and IL-6 (catalog number DY406-05; R&D
Systems), respectively.
Statistical analysis. Statistical analysis was done using unpaired Student’s t test or one-way analysis
of variance (ANOVA) followed by Dunnett’s post hoc comparison test. Differences were considered
significant at P values of ⬍0.05, 0.01, 0.001, and ⬍0.0001, as indicated in the figures. Error bars indicate
means ⫾ SD (n ⫽ 3).
Data availability. The mass spectrometry proteomics data have been deposited in the ProteomeXchange Consortium via the PRIDE (78) partner repository under data set accession number PXD014986.
SUPPLEMENTAL MATERIAL
Supplemental material for this article may be found at https://doi.org/10.1128/
mSystems.00481-19.
FIG S1, TIF file, 0.5 MB.
FIG S2, TIF file, 0.6 MB.
FIG S3, TIF file, 0.7 MB.
FIG S4, TIF file, 0.4 MB.
TABLE S1, DOCX file, 0.1 MB.
TABLE S2, DOCX file, 0.1 MB.
DATA SET S1, XLSX file, 4.7 MB.
DATA SET S2, XLSX file, 0.02 MB.
DATA SET S3, XLSX file, 0.1 MB.
DATA SET S4, XLSX file, 0.02 MB.
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Sharma et al.
ACKNOWLEDGMENTS
The work benefited from a DBT-AIST International Center for Translational and
Environmental Research (DIACENTER) grant (BT/BI/14/042/2017) to S.V. K.B.S. is supported by a UGC SRF fellowship. S.A. is supported by an ICMR-SRF grant [BIC/11/(17)/
2015], and A.K.Y. is supported by the DBT-IYBA (DO number BT/07/IYBA/2013) and a
DBT-Big Data Initiative grant (BT/PR16456/BID/7/624/2016). This work was supported
by the SERB under grant EMR/2015/001506 and by THSTI and RCB intramural research
funds. The funders had no role in study design, data collection and interpretation, or
the decision to submit the work for publication.
We acknowledge Ryan Kunj and Mark Jedrychowski at the Thermo Fisher Center for
Multiplexed Proteomics (TCMP) facility at Harvard Medical School for their support with
TMT-based mass spectrometry and data searches. We thank Sankar Bhattacharyya,
Vikas Sood, Vishal Gupta, Nirpendra Singh, Mohd. Ayub Qadri, and C. V. Srikanth for
inputs and help with reagents. We acknowledge all virology lab members for constant
support and encouragement.
We have no conflict of interest to declare.
REFERENCES
1. Deretic V, Saitoh T, Akira S. 2013. Autophagy in infection, inflammation
and immunity. Nat Rev Immunol 13:722–737. https://doi.org/10.1038/
nri3532.
2. He C, Klionsky DJ. 2006. Autophagy and neurodegeneration. ACS Chem
Biol 1:211–213. https://doi.org/10.1021/cb600182h.
3. Levine B, Kroemer G. 2008. Autophagy in the pathogenesis of disease.
Cell 132:27– 42. https://doi.org/10.1016/j.cell.2007.12.018.
4. Klionsky DJ, Cregg JM, Dunn WA, Jr, Emr SD, Sakai Y, Sandoval IV, Sibirny
A, Subramani S, Thumm M, Veenhuis M, Ohsumi Y. 2003. A unified
nomenclature for yeast autophagy-related genes. Dev Cell 5:539 –545.
https://doi.org/10.1016/S1534-5807(03)00296-X.
5. Furuya N, Yu J, Byfield M, Pattingre S, Levine B. 2005. The evolutionarily
conserved domain of Beclin 1 is required for Vps34 binding, autophagy
and tumor suppressor function. Autophagy 1:46 –52. https://doi.org/10
.4161/auto.1.1.1542.
6. Hosokawa N, Hara T, Kaizuka T, Kishi C, Takamura A, Miura Y, Iemura S,
Natsume T, Takehana K, Yamada N, Guan JL, Oshiro N, Mizushima N.
