ATF3 induces RAB7 to govern autodegradation in paligenosis, a conserved cell plasticity program
Differentiated cells across multiple species and organs can re-enter the cell cycle to aid in injury-induced tissue regeneration by a cellular program called paligenosis. Here, we show that activating transcription factor 3 (ATF3) is induced early during paligenosis in multiple cellular contexts, transcriptionally activating the lysosomal trafficking gene Rab7b. ATF3 and RAB7B are upregulated in gastric and pancreatic digestive-enzyme-secreting cells at the onset of paligenosis Stage 1, when cells massively induce autophagic and lysosomal machinery to dismantle differentiated cell morphological features. Their expression later ebbs before cells enter mitosis during Stage 3. Atf3–/– mice fail to induce RAB7-positive autophagic and lysosomal vesicles, eventually causing increased death of cells en route to Stage 3. Finally, we observe that ATF3 is expressed in human gastric metaplasia and during paligenotic injury across multiple other organs and species. Thus, our findings indicate ATF3 is an evolutionarily conserved gene orchestrating the early paligenotic autodegradative events that must occur before cells are poised to proliferate and contribute to tissue repair.
Pancreatic and gastric exocrine cells regenerate after injury through a process called paligenosis. Injury-induced ATF3 promotes cell autodegradation via transcriptional activation of Rab7b, a regulator of late endosomal and lysosomal trafficking. Atf3 upregulation in injury across diverse organs and species suggests a conserved role in governing the cell plasticity program of paligenosis.
Injury in adult organisms can trigger differentiated cells to reprogram to an embryonic-like, progenitor state. The change from a differentiated cell to a proliferating progenitor-like cell has been shown in nearly every organ, for example, kidney (Kusaba et al, 2014), lung (Hong et al, 2001; Tata et al, 2013), stomach (Nam et al, 2010; Leushacke et al, 2017; Radyk et al, 2018; Willet et al, 2018; Meyer et al, 2019), pancreas (Mills & Sansom, 2015; Willet et al, 2018), intestine (van Es et al, 2012; Jones et al, 2019), and liver (Raven et al, 2017; Chen et al, 2020). As early as 1900, it was proposed that such cellular retooling was a fundamental feature shared by cells, suggesting an evolutionarily conserved program that mature cells could invoke to reroute their energy from performing differentiated cell functions (like secretion of digestive enzymes) to instead undergo mitosis (Adami, 1900).
In the last few years, we have begun to delineate the shared features of injury-induced conversion of mature cells to regenerating proliferative cells (a process termed paligenosis) (Willet et al, 2018). Paligenosis progresses via three distinct, sequential stages: (i) autodegradation of mature cell structures via lysosomal and autophagy pathways, (ii) shift to expression of a progenitor or embryonic gene network, and (iii) re-entry into the cell cycle. Much evidence indicates metaplasias largely arise via cell plasticity (often paligenosis), in particular spasmolytic polypeptide-expressing metaplasia (SPEM) in the stomach and acinar-to-ductal metaplasia (ADM) in the pancreas (Storz, 2017; Burclaff & Mills, 2018; Meyer & Goldenring, 2018). Metaplasia is a lesion characterized by expression of progenitor/embryonic genes, often with increased proliferation, ultimately leading to increased risk for tumorigenesis. Recently, it has become clear that metaplasia in healthy organisms is an evolutionarily conserved injury response that is usually simply a transient, regenerative state that allows tissue to recruit mature cells to help repair injury after large-scale damage (Goldenring, 2018; Saenz & Mills, 2018; Saenz et al, 2018; Burclaff et al, 2020). It is likely that increased cancer risk occurs when metaplasia is chronic and/or with repeated injury (Amieva & Peek, 2016; Giroux & Rustgi, 2017; Storz, 2017; Jin & Mills, 2019; Wroblewski et al, 2019). Accordingly, loss of a key paligenosis gene, Ddit4, increases tumorigenesis by allowing cells to proliferate even with DNA damage present (Miao et al, 2021). This further demonstrates the need to better understand paligenosis as a process that guards against cancer initiation.
Given the evolutionarily conserved role of paligenosis as a mechanism underlying both regeneration and tumorigenesis, we attempted to identify the core set of genes that might be largely dedicated to executing paligenosis. Such paligenosis genes are expected to be evolutionarily conserved, shared across all tissue types, and required only for injury-induced proliferation of differentiated cells but not in dedicated stem cells or during embryonic development. We recently showed that two genes meeting those criteria are Ddit4 (mentioned above) and Ifrd1. DDIT4 is invoked early in paligenosis to quench mTORC1, which must be shut off for the massive autophagy and lysosomal activity of Stage 1, while IFRD1 is essential to restore mTORC1 activity for entry into S phase (Miao et al, 2020b).
Here, we dissect the conserved genetic program that drives the activation of the autodegradation activity in Stage 1. We focus on mechanisms conserved across two exocrine cell populations in two different organs: gastric zymogenic chief cells (ZCs) and pancreatic acinar cells (ACs). These, almost entirely postmitotic, cells live months to years in the absence of injury. ZCs and ACs have large, polarized morphologies with abundant rough endoplasmic reticulum (rER) and numerous, large secretory granules. Their secretory architecture is maintained almost entirely by a two-step transcriptional regulation program with X-box-binding protein 1 (Huh et al, 2010; Hess et al, 2011) transcriptionally activating the secretory granule trafficking transcription factor MIST1 (encoded by Bhlha15) (Pin et al, 2001; Ramsey et al, 2007; Lo et al, 2017; Dekaney et al, 2019). MIST1 induces and maintains expression of numerous transcriptional targets whose gene products in turn coordinate cellular organization, vesicular trafficking, and stress responses (Kowalik et al, 2007). For example, MIST1 binds to and directly upregulates the pro-exocrine secretory apparatus Rab proteins RAB26 and RAB3D by direct transcriptional upregulation of their genes (Tian et al, 2010; Mills & Taghert, 2012; Jin & Mills, 2014). MIST1 is an unique transcription factor; in that, it acts as a scaling factor for cell architecture and maturity by regulating abundance of cell trafficking proteins (Mills & Taghert, 2012).