2009. Nutrient-dependent mTORC1 association with the ULK1-Atg13FIP200 complex required for autophagy. Mol Biol Cell 20:1981–1991.
https://doi.org/10.1091/mbc.e08-12-1248.
7. Fujita N, Itoh T, Omori H, Fukuda M, Noda T, Yoshimori T. 2008. The
Atg16L complex specifies the site of LC3 lipidation for membrane biogenesis in autophagy. Mol Biol Cell 19:2092–2100. https://doi.org/10
.1091/mbc.e07-12-1257.
8. Hanada T, Noda NN, Satomi Y, Ichimura Y, Fujioka Y, Takao T, Inagaki F,
Ohsumi Y. 2007. The Atg12-Atg5 conjugate has a novel E3-like activity
for protein lipidation in autophagy. J Biol Chem 282:37298 –37302.
https://doi.org/10.1074/jbc.C700195200.
9. Burger E, Araujo A, Lopez-Yglesias A, Rajala MW, Geng L, Levine B,
Hooper LV, Burstein E, Yarovinsky F. 2018. Loss of Paneth cell autophagy
causes acute susceptibility to Toxoplasma gondii-mediated inflammation. Cell Host Microbe 23:177–190. https://doi.org/10.1016/j.chom.2018
.01.001.
10. Fujimoto C, Iwasaki S, Urata S, Morishita H, Sakamaki Y, Fujioka M, Kondo
K, Mizushima N, Yamasoba T. 2017. Autophagy is essential for hearing in
mice. Cell Death Dis 8:e2780. https://doi.org/10.1038/cddis.2017.194.
11. Hara T, Nakamura K, Matsui M, Yamamoto A, Nakahara Y, SuzukiMigishima R, Yokoyama M, Mishima K, Saito I, Okano H, Mizushima N.
2006. Suppression of basal autophagy in neural cells causes neurodegenerative disease in mice. Nature 441:885– 889. https://doi.org/10
.1038/nature04724.
12. Kuma A, Hatano M, Matsui M, Yamamoto A, Nakaya H, Yoshimori T,
Ohsumi Y, Tokuhisa T, Mizushima N. 2004. The role of autophagy during
the early neonatal starvation period. Nature 432:1032–1036. https://doi
.org/10.1038/nature03029.
13. Li Y, Chao X, Yang L, Lu Q, Li T, Ding WX, Ni HM. 2018. Impaired
fasting-induced adaptive lipid droplet biogenesis in liver-specific Atg5deficient mouse liver is mediated by persistent nuclear factor-like 2
November/December 2019 Volume 4 Issue 6 e00481-19
14.
15.
16.
17.
18.
19.
20.
21.
22.
23.
24.
25.
activation. Am J Pathol 188:1833–1846. https://doi.org/10.1016/j.ajpath
.2018.04.015.
Mizushima N, Yamamoto A, Hatano M, Kobayashi Y, Kabeya Y, Suzuki K,
Tokuhisa T, Ohsumi Y, Yoshimori T. 2001. Dissection of autophagosome
formation using Apg5-deficient mouse embryonic stem cells. J Cell Biol
152:657– 668. https://doi.org/10.1083/jcb.152.4.657.
Nakai A, Yamaguchi O, Takeda T, Higuchi Y, Hikoso S, Taniike M, Omiya
S, Mizote I, Matsumura Y, Asahi M, Nishida K, Hori M, Mizushima N, Otsu
K. 2007. The role of autophagy in cardiomyocytes in the basal state and
in response to hemodynamic stress. Nat Med 13:619 – 624. https://doi
.org/10.1038/nm1574.
Oh DS, Lee HK. 22 March 2019. Autophagy protein ATG5 regulates CD36
expression and anti-tumor MHC class II antigen presentation in dendritic
cells. Autophagy https://doi.org/10.1080/15548627.2019.1596493.
Perot BP, Boussier J, Yatim N, Rossman JS, Ingersoll MA, Albert ML. 2018.
Autophagy diminishes the early interferon-beta response to influenza A
virus resulting in differential expression of interferon-stimulated genes.
Cell Death Dis 9:539. https://doi.org/10.1038/s41419-018-0546-5.
Pua HH, Dzhagalov I, Chuck M, Mizushima N, He YW. 2007. A critical role
for the autophagy gene Atg5 in T cell survival and proliferation. J Exp
Med 204:25–31. https://doi.org/10.1084/jem.20061303.
Stephenson LM, Miller BC, Ng A, Eisenberg J, Zhao Z, Cadwell K, Graham
DB, Mizushima NN, Xavier R, Virgin HW, Swat W. 2009. Identification of
Atg5-dependent transcriptional changes and increases in mitochondrial
mass in Atg5-deficient T lymphocytes. Autophagy 5:625– 635. https://
doi.org/10.4161/auto.5.5.8133.
Wei J, Long L, Yang K, Guy C, Shrestha S, Chen Z, Wu C, Vogel P, Neale
G, Green DR, Chi H. 2016. Autophagy enforces functional integrity of
regulatory T cells by coupling environmental cues and metabolic homeostasis. Nat Immunol 17:277–285. https://doi.org/10.1038/ni.3365.
Yoshii SR, Kuma A, Mizushima N. 2017. Transgenic rescue of Atg5-null
mice from neonatal lethality with neuron-specific expression of ATG5:
systemic analysis of adult Atg5-deficient mice. Autophagy 13:763–764.
https://doi.org/10.1080/15548627.2017.1280221.
Yates JR, III. 2019. Recent technical advances in proteomics.
F1000Research 8:351. https://doi.org/10.12688/f1000research.16987.1.
Thompson A, Schafer J, Kuhn K, Kienle S, Schwarz J, Schmidt G, Neumann T, Johnstone R, Mohammed AK, Hamon C. 2003. Tandem mass
tags: a novel quantification strategy for comparative analysis of complex
protein mixtures by MS/MS. Anal Chem 75:1895–1904. https://doi.org/
10.1021/ac0262560.
Kalvari I, Tsompanis S, Mulakkal NC, Osgood R, Johansen T, Nezis IP,
Promponas VJ. 2014. iLIR: a Web resource for prediction of Atg8-family
interacting proteins. Autophagy 10:913–925. https://doi.org/10.4161/
auto.28260.
Wu X, Won H, Rubinsztein DC. 2013. Autophagy and mammalian development. Biochem Soc Trans 41:1489 –1494. https://doi.org/10.1042/
BST20130185.
msystems.asm.org 18
Autophagy-Deficient Basal Fibroblast Proteome
26. Cecconi F, Levine B. 2008. The role of autophagy in mammalian
development: cell makeover rather than cell death. Dev Cell 15:344 –357.
https://doi.org/10.1016/j.devcel.2008.08.012.
27. Mizushima N, Levine B. 2010. Autophagy in mammalian development
and differentiation. Nat Cell Biol 12:823– 830. https://doi.org/10.1038/
ncb0910-823.
28. Cheng M, Xue H, Cao W, Li W, Chen H, Liu B, Ma B, Yan X, Chen YG. 2016.
Receptor for activated C kinase 1 (RACK1) promotes Dishevelled protein
degradation via autophagy and antagonizes Wnt signaling. J Biol Chem
291:12871–12879. https://doi.org/10.1074/jbc.M115.708818.
29. Ding Y, Kim S, Lee SY, Koo JK, Wang Z, Choi ME. 2014. Autophagy
regulates TGF-beta expression and suppresses kidney fibrosis induced
by unilateral ureteral obstruction. J Am Soc Nephrol 25:2835–2846.
https://doi.org/10.1681/ASN.2013101068.
30. Gao C, Cao W, Bao L, Zuo W, Xie G, Cai T, Fu W, Zhang J, Wu W, Zhang
X, Chen YG. 2010. Autophagy negatively regulates Wnt signalling by
promoting Dishevelled degradation. Nat Cell Biol 12:781–790. https://
doi.org/10.1038/ncb2082.
31. Jia Z, Wang J, Wang W, Tian Y, XiangWei W, Chen P, Ma K, Zhou C. 2014.
Autophagy eliminates cytoplasmic beta-catenin and NICD to promote
the cardiac differentiation of P19CL6 cells. Cell Signal 26:2299 –2305.
https://doi.org/10.1016/j.cellsig.2014.07.028.