Rab proteins, like RAB26, RAB3D, and RAB27, are important in gastric zymogenic chief cells and pancreatic acinar cells because they help maintain secretory cell function and cell state (Ohnishi et al, 1996; Tian et al, 2010; Jin & Mills, 2014; Hou et al, 2015; Lo et al, 2017). Other Rab GTPases, like RAB5, RAB7, and RAB9, organize the endolysosomal system. RAB5 traffics the early endosome, RAB7 traffics the late endosome, lysosome, and autophagosome, and RAB9 traffics late endosomes as they transition to the trans-Golgi network (Wandinger-Ness & Zerial, 2014; Langemeyer et al, 2018). There are over 70 human Rab GTPases, which exhibit some overlap in function but can also exhibit distinct functions based on intrinsic characteristics or through protein cofactors. For example, RAB7A and RAB7B are both known to control late endosome maturation and lysosome biogenesis (Guerra & Bucci, 2016); however, they cannot be defined as isoforms because they do not share conserved motifs (Pereira-Leal & Seabra, 2000). The function of RAB7A is generally restricted to late endosomes and facilitates the transition to lysosomes (Bucci et al, 2000), while RAB7B can control endosomal transport to the trans-Golgi network (Guerra & Bucci, 2016) and can interact with cystine protease ATG4B to modulate autophagy (Kjos et al, 2017).
We will show that activating transcription factor 3 (ATF3) is induced during paligenotic injury in diverse organs, working to reverse the MIST1 cell maturation program early in Stage 1. ATF3 is a highly conserved transcription factor with clear orthologues even in primitive multicellular organisms like sea anemones (Nematostella vectensis; https://omabrowser.org/oma/home/) (Altenhoff et al, 2018). ATF3 is rapidly induced following injury, and Atf3 loss in multiple organisms and tissues generally exhibits phenotypes after injury (Hartman et al, 2004; Li et al, 2010; Wang et al, 2012; Brooks et al, 2015; Gey et al, 2016; Fazio et al, 2017; Zhao et al, 2017; Zhu et al, 2018). ATF3 has also been shown to transcriptionally repress MIST1 (Fazio et al, 2017).
Here, we show that ATF3 has a surprising role in vesicle trafficking: it binds to and transcriptionally activates Rab7b (also previously identified as Rab42; Itoh et al, 2006; Marubashi & Fukuda, 2020), which helps govern the maturation of late endosomes to lysosomes (Yang et al, 2004; Progida et al, 2010; Stroupe, 2018). We show RAB7 expression increases dramatically in early paligenotic exocrine cells, forming large accumulations of vesicles and co-labeling, as expected, with autophagic and lysosomal vesicles. Using ATF3 overexpression and knockdown constructs in human epithelial cells and Atf3−/− mice, we show that autodegradative machinery depends on ATF3, partly through transcriptional regulation of Rab7b. Owing to failed degradation in Stage 1, Atf3−/− mice also have markedly aberrant later stages of paligenosis with increased cell death and decreased proliferation and repair in paligenosis Stage 3. We also find ATF3 expression focally in human SPEM, suggesting ATF3 is a staple in early transitions to metaplasia. These data indicate that ATF3 is a key evolutionarily conserved paligenosis gene that acts as one of the first proteins activated in paligenotic injury. It works principally to induce autodegradation, in part, by increasing the lysosome and autophagy coordinator Rab7b.
Degradation of specialized cell features follows exocrine cell injury
To better characterize the early, autodegradation phase of paligenosis at ultrastructural resolution, we identified the organelles and trafficking features that characterize the earliest morphological changes after injury. To induce stomach injury, we used high-dose tamoxifen (HDT), which has been described by our laboratory and others to quickly and synchronously elicit a stomach injury and induce SPEM independent of estrogen receptor activity or sex of mice (Huh et al, 2012; Saenz et al, 2016; Leushacke et al, 2017; Keeley et al, 2019). To induce pancreas injury, we repeatedly treated with the secretagogue cerulein, which has long been described to cause damage to the exocrine pancreas (Adler et al, 1985; Niederau et al, 1985; Saluja et al, 1985; Willet et al, 2018). Injury timelines and how the time points correspond to paligenosis stages are indicated in Fig EV1A and B.
We analyzed the initial downscaling stage of paligenosis via focused ion beam-scanning electron microscopy (FIB-SEM) three-dimensional (3D) nanotomography (Fig 1A and Movies EV1–EV4). FIB-SEM of vehicle-treated ZCs compared to 24-h HDT-treated ZCs revealed a dense accumulation of lysosomes and autolysosomes in the basal region of the cell, where the cell’s rER network and many mitochondria are concentrated. In addition to loss of rER, we saw exocrine granule degradation as well as swelling and fragmenting of mitochondria. The ultrastructural changes were corroborated by immunofluorescence at 6 and 24-h HDT showing gradual loss of GIF+ exocrine granules coincident with increased LAMP1+ lysosomes (Fig 1B). Transmission electron microscopy (tEM) showed that ZCs following 24-h HDT injury harbored increased lysosomes and double-membrane bound vesicles (consistent with autophagosomes) filled with cell components, such as granules, ER, and cytosol (Fig 1C). Granular census was also reduced (Fig 1D), consistent with downscaling of mature cell architecture and an increase in single- and double-membraned vesicles, which we summarize and quantify as autodegradation events (Fig 1E). Similarly, we saw decreased granule number and increased autodegradation events in pancreatic ACs following repeated cerulein (CER) injury for one day (Fig 1F–H). These results support our initial description (Willet et al, 2018) that Stage 1 of paligenosis consists of an increase in both lysosomal and autophagic degradation pathways and further clarifies which organelles are targeted for degradation.
We wanted to determine whether lysosomes and autophagosomes are required for paligenosis progression in the stomach, so we treated mice with hydroxychloroquine (HCQ; 60 mg/kg/day). Intraperitoneal injection of HCQ dampens autophagic activity by blocking autophagosome–lysosome fusion (Rosenfeldt et al, 2013; Cao et al, 2017). A 3-day course of HCQ significantly decreased the fraction of stomach units that exhibit SPEM (Fig EV1, EV2-EV5C–F). We also saw many ZCs that appeared to never downscale their granules (meaning they did not undergo the autodegradative processes Stage 1), as marked by sustained GIF expression and residually large apical cytoplasms (Fig EV1, EV2-EV5D–F). Thus, lysosomes and autophagosomes are necessary for Stage 1 of paligenosis and, consequently, for subsequent progression of cells to Stage 2, which is characterized by induction of SPEM markers.
The massive degradation events occurring early in paligenosis indicated that cellular membrane trafficking was dramatically altered and pointed to alterations in the Rab family of small GTPases. RABs facilitate vesicle and organelle movement and are especially important for cells with secretory functions, like exocrine cells in the stomach and pancreas (Johnson et al, 2004; Faust et al, 2008; Fukuda, 2008; Tian et al, 2010; Jin & Mills, 2014; Takahashi et al, 2017). RAB function can be regulated at the transcriptional level in exocrine cells (Johnson et al, 2004; Tian et al, 2010). Accordingly, we found a significant increase in Rab7b (though not Rab5, Rab7a, Rab9) mRNA at 12-h HDT treatment: the time when the majority of ZCs are in Stage 1 of paligenosis (Fig 1I). Our analysis of a previously published dataset (Kowalik et al, 2007) also suggests that Rab7b is expressed in pancreatic acinar cells following cerulein-induced pancreatitis. Together the findings suggest that, like Rab26 and Rab3d, Rab7b is transcriptionally controlled in exocrine cells.