32. Jimenez-Sanchez M, Menzies FM, Chang YY, Simecek N, Neufeld TP,
Rubinsztein DC. 2012. The Hedgehog signalling pathway regulates autophagy. Nat Commun 3:1200. https://doi.org/10.1038/ncomms2212.
33. Wu X, Fleming A, Ricketts T, Pavel M, Virgin H, Menzies FM, Rubinsztein
DC. 2016. Autophagy regulates Notch degradation and modulates stem
cell development and neurogenesis. Nat Commun 7:10533. https://doi
.org/10.1038/ncomms10533.
34. Petherick KJ, Williams AC, Lane JD, Ordonez-Moran P, Huelsken J, Collard
TJ, Smartt HJ, Batson J, Malik K, Paraskeva C, Greenhough A. 2013.
Autolysosomal beta-catenin degradation regulates Wnt-autophagy-p62
crosstalk. EMBO J 32:1903–1916. https://doi.org/10.1038/emboj.2013
.123.
35. Araki S, Izumiya Y, Rokutanda T, Ianni A, Hanatani S, Kimura Y, Onoue Y,
Senokuchi T, Yoshizawa T, Yasuda O, Koitabashi N, Kurabayashi M, Braun T,
Bober E, Yamagata K, Ogawa H. 2015. Sirt7 contributes to myocardial tissue
repair by maintaining transforming growth factor-beta signaling pathway.
Circulation 132:1081–1093. https://doi.org/10.1161/CIRCULATIONAHA.114
.014821.
36. Hata A, Shi Y, Massague J. 1998. TGF-beta signaling and cancer: structural and functional consequences of mutations in Smads. Mol Med
Today 4:257–262. https://doi.org/10.1016/S1357-4310(98)01247-7.
37. Murakami G, Watabe T, Takaoka K, Miyazono K, Imamura T. 2003.
Cooperative inhibition of bone morphogenetic protein signaling by
Smurf1 and inhibitory Smads. Mol Biol Cell 14:2809 –2817. https://doi
.org/10.1091/mbc.e02-07-0441.
38. Mowers EE, Sharifi MN, Macleod KF. 2017. Autophagy in cancer metastasis. Oncogene 36:1619 –1630. https://doi.org/10.1038/onc.2016.333.
39. Nighot P, Ma T. 2016. Role of autophagy in the regulation of epithelial cell
junctions. Tissue Barriers 4:e1171284. https://doi.org/10.1080/21688370
.2016.1171284.
40. Catalano M, D’Alessandro G, Lepore F, Corazzari M, Caldarola S, Valacca
C, Faienza F, Esposito V, Limatola C, Cecconi F, Di Bartolomeo S. 2015.
Autophagy induction impairs migration and invasion by reversing EMT
in glioblastoma cells. Mol Oncol 9:1612–1625. https://doi.org/10.1016/j
.molonc.2015.04.016.
41. Pang M, Wang H, Rao P, Zhao Y, Xie J, Cao Q, Wang Y, Wang YM, Lee VW,
Alexander SI, Harris DC, Zheng G. 2016. Autophagy links beta-catenin
and Smad signaling to promote epithelial-mesenchymal transition via
upregulation of integrin linked kinase. Int J Biochem Cell Biol 76:
123–134. https://doi.org/10.1016/j.biocel.2016.05.010.
42. Nighot PK, Hu CA, Ma TY. 2015. Autophagy enhances intestinal epithelial
tight junction barrier function by targeting claudin-2 protein degradation. J Biol Chem 290:7234 –7246. https://doi.org/10.1074/jbc.M114
.597492.
43. Kawano S, Torisu T, Esaki M, Torisu K, Matsuno Y, Kitazono T. 2017.
Autophagy promotes degradation of internalized collagen and regulates
distribution of focal adhesions to suppress cell adhesion. Biol Open
6:1644 –1653. https://doi.org/10.1242/bio.027458.