ATF3 binds to and directly induces the Rab7b gene during paligenotic downscaling
While there was little RAB7 expression in vehicle-treated stomach and pancreas, we observed large balloons and crescents of RAB7+ vesicles during stage 1 of paligenosis in stomach and pancreas (Fig 2A and D). Note that we have not found an antibody that can distinguish RAB7B from RAB7A in tissue sections, so we used total RAB7 antibody for these immunostaining studies. However, we favor the interpretation that the majority of the RAB7+ vesicles are likely RAB7B vesicles, given qRT–PCR and Western blot showed only Rab7b mRNA and RAB7B protein are induced consistently after paligenotic injury in pancreas and stomach (Fig EV2A and B). In contrast, there was no consistent pattern of increased expression in any of the following paligenotic injury scenarios in pancreas and stomach: total RAB7 protein by Western blot of whole tissue (Fig EV2A and B), Rab7a mRNA by qRT–PCR from whole tissue (Fig 1I), and RAB7A protein by Western blot of whole tissue (Fig EV2A and B).
We reasoned that the transcriptional upregulation of Rab7b specifically within early paligenosis might give us a route to identify, for the first time, early transcriptional regulators of the paligenosis process. Our previous work showed that MIST1 activates Rab transcription (e.g., Rab3d and Rab26) by binding within well-conserved cis-regulatory regions within the first intron. Thus, we used the MEME Suite web server (Bailey et al, 2009) and FIMO (Find Individual Motif Occurrences) software (Grant et al, 2011) to identify transcription factor binding sites within the first intron of Rab7b. A putative ATF3-binding motif was identified within this region. More detailed analysis using Contra v3 (Kreft et al, 2017) (http://bioit2.irc.ugent.be/contra/v3) (Fig EV3A–C) further corroborated that a potential ATF3 site was highly evolutionarily conserved across mammals. ATF3 was previously characterized in the early stages of cerulein-induced pancreatitis in mice (Fazio et al, 2017; Data ref: Fazio et al, 2017) and our in silico-predicted ATF3-binding site matched a site from chromatin immunoprecipitation sequencing (ChIP-Seq) analysis of genomic ATF3 binding early after cerulein injury from the published dataset (Fig EV3A–C). ATF3 was also an appealing target because it was previously described as one of the most highly upregulated genes in a mouse model of SPEM (Nozaki et al, 2008; Miao et al, 2020b). Thus, the data pointed to ATF3 as a key transcription factor early in paligenosis, potentially activating Rab7 to facilitate the massive autophagic changes in Stage 1.
Accordingly, ATF3 was rapidly induced specifically within ZCs and ACs following injury (Fig 2A and D), and Atf3 transcript and ATF3 protein were also both increased in whole tissue analysis of the stomach and pancreas (Fig 2B and C). ATF3 was dramatically increased early in paligenosis Stage 1, but its expression returned to almost homeostatic levels in paligenosis Stage 3. Moreover, ATF3 binding to the Rab7b gene in stomach tissue was confirmed using ChIP (Fig 2E) with primers designed to amplify genomic DNA including the consensus ATF3 intronic binding site described above (Fazio et al, 2017). We used an equivalent intronic region in the Rab9a gene (which has similar function and gene structure; Mackiewicz & Wyroba, 2009) as a negative control and a previously identified ATF3-binding site within the Atf3 gene as a positive control (as ATF3 can transcriptionally regulate itself (Inoue et al, 2004)). As predicted, ATF3 specifically bound both to Atf3 and Rab7b (vs. non-specific IgG and Rab9 negative controls) with binding greatly increased early (6 h) after injury. Thus, induction of ATF3 activity and the consequent activation of Rab7 occurs very early following injury; indeed, it is the earliest conserved molecular event we have so far identified in paligenosis.
ATF3 can act as a transcriptional activator or repressor depending on the gene and the context (Hai et al, 1999). To confirm that ATF3 activated Rab7b and to test if their molecular interaction was conserved across species, we used AGS cells (a human gastric epithelial line) to generate stable cell clones that overexpressed ATF3 or stably repressed ATF3 using shRNAs. AGS cells did not express substantial endogenous ATF3, though cells expressing anti-ATF3 shRNA (ATF3-KD) still expressed less (Fig 3A). ATF3-KD caused statistically significant decrease in RAB7B mRNA and fewer cells with detectable RAB7 protein, and conversely, when ATF3 protein was overexpressed (ATF3-OE), we saw an induction of RAB7 protein and mRNA (Fig 3A and B). Of note, many of the ATF3-OE cells showed large RAB7+ globular and crescentic vesicular formations phenocopying those seen in vivo in paligenotic murine cells (Fig 3C). Our in vivo data suggested that ATF3 could induce autophagy in part via directly increasing RAB7 abundance. Supporting our hypothesis, we noted increased cathepsin D (CTSD)-positive lysosomes in cells with higher expression of ATF3 correlating consequently with increased RAB7B (Fig 3C). To determine whether RAB7B was sufficient, even in the absence of ATF3, to induce these large vesicles observed in vivo and in vitro, we forced expression of FLAG-tagged, WT RAB7B in ATF3-KD cells. Figure 3D shows the large vesicular phenotype is even more dramatic with RAB7B overexpression. On the other hand, transfection with RAB7BT22N, a GTPase-dead RAB7B mutant (GTPase cycling is critical for RABs to traffic and maintain vesicular compartments), abrogated the phenotype (Fig 3D). These results are consistent with previous reports that RAB7BT22N impairs endolysosomal trafficking necessary for maturation of cathepsin D, which is activated in its pro-form in the lysosome (Progida et al, 2010). Taken together, ATF3 is sufficient to transcriptionally activate RAB7B, and RAB7B itself (whether ATF3-induced or transfected) is sufficient to activate the endolysosomal pathway to facilitate cell autodegradation. While ATF3, a transcription factor, may also induce other genes that activate autodegradation pathways, our results indicate RAB7B appears to be a principal target in paligenosis.