44. Sharifi MN, Mowers EE, Drake LE, Collier C, Chen H, Zamora M, Mui S,
Macleod KF. 2016. Autophagy promotes focal adhesion disassembly and
cell motility of metastatic tumor cells through the direct interaction of
November/December 2019 Volume 4 Issue 6 e00481-19
45.
46.
47.
48.
49.
50.
51.
52.
53.
54.
55.
56.
57.
58.
59.
60.
61.
62.
paxillin with LC3. Cell Rep 15:1660 –1672. https://doi.org/10.1016/j
.celrep.2016.04.065.
Chu LY, Hsueh YC, Cheng HL, Wu KK. 2017. Cytokine-induced autophagy
promotes long-term VCAM-1 but not ICAM-1 expression by degrading
late-phase IkappaBalpha. Sci Rep 7:12472. https://doi.org/10.1038/
s41598-017-12641-8.
Wang CY, Chiang TH, Chen CL, Tseng PC, Chien SY, Chuang YJ, Yang TT,
Hsieh CY, Choi PC, Lin CF. 2014. Autophagy facilitates cytokine-induced
ICAM-1 expression. Innate Immun 20:200 –213. https://doi.org/10.1177/
1753425913488227.
Sotthibundhu A, McDonagh K, von Kriegsheim A, Garcia-Munoz A,
Klawiter A, Thompson K, Chauhan KD, Krawczyk J, McInerney V,
Dockery P, Devine MJ, Kunath T, Barry F, O’Brien T, Shen S. 2016.
Rapamycin regulates autophagy and cell adhesion in induced pluripotent stem cells. Stem Cell Res Ther 7:166. https://doi.org/10.1186/
s13287-016-0425-x.
Kumar KG, Barriere H, Carbone CJ, Liu J, Swaminathan G, Xu P, Li Y, Baker
DP, Peng J, Lukacs GL, Fuchs SY. 2007. Site-specific ubiquitination exposes a linear motif to promote interferon-alpha receptor endocytosis. J
Cell Biol 179:935–950. https://doi.org/10.1083/jcb.200706034.
Kumar KG, Krolewski JJ, Fuchs SY. 2004. Phosphorylation and specific
ubiquitin acceptor sites are required for ubiquitination and degradation
of the IFNAR1 subunit of type I interferon receptor. J Biol Chem 279:
46614 – 46620. https://doi.org/10.1074/jbc.M407082200.
Xia C, Wolf JJ, Vijayan M, Studstill CJ, Ma W, Hahm B. 2018. Casein kinase
1alpha mediates the degradation of receptors for type I and type II
interferons caused by hemagglutinin of influenza A virus. J Virol 92:
e00006-18. https://doi.org/10.1128/JVI.00006-18.
Chin YR, Horwitz MS. 2005. Mechanism for removal of tumor necrosis
factor receptor 1 from the cell surface by the adenovirus RIDalpha/
beta complex. J Virol 79:13606 –13617. https://doi.org/10.1128/JVI.79
.21.13606-13617.2005.
Yu C, Kastin AJ, Tu H, Pan W. 2007. Opposing effects of proteasomes and
lysosomes on LIFR: modulation by TNF. J Mol Neurosci 32:80 – 89. https://
doi.org/10.1007/s12031-007-0017-4.
King BC, Renstrom E, Blom AM. 2019. Intracellular cytosolic complement
component C3 regulates cytoprotective autophagy in pancreatic beta
cells by interaction with ATG16L1. Autophagy 15:919 –921. https://doi
.org/10.1080/15548627.2019.1580515.
Sorbara MT, Foerster EG, Tsalikis J, Abdel-Nour M, Mangiapane J, SirluckSchroeder I, Tattoli I, van Dalen R, Isenman DE, Rohde JR, Girardin SE,
Philpott DJ. 2018. Complement C3 drives autophagy-dependent restriction of cyto-invasive bacteria. Cell Host Microbe 23:644 – 652. https://doi
.org/10.1016/j.chom.2018.04.008.