Atf3 is required for massive lysosome and autophagy induction in Stage 1 of paligenosis
To determine whether loss of Atf3 results in decreased Rab7 in vivo, we studied paligenosis in stomach and pancreas of Atf3−/− mice (Hartman et al, 2004). It is important to note that these mice have a global loss of Atf3, meaning Atf3 is neither in differentiated nor in progenitor cells. However, since we only see ATF3 induction in differentiated cells after injury, Atf3’s main role is primarily in differentiated cells. In addition, we observed ATF3 induction in ACs in the pancreas, where there is no adult stem cell population, again suggesting that ATF3 mainly functions in differentiated cells after injury. In WT mice, we observed scant RAB7 in vehicle tissue of the stomach or pancreas, but following injury in WT animals, we saw the previously observed RAB7+ vesicles and large circular aggregates. Many of the large RAB7-vesicles were lysosomes or autolysosomes as indicated by enclosed CTSD (Fig 4A and B). Although low-abundance RAB7 could still be detected in ZCs and ACs of Atf3−/− mice, the large RAB7-positive vesicles were predominantly lacking. Injury induced RAB7+ vesicles in WT mice, but in Atf3−/− mice, we did not observe upregulation of large RAB7+ vesicles (Fig 4A and B).
Cathepsin D is a marker of both lysosomes and autolysosomes, so we next examined whether loss of ATF3 and RAB7 affected autophagic trafficking. We observed that the autophagic vesicle marker MAP1LC3B (LC3) was induced in Stage 1 of paligenosis in the stomach, consistent with previous work and our EM analysis indicating increased autophagic trafficking (Willet et al, 2018; Meyer et al, 2019; Fig 4C). Such LC3+ autophagic puncta were not induced in the absence of ATF3. We confirmed ATF3-dependent induction of lysosomes and autophagosomes using TEM (Fig 4D and E).
The results indicate ATF3 is induced rapidly in paligenosis and is required for RAB7-associated autophagy/lysosomal trafficking. Thus, ATF3 is both necessary and sufficient to induce the endolysosome-trafficking protein RAB7 and is critical for the massive induction of autodegradative machinery that cells use in Stage 1 of paligenosis to downscale much of their mature cell architecture.
Atf3 loss results in less repair and more cell death after secretory cell injury
Paligenosis is a stepwise process, that can be inhibited between each stage. We have previously shown that blocking autodegradative function during paligenosis impairs regeneration (Willet et al, 2018). We reasoned the aberrant induction of autodegradation in the absence of ATF3 would affect the fraction of cells able to progress to Stage 2 (expressing metaplastic/progenitor genes) and Stage 3 (entering the cell cycle). Stage 2 is easily measured by induction of the epitope for the lectin GSII in ZCs, with the resultant cells (known as SPEM cells) co-labeling with GSII and ZC markers (like PGC or GIF). Atf3−/− mice showed profound loss of progression to Stage 2, with only rare SPEM cells (Figs 5A and EV4A–C). Stage 2 failure was corroborated by a second SPEM marker CD44v (Fig EV4A; Khurana et al, 2013; Engevik et al, 2016; Meyer et al, 2019). Moreover, the failure to produce Stage 2 SPEM cells correlated with reduced proliferation (Figs 5B and C, and EV4D). Note that progenitors higher up in the gastric unit (in the isthmus and neck) are induced to proliferate via a non-paligenotic mechanism (Willet et al, 2018; Choi et al, 2019; Miao et al, 2020a; Miao et al, 2020b). As expected, those non-paligenotic cells were still induced to proliferate after injury, so overall proliferation in the injured stomach was less affected by loss of ATF3 than paligenotic proliferation specifically (Fig EV4D; cf: Fig 5B vs. Fig 5C showing basal, paligenotic proliferation).
We noticed that the lack of paligenotic progression to stages 2 and 3 did not indicate mature cells were delayed in the paligenotic process, as many of the bases of gastric units, where ZCs or paligenotic cells should be, were simply missing. This pattern was consistent with dropout of whole gastric unit bases, a phenomenon we have previously described when there is a failure to progress through paligenosis (Willet et al, 2018; Miao et al, 2020b). Inability to complete paligenosis resulted in marked base dropout with approximately 1/3 of gastric unit bases missing (Fig 5D). As might be expected, the increased base dropout in Atf3−/− correlated with significantly increased cleaved-CASP3 positivity, indicating cell death by apoptosis (Fig EV4E and F). In the pancreas, ATF3 was also required for paligenosis progression, as Atf3−/−ACs had significantly higher cleaved-CASP3 expression (Fig 5E and F) as well as decreased Stage 3 proliferation induction (Fig 5G and H).
Overall, the results indicate that the failure to upregulate autodegradation in Stage 1, in the absence of Atf3, led to the failure to progress through Stage 2 of paligenosis and finally resulted in increased cell death in Stage 3, in both stomach and pancreas.
ATF3 is critical for injury responses across organs
Our studies thus far showed that ATF3 could regulate autodegradative activity in a conserved way across tissue and species by regulating RAB7. In addition, loss of ATF3 caused the same Stage 1 failure with associated overall paligenosis failure in two different organs, suggesting that early ATF3 induction might be a conserved feature of paligenosis. HDT injury-producing SPEM in mice is a model of the SPEM that occurs in chronic atrophic gastritis in humans (Petersen et al, 2017). Using human stomach samples of tissue adjacent to gastric tumor tissue, we have previously extensively characterized (Lennerz et al, 2010; Radyk et al, 2018; Willet et al, 2018), we observed expression of ATF3 in SPEM. However, as might be expected, given ATF3 expression was early and transient following injury in mice, and most SPEM is chronic and mitotically quiescent in humans (Willet et al, 2018; Burclaff et al, 2020) scattered, potentially transitional SPEM cells were ATF3-positive (Fig 6). Morphologically normal human gastric epithelial cells lacked ATF3 expression (Fig 6).
As ATF3 is highly conserved, we took advantage of a previously published Axolotl single-cell RNA-sequencing analysis of limb regeneration (Gerber et al, 2018; Data ref: Gerber et al, 2018) that shows high correlation with gene expression in mouse paligenosis (Miao et al, 2020b). We found that, like the previously identified paligenosis gene IFRD1, ATF3 is induced during limb regeneration. RAB7B is induced at the next time point after ATF3 (Fig EV5A), as represented by the fraction of cells that express these genes throughout the course of repair after limb amputation. We previously showed that regenerative proliferation in kidney and liver occurs by paligenosis (Willet et al, 2018), and activation of muscle satellite cells following injury (Yue et al, 2020) also appears to involve a paligenosis-like process involving emergence from quiescence. We assayed genes whose expression was increased after paligenotic injury in all 5 organs: stomach, pancreas, liver, kidney, and muscle to determine potential core paligenosis genes (Fig EV5B). We found only 7 genes were upregulated in all 5 datasets: Atf3, Cebpb, Hmox1, Ier3, Ifrd1 (Fahling et al, 2013; Data ref: Fahling et al, 2013; Kowalik et al, 2007; Data ref: Kowalik et al, 2007; Moore et al, 2015; Data ref: Moore et al, 2015; Otu et al, 2007; Data ref: Otu et al, 2007; Yue et al, 2020; Data ref: Yue et al, 2020), Junb, and Zfp36. Thus, the results indicate Atf3 may play a conserved role in mediating paligenosis across multiple tissues and species.