Haan C, Is’harc H, Hermanns HM, Schmitz-Van De Leur H, Kerr IM,
Heinrich PC, Grötzinger J, Behrmann I. 2001. Mapping of a region within
the N terminus of Jak1 involved in cytokine receptor interaction. J Biol
Chem 276:37451–37458. https://doi.org/10.1074/jbc.M106135200.
Jounai N, Takeshita F, Kobiyama K, Sawano A, Miyawaki A, Xin KQ, Ishii
KJ, Kawai T, Akira S, Suzuki K, Okuda K. 2007. The Atg5 Atg12 conjugate
associates with innate antiviral immune responses. Proc Natl Acad Sci
U S A 104:14050 –14055. https://doi.org/10.1073/pnas.0704014104.
Tal MC, Sasai M, Lee HK, Yordy B, Shadel GS, Iwasaki A. 2009. Absence of
autophagy results in reactive oxygen species-dependent amplification
of RLR signaling. Proc Natl Acad Sci U S A 106:2770 –2775. https://doi
.org/10.1073/pnas.0807694106.
Kang JY, Nan X, Jin MS, Youn SJ, Ryu YH, Mah S, Han SH, Lee H, Paik SG,
Lee JO. 2009. Recognition of lipopeptide patterns by Toll-like receptor
2-Toll-like receptor 6 heterodimer. Immunity 31:873– 884. https://doi
.org/10.1016/j.immuni.2009.09.018.
Jin MS, Kim SE, Heo JY, Lee ME, Kim HM, Paik SG, Lee H, Lee JO. 2007.
Crystal structure of the TLR1-TLR2 heterodimer induced by binding of a
tri-acylated lipopeptide. Cell 130:1071–1082. https://doi.org/10.1016/j
.cell.2007.09.008.
Zhang T, Shen S, Qu J, Ghaemmaghami S. 2016. Global analysis of
cellular protein flux quantifies the selectivity of basal autophagy. Cell
Rep 14:2426 –2439. https://doi.org/10.1016/j.celrep.2016.02.040.
Zhang T, Wolfe C, Pierle A, Welle KA, Hryhorenko JR, Ghaemmaghami S.
2017. Proteome-wide modulation of degradation dynamics in response
to growth arrest. Proc Natl Acad Sci U S A 114:E10329 –E10338. https://
doi.org/10.1073/pnas.1710238114.
Beauvarlet J, Bensadoun P, Darbo E, Labrunie G, Rousseau B, Richard E,
Draskovic I, Londono-Vallejo A, Dupuy JW, Nath Das R, Guedin A, Robert
G, Orange F, Croce S, Valesco V, Soubeyran P, Ryan KM, Mergny JL,
msystems.asm.org 19
Sharma et al.
63.
64.
65.
66.
67.
68.
69.
70.
71.
Djavaheri-Mergny M. 2019. Modulation of the ATM/autophagy pathway
by a G-quadruplex ligand tips the balance between senescence and
apoptosis in cancer cells. Nucleic Acids Res 47:2739 –2756. https://doi
.org/10.1093/nar/gkz095.
Have M, Balliau T, Cottyn-Boitte B, Derond E, Cueff G, Soulay F, Lornac A,
Reichman P, Dissmeyer N, Avice JC, Gallois P, Rajjou L, Zivy M, MasclauxDaubresse C. 2018. Increases in activity of proteasome and papain-like
cysteine protease in Arabidopsis autophagy mutants: back-up compensatory effect or cell-death promoting effect? J Exp Bot 69:1369 –1385.
https://doi.org/10.1093/jxb/erx482.
Marshall RS, Hua Z, Mali S, McLoughlin F, Vierstra RD. 2019. ATG8binding UIM proteins define a new class of autophagy adaptors and
receptors. Cell 177:766 –781. https://doi.org/10.1016/j.cell.2019.02.009.
Zhao X, Zhu H, Yu J, Li H, Ge J, Chen W. 2016. c-Cbl-mediated ubiquitination of IRF3 negatively regulates IFN-beta production and cellular
antiviral response. Cell Signal 28:1683–1693. https://doi.org/10.1016/j
.cellsig.2016.08.002.