Our work here shows that ATF3, induced early in Stage 1 of paligenosis, is required for initiation of the autodegradative machinery. Though there are likely additional targets critical for ATF3 actions in paligenosis, we show both in mouse paligenosis models and in human epithelial cells that ATF3 binds and activates Rab7b, which encodes a protein critical in turn for trafficking autophagic vesicles and lysosomes. ATF3 is necessary for RAB7 induction and for induction of a large complement of autophagolysosomes. ATF3 induction after paligenotic injury is conserved across tissues and species with ATF3 increased even in human metaplasia.
The concept of an evolutionarily conserved program, paligenosis, which mechanizes cell plasticity for mature cells, like pancreatic or gastric exocrine cells, is recent. Paligenosis, as originally defined, is a stepwise program that retools cell architecture to convert a mature cell to a regenerative, progenitor-like phenotype. The three paligenosis stages (1. autodegradation, 2. increased progenitor/metaplastic expression, and 3. cell cycle re-entry) can be genetically and morphologically defined, and progression from stage to stage can be blocked by inhibitors or deletion of key genes (Fig 7). The stepwise, conserved nature of the program allows us to determine whether there are dedicated, paligenosis genes and genetic machinery, independent of tissue and conserved across evolutionary phyla, as is the case with other cellular programs like apoptosis. We recently identified Ifrd1 and Ddit4 as paligenosis-governing genes and proposed that paligenosis genes in general would be: (i) largely dispensable for normal development or proliferative activity; (ii) activated primarily during regeneration-inducing injury; and (iii) highly evolutionarily conserved. We argue here that ATF3 is a similar such gene required for paligenosis. It is upregulated early in paligenosis in multiple tissues, is known to be induced by injury, and is conserved from sea anemones to humans, and, in general, organisms null for ATF3 have phenotypes only after injury. Furthermore, we show evidence here that ATF3 is expressed during transition to metaplasia in humans, which is representative of a much larger cohort (> 500) that we are currently analyzing for expression of paligenosis genes. We observe 11% of human metaplastic lesions have focal ATF3 in non-proliferative foci, consistent with ATF3 being upstream of the decision for cells to proliferation.
We describe a model (Fig 7) in which ATF3 is induced early after injury to help transcriptionally upregulate Rab7b and other genes important for autophagy and lysosomal accumulation during paligenosis Stage 1. During this time ATF3 also likely transcriptionally represses genes involved in cell differentiation/maturation like MIST1, a relationship that has been shown before in pancreas (Fazio et al, 2017). Shortly after Stage 1, ATF3 decreases, and the cell progresses through the remainder of paligenosis. Without Atf3, the defects in Stage 1 (autodegradation) obstruct the cell’s ability to become regenerative, metaplastic cells. A greater proportion of cells die and tissue repair is compromised. In addition, we describe a new signaling axis for injury-induced cell plasticity by ATF3 transcriptional regulation of Rab7b during paligenosis.
Atf3 joins aforementioned Ddit4 and Ifrd1 as paligenosis-governing genes (Miao et al, 2020b). At the tissue level, loss of Atf3 appears most similar to loss of Ifrd1 as lack of either gene leads to increased cell death in paligenosis Stage 3. While IFRD1 functions to suppress p53-mediated repression of mTORC1, allowing proliferation in Stage 3, ATF3 instead activates autodegradation pathways for proper clearance of differentiated/specialized cell features. Though both ATF3 and IFRD1 have different mechanisms to govern paligenosis, it is clear that failure to clear paligenosis checkpoints, either by inability to upregulate autodegradation (Atf3−/−) or by inability to re-activate mTORC1 (Ifrd1−/−), leads to decreased tissue recovery after injury. ATF3 and DDIT4 both function in Stage 1 to control autodegradation. Unlike Atf3, however, Ddit4−/− mice have increased proliferation. DDIT4 functions during initial stages to deactivate mTORC1; hence, Ddit4−/− mice express constitutively high mTORC1 throughout paligenosis, which overrides a checkpoint (Miao et al, 2020b). Additionally, loss of Ddit4 and induction of metaplasia increases tumorigenesis in an N-methyl-N-nitrosourea spontaneous gastric cancer model (Miao et al, 2021).
Activating transcription factor 3 is a member of the ATF/CREB family of transcription factors and shares similar binding sites with AP-1 (also from the ATF/CREB and c-Fos/c-Jun families), which regulates immediate early genes following stress/injury. Atf3 has been implicated in injury settings in many organs including cerebral ischemia (Wang et al, 2012), axon regeneration (Hunt et al, 2012; Gey et al, 2016), acute lung injury (Zhao et al, 2017), heart failure (Brooks et al, 2015), alcohol liver damage (Tsai et al, 2015), liver ischemia-reperfusion injury (Zhu et al, 2018), stress-induced β-cell apoptosis (Hartman et al, 2004), ADM (Fazio et al, 2017; Azizi et al, 2021), and acute kidney injury (Li et al, 2010). ATF3 is also important for injury responses in Drosophila (Zhou et al, 2017) and Axolotl (Gerber et al, 2018). In all those cases, Atf3 loss exacerbates the injury phenotype but is dispensable for homeostasis and embryonic development, just as we observed here in stomach and pancreas injury. A recent publication similarly showed that Atf3 loss leads to decreased ADM and that absence of Atf3 in a spontaneous cancer mouse model actually prevented KRASG12D-driven pancreatic cancer (Azizi et al, 2021). That may be consistent with our results here, as mutant KRAS-driven cancer depends on ADM, which depends on ATF3 and paligenosis. Cells lacking ATF3 may die rather than transform. Thus, the role of ATF3 in cancer is complex and under active study.
It has not been previously reported that injury-responsive ATF3 accumulation induces autophagy and lysosomal activity, but ATF3 has been reported to interact with individual autophagy pathway members. For example, ATF3 regulates Beclin-1 (Lin et al, 2014) and Atg5 (Sood et al, 2017). There may also exist an autophagy-ATF3 feedback loop because defective autophagy (Atg4b loss) impairs ATF3 activity in a mouse lung injury model (Aguirre et al, 2014).
To our knowledge, there are no previous reports of ATF transcription factors transcriptionally regulating any Rabs, though potential ATF binding sites have been described to be present in the 5’-flanking region of Rab7 (Bhattacharya et al, 2006). In fact, in general, transcriptional regulation of RABs or regulation of RAB function via titrating protein abundance is usually not studied, with some few exceptions such as MIST1 scaling RABs, and a report of c-Myc helping drive melanoma by activating Rab7 (Alonso-Curbelo et al, 2014). However, an ATF-related protein, AP-1, regulates Rab11a in B cells in mice (Lizundia et al, 2007), suggesting that ATF/CREB transcription factors may have an underappreciated and understudied role in transcriptionally regulating RABs.
RAB7A and RAB7B are regulators of endosomal trafficking and maturation. RAB7 proteins are largely localized to late endosomes and lysosomes to aid in the autophagosome–lysosome fusion and mitochondrion–lysosome contacts (Stroupe, 2018), events undoubtedly important during Stage 1 of paligenosis. As such, complete Rab7 loss in pancreatic acinar cells impairs autophagic and endocytic pathways in mouse models of pancreatitis (Takahashi et al, 2017). Here, we show that Atf3 loss impairs autophagic and lysosomal pathways, further supporting the notion of ATF3 function through Rab7b during paligenosis and injury. There are few studies specifically focused on RAB7B, identified because of its size and sequence similarity to RAB7A. RAB7B has similar functions as RAB7A and was, accordingly, first observed to be associated with lysosomes in monocytes (Yang et al, 2004). More recently, RAB7B has been shown to interact with ATG4B on vesicles and negatively regulate autophagy (Kjos et al, 2017), indicating it also, like RAB7A, regulates autophagic trafficking. There may not be complete concordance between the two RAB7 proteins, however, as RAB7B may have an added function in some circumstances of aiding retrograde transport from late endosomes or lysosomes to the Golgi (Progida et al, 2010).
Using AGS cells, we demonstrated that expression of RAB7B was sufficient to form the large vesicular compartments observed following injury in murine tissue. This effect was independent of ATF3 expression, as vesicles were readily observed with ATF3 knockdown and RAB7B overexpression. In addition, vesicle formation was dependent on RAB7B’s GTPase activity, as no vesicles were observed with the RAB7BT22N mutant, even with overexpression of ATF3.
Recent studies have shown the importance of degradation and autophagy in regulating cell plasticity in several organs (Saera-Vila et al, 2016; Call & Nichenko, 2020; Li et al, 2020; Romermann et al, 2020). We speculate that Stage 1 of paligenosis is not only required to change the cell structure to one that is more physiologically progenitor-like but also to generate enough energy for DNA replication and cell division. Ribosomes are an enormous pool for nucleotides, which may be one reason we see so much degradation machinery accumulate in the rER portion of the cell, where there may be release of nucleotides from ribosomes. As mentioned above, functional degradation machinery may also act as a checkpoint indicating a cell is healthy enough to commit to cell cycle re-entry. This was the case when we administered hydroxychloroquine to inhibit lysosome–autophagosome fusion (Fig EV1, EV2-EV5C–F) and when we blocked lysosome activity during paligenosis (Willet et al, 2018) which, like Atf3 and Ifrd1 loss, also ultimately led to increased cell death.
Activating transcription factor 3 may transcriptionally regulate other targets during Stage 1 that do not control degradation. ATF3 can repress Mist1, the secretory cell scaling factor expressed only in mature ZCs and ACs; Mist1 downregulation is a key early step in ZC and AC paligenosis (Kowalik et al, 2007; Nozaki et al, 2008; Lennerz et al, 2010; Karki et al, 2015; Meyer et al, 2019). It also represses Sox9 (Fazio et al, 2017), a metaplastic gene whose induction defines transition from Stage 1 to Stage 2, supporting the hypothesis that ATF3 plays several roles in Stage 1 of paligenosis. It is not clear how ATF3 is upregulated for paligenosis and metaplasia initiation, but once accumulated, ATF3 acts in a positive feedback loop to regulate itself. Reactive oxygen species are also induced en route to SPEM and may contribute to autodegradation and antioxidant pathway activation, as shown by the induction of antioxidant gene xCT, a cysteine/glutamate transporter in SPEM (Meyer et al, 2019). Likewise, reactive oxygen species are important for ADM induction and progression to pancreatic adenocarcinoma (Liou et al, 2016; Cheung et al, 2020).
The current study stimulates several important questions. First, how does metabolism affect the cell fate transitions in paligenosis? We saw dramatic structural changes in mitochondria during paligenosis, which likely reflect changes in metabolism. The metabolic profile of cells as they transition from their normal state to a metaplastic state is not well characterized, though a recent study demonstrated disrupted acinar cell cholesterol metabolism underlies pancreatitis in mouse models (Mareninova et al, 2021). We showed a dependency on dynamic mTORC1 activity during metaplasia (Willet et al, 2018) and recent studies show acetyl-CoA metabolism contributes to cell plasticity in the pancreas and potentially tumorigenesis via epigenetic regulation (Carrer et al, 2019). Epigenetics also plays a role in SPEM initiation, most recently shown by miR148a repression of DNA-methylating gene DNMT1, a pro-metaplasia gene (Shimizu et al, 2020). Second, which cells are poised to undergo paligenosis and become metaplastic? Not all mature cells in a tissue may have the ability to re-enter the cell cycle after injury, but organs experiencing chronic damage (like GI organs) harbor cells that act as facultative progenitors if the injury is severe enough, though the age of cells in the GI system is a factor for their ability to contribute to plasticity (Engevik et al, 2016; Weis et al, 2017) and some cell types like acid-secreting parietal cells seem unable to return to the cell cycle. Further study of general, conserved genes that govern paligenosis in diverse contexts should help us have a better understanding of regeneration, tumorigenesis, and also potentially how plasticity arose as a way for multicellular organisms to use cells for both specialized, differentiated function and as progenitors after damage.
Materials and Methods
Reagents and Tools table
|Reagent/Resource||Reference or Source||Identifier or Catalog number|
|C57BL/6J (M. musculus)||Jackson Lab||Stock No: 000664|
|Atf3–/– (M. musculus)||Hartman et al (2004)|
|AGS cells (H. sapiens)||ATCC||CLR-1739|
|XL-10 Gold Ultracompetent Cells||Agilent||Cat #200317|
|Human patient samples||Lennerz et al (2010), Capoccia et al (2013), Khurana et al, (2013), Radyk et al (2018)|
|ATF3 (human)||Sequence cloned out of Addgene #26115 and inserted into a homemade PiggyBac Transposon vector for overexpression (vector also used in ref. Miao et al (2020)||Cat #26115|
This sequence template was also used to generate the RAB7BT22N mutant by amplifying a truncated C-terminal domain and a three-part ligation using oligos encoding the mutant N-terminal domain.