Jiang LQ, Xia T, Hu YH, Sun MS, Yan S, Lei CQ, Shu HB, Guo JH, Liu Y.
2018. IFITM3 inhibits virus-triggered induction of type I interferon by
mediating autophagosome-dependent degradation of IRF3. Cell Mol
Immunol 15:858 – 867. https://doi.org/10.1038/cmi.2017.15.
Harris J. 2011. Autophagy and cytokines. Cytokine 56:140 –144. https://
doi.org/10.1016/j.cyto.2011.08.022.
Levine B, Deretic V. 2007. Unveiling the roles of autophagy in innate and
adaptive immunity. Nat Rev Immunol 7:767–777. https://doi.org/10
.1038/nri2161.
Levine B, Mizushima N, Virgin HW. 2011. Autophagy in immunity and
inflammation. Nature 469:323–335. https://doi.org/10.1038/nature09782.
Mathew R, Khor S, Hackett SR, Rabinowitz JD, Perlman DH, White E. 2014.
Functional role of autophagy-mediated proteome remodeling in cell
survival signaling and innate immunity. Mol Cell 55:916 –930. https://doi
.org/10.1016/j.molcel.2014.07.019.
Trocoli A, Djavaheri-Mergny M. 2011. The complex interplay between
November/December 2019 Volume 4 Issue 6 e00481-19
72.
73.
74.
75.
76.
77.
78.
autophagy and NF-kappaB signaling pathways in cancer cells. Am J
Cancer Res 1:629 – 649.
Lin H, Hua F, Hu ZW. 2012. Autophagic flux, supported by Toll-like receptor
2 activity, defends against the carcinogenesis of hepatocellular carcinoma.
Autophagy 8:1859–1861. https://doi.org/10.4161/auto.22094.
Fang L, Wu HM, Ding PS, Liu RY. 2014. TLR2 mediates phagocytosis and
autophagy through JNK signaling pathway in Staphylococcus aureusstimulated RAW264.7 cells. Cell Signal 26:806 – 814. https://doi.org/10
.1016/j.cellsig.2013.12.016.
Li X, He S, Zhou X, Ye Y, Tan S, Zhang S, Li R, Yu M, Jundt MC, Hidebrand
A, Wang Y, Li G, Huang C, Wu M. 2016. Lyn delivers bacteria to lysosomes
for eradication through TLR2-initiated autophagy related phagocytosis.
PLoS Pathog 12:e1005363. https://doi.org/10.1371/journal.ppat.1005363.
Chuang SY, Yang CH, Chou CC, Chiang YP, Chuang TH, Hsu LC. 2013.
TLR-induced PAI-2 expression suppresses IL-1beta processing via increasing autophagy and NLRP3 degradation. Proc Natl Acad Sci U S A
110:16079 –16084. https://doi.org/10.1073/pnas.1306556110.
Carmona-Saez P, Chagoyen M, Tirado F, Carazo JM, Pascual-Montano A.
2007. GENECODIS: a Web-based tool for finding significant concurrent
annotations in gene lists. Genome Biol 8:R3. https://doi.org/10.1186/gb
-2007-8-1-r3.
Zhou Y, Zhou B, Pache L, Chang M, Khodabakhshi AH, Tanaseichuk O,
Benner C, Chanda SK. 2019. Metascape provides a biologist-oriented
resource for the analysis of systems-level datasets. Nat Commun 10:
1523. https://doi.org/10.1038/s41467-019-09234-6.
Perez-Riverol Y, Csordas A, Bai J, Bernal-Llinares M, Hewapathirana S,
Kundu DJ, Inuganti A, Griss J, Mayer G, Eisenacher M, Pérez E, Uszkoreit
J, Pfeuffer J, Sachsenberg T, Yilmaz S, Tiwary S, Cox J, Audain E, Walzer
M, Jarnuczak AF, Ternent T, Brazma A, Vizcaíno JA. 2019. The PRIDE
database and related tools and resources in 2019: improving support for
quantification data. Nucleic Acids Res 47:D442–D450. https://doi.org/10
.1093/nar/gky1106.
msystems.asm.org 20