Methods and Protocols
Animal studies and reagents
All experiments involving animals were performed according to protocols approved by the Washington University School of Medicine Animal Studies Committee. Mice were maintained in a specified pathogen-free barrier facility under a 12-h light cycle. All mice used in experiments were 6−8 weeks old. Male and female mice were used for each experiment, and we did not note any differences due to sex. Statistical justification for animal numbers is based on our previous experience, consultation with biostatisticians, and using the sampling power analysis approach. Animals were randomized when allocating into each treatment groups. Experimental cohorts were randomly designated at birth for specific animals to minimize bias. Wild-type C57BL/6 mice were purchased from Jackson Laboratories (Bar Harbor, ME). Atf3–/– mice were bred onto a C57BL/6 background and received from Dr. Tsonwin Hai at the Ohio State University Medical Center. Atf3–/– mice were first described in Ref. Hartman et al (2004).
Tamoxifen (250 mg/kg body weight; Toronto Research Chemicals, Inc, Toronto, Canada) was administered by intraperitoneal (IP) injection to induce SPEM in the stomach (see Fig EV1 for timeline; Saenz et al, 2016). Tamoxifen was prepared in a 10% ethanol and 90% sunflower oil solution by sonication (Sigma, St Louis, MO).
Pancreatitis was induced by 6 hourly IP injections of 50 μg/kg (in 0.9% saline) cerulein (Sigma-Aldrich) given every other day for up to 7 days (see Fig EV1 for timeline). Mice were sacrificed 24-h after the final cerulein injection.
All mice were given an intraperitoneal injection containing BrdU (120 mg/kg) and 5-fluoro-2′-deoxyuridine (12 mg/kg) 90 min before sacrifice to capture cells in S phase at the experimental endpoint.
Immunofluorescence and immunohistochemistry
Mouse tissues were excised, flushed with phosphate-buffered saline (PBS), and then inflated with freshly prepared 4% paraformaldehyde. The stomach was clamped and suspended in fixative in a 50-ml conical overnight, followed by rinses in PBS and 70% ethanol, arrangement in 3% agar in a tissue cassette, and paraffin processing. Sections (5 μm) were cut, deparaffinized, and rehydrated with graded Histo-Clear (National Diagnostics), ethanol, and water, then antigen-retrieved in sodium citrate buffer (2.94 g sodium citrate, 500 μl Tween 20, pH 6.0) using a pressure cooker. Slides were blocked in 5% normal serum, 0.2% Triton X-100, in PBS. Slides were incubated overnight at 4°C in primary antibodies (see Reagent Table), then rinsed in PBS, incubated 1 h at room temperature in secondary antibodies, and/or fluorescently labeled lectin rinsed in PBS, mounted in ProLong Gold Antifade Mountant with 4′6-diamidino-2-phenylindole (DAPI) (Molecular Probes).
For immunohistochemistry, steps were identical except the following. An extra quenching step was performed for 15 min in a methanol solution containing 1.5% H2O2 before antigen retrieval. Substrate reaction and detection was performed using ImmPACT VIP Peroxidase (horseradish peroxidase) Substrate Kit (Vector Laboratories, Burlingame, CA) as detailed per the manufacturer’s protocol, and sections were developed with DAB for desired time and counterstained with hematoxylin and/or eosin. Slides were mounted in Permount Mounting Medium.
Approximately 75 mg mouse corpus stomach or pancreas tissue were sonicated in RIPA buffer with 1× protease inhibitor cocktail (Thermo). Protein was separated using NuPAGE 10% Bis-Tris gels and transferred to an Invitrogen nitrocellulose membrane. Membranes were then blocked with 3% bovine serum albumin (BSA) and incubated overnight at 4°C with primary antibodies (see Reagent Table for antibodies). The membranes were rinsed in Tris-buffered saline (TBS) pH 8.0, incubated 1 hour at room temperature in secondary antibody in 5% low-fat milk. Actin antibody was used as a control to ensure equal loading of protein in each gel lane. Secondary antibody signals were imaged and detected by SuperSignal West Pico PLUS Chemiluminescent Substrate Kit.
Imaging and quantifications
Fluorescence microscopy was performed using a Zeiss Axiovert 200 microscope with an Axiocam MRM camera and Apotome II instrument for grid-based optical sectioning. Post-imaging adjustments, including contrast, fluorescent channel overlay, and pseudocoloring, were performed with AxioVision and Adobe Photoshop CS6. Histology of stomach and immunohistochemistry were imaged using an Olympus BX51 light microscope and Olympus SZX12 dissecting microscope w/12 MPixel Olympus DP70 camera. Images were analyzed, and post-imaging adjustments were performed with Adobe Photoshop CS6.
Quantification of BrdU proliferation rates was done by counting 5 or more 20× fields from a whole-slide scanned images from the Hamamatsu NanoZoomer 2.0-HT system.
FIB-SEM 3D Nanotomography
FIB-SEM 3D nanotomography was performed as described in ref. Lo et al (2017). Mouse gastric tissues were bisected into fixative containing 2.5% glutaraldehyde and 2% paraformaldehyde in 0.15 M cacodylate buffer containing 2 mM CaCl2 (pH 7.4), fixed for 15 min at 37°C and then overnight at 4°C, sliced into ∼1.5-mm-thick pieces, rinsed in cacodylate buffer for 10 min at room temperature, and subjected to secondary fixation in 1% osmium tetroxide/0.3% potassium ferrocyanide in cacodylate buffer for 1 h on ice. The samples were then washed in ultrapure water and stained en bloc in 2% aqueous uranyl acetate for 1 h. After staining, samples were briefly washed in ultrapure water, dehydrated in a graded acetone series, and infiltrated with microwave assistance (Pelco BioWave Pro) into LX112 resin, which was cured in an oven for 48 h at 60°C. Cured blocks were trimmed and mounted onto SEM pins with silver epoxy and faced with a diamond knife. Toluidine blue-stained sections (300 nm thick) were used to locate a region of interest. Blocks were sputter-coated with 10 nm of iridium (Leica, ACE 600) with rotation on a planetary stage to ensure saturation. Regions of interest on a FIB-SEM (Zeiss, Crossbeam 540) were located by secondary electron imaging at 10 KeV. Once a region was found, the sample was prepared using the ATLAS (Fibics) 3D nanotomography engine. In short, a platinum pad was deposited on a 40-µm × 40-µm region of interest with the FIB set to 30 KeV and 1.5 nA. Three vertical lines for focus and sigmation and two angled lines for z-tracking were milled into the platinum pad at 50 pA, and a protective pad of carbon was deposited on top of the milled platinum at 1.5 nA. Following this, a rough trench 50 µm wide and 55 µm deep was milled at 30 nA and polished at 7 nA. Once polishing of the block face was complete, face detection, focusing, and z-tracking were all performed on the fiducial marks that were milled into the platinum pad. Imaging was performed at 2 KeV and 1.1 nA using the EsB (energy selective backscatter) detector with a grid voltage of 1100 V. The block was milled at a current of 700 pA with 20 nm slices, and 2,000 × 1,750 pixel images were acquired at a resolution of 20 nm/pixel with a dwell of 8 or 10 µs and a line average of 3 for a total z-depth of 35 µm.
3D reconstruction was performed as described in ref. Lo et al (2017). All EM serial images were imported into the Amira 6 3D software package for 3D reconstruction. Areas of interest were manually segmented into data objects with intervening unsegmented slices (“X”) based on object volume. For organelles with suboptimal contrast, the thresholding function was used for manual segmentation. The interpolation function was used to highlight areas of interest between manually segmented slices. 3D models were generated from labeled objects. The “Smooth” and “Simplify” functions were used for model generation, and pseudocoloring was used to enhance visualization for each organelle. Animations were created with the Animation Director in the software.
For TEM, stomachs were fixed, sectioned, stained, and imaged as previously described (Willet et al, 2018). Briefly, tissue was collected as described above, fixed overnight at 4°C in modified Karnovsky’s fixative, and sectioned. Tissue was processed by the Washington University in St. Louis Department of Pathology and Immunology Electron Microscopy Facility.
Human cancer cell culture
AGS cells (ATCC) were grown under standard conditions (Advanced DMEM/F12, 10% FBS, Nonessential amino acids, and Pen/Strep at 37°C and 5% CO2) and were cotransfected with a transposon expressing shRNA against ATF3 (TRCN0000329691) under a U6 promoter as well as a homemade plasmid expressing hyperactive PiggyBac transposase to generate stable incorporation of the vector into the genome. After selection with puromycin, passaged cells were obtained for experiments within the first 10 passages. To generate ATF3 overexpression lines, the human ATF3 sequence was cloned from Addgene #26115 and inserted into a homemade PiggyBac transposon vector for overexpression.
Following selection of stable ATF3 overexpression or ATF3 knockdown constructs, the cells were transfected with transposons containing either wild-type or T22N point mutant of RAB7B containing an N-terminal 3x-FlagTag. RAB7B template was purchased from OriGene (Catalog #RC202283), and the mutant was generated by amplifying a truncated C-terminal domain and a three-part ligation using oligos encoding the mutant N-terminal domain. All sequences were confirmed by Sanger sequencing services provided by Genewiz. Two days after transfection with RAB7B constructs, the cells were fixed and stained with an anti-FLAG antibody, which permitted specific identification of those doubly transfected cells and to determine the cellular localization of mutated RAB7BT22N.
For immunofluorescence experiments, cells were grown on coverslips and blocking and staining was completed in 12-well culture plates. For imaging, the coverslips were mounted onto slides with ProLong Gold Antifade Mountant with 4′6-diamidino-2-phenylindole (DAPI) (Molecular Probes).
RNA was isolated using RNeasy (Qiagen) per the manufacturer’s protocol. The integrity of the mRNA was verified with a BioTek Take3 spectrophotometer and electrophoresis on a 2% agarose gel. RNA was treated with DNase I (Invitrogen), and 1 µg of RNA was reverse-transcribed with SuperScript III (Invitrogen) following the manufacture’s protocol. Measurements of cDNA abundance were performed by qRT–PCR using Applied Biosystems QuantStudio 3 Real-time PCR system. Power SYBR Green master mix (Thermo Scientific) fluorescence was used to quantify the relative amplicon amounts of each gene. Primer sequences are located in Table EV1.
Approximately 25 mg of stomach corpus tissue was flash-frozen in liquid nitrogen until IP was performed. The SimpleChIP Plus Enzymatic Chromatic IP Kit (Cell Signaling Technology) was used for tissue prep and IP per the manufacturer’s protocol (see Reagent table for antibody concentrations). Tissue was fixed with PFA for 20 min and disaggregated with a Medimachine (BD Biosciences). Standard PCR was used to determine ATF3 binding at the Rab7b first intron (see Table EV2 for primer sequences).
Human patient samples
Human gastric pathological tissue specimens were obtained with approval by the Institutional Review Board of Washington University School of Medicine. Samples used are deidentified tissues archived from standard-of-care procedures. Informed consent was received from all patients for the use of their tissue and experiments conformed to the principles set out in the WMA Declaration of Helsinki and the Department of Health and Human Services Belmont Report. Our research team does not have contact with patients and patient information is deidentified. All specimens are stored behind double-locked doors, and only approved members of the research team have access. Gastric clinical samples have been previously described in Ref. Lennerz et al (2010), Capoccia et al (2013), Radyk et al (2018), Willet et al (2018).
Graphing and statistical analysis
Graphs and statistics were done with GraphPad Prism (La Jolla, CA). In cases involving more than two samples to compare, significance was determined using ANOVA with post-hoc correction: Tukey was used to assess statistical significance if multiple conditions were compared; Dunnett post-hoc when comparing multiple samples to a single control. Otherwise, unpaired, two-tailed Student’s t-test was used to determine significance. Data that would violate normalcy by study design were analyzed by nonparametric Mann–Whitney U-test. Most data (e.g., cell counts) were first analyzed as mean values of measurements from multiple fields across multiple sections of an organ for each animal, and then, the mean of those means was plotted. A P-value of ≤ 0.05 was considered significant. Samples were randomized, and measurements were blinded to prevent the introduction of experimental bias. Formal tests for normalcy were not performed. At least the minimum numbers of animals are used to achieve statistical significance in any determinations.
This study includes no data deposited in external repositories.
We thank Dr. Tsonwin Hai at the Ohio State University for the Atf3−/− mice. We thank Karen Green, Lisa Snipes, and Kevin Boyer of the Department of Pathology Electron Microscopy Center. We acknowledge the AITAC of the Washington University Digestive Disease Center (DDRCC: P30 DK052574) and the NIH Shared Instrumentation Grant S10RR0227552 (for NanoZoomer slide scanning). FIB-SEM nanotomography was performed in the Washington University Center for Cellular Imaging (WUCCI), which is funded, in part, by the Children’s Discovery Institute of Washington University and St. Louis Children’s Hospital (CDI-CORE-2015-505 and CDI-CORE-2019-813), the Foundation for Barnes-Jewish Hospital (3770), and Siteman Cancer Center (P30CA091842). MDR was funded by F31CA236506-01 (NIH NCI), the Philip and Sima Needleman Student Fellowship in Regenerative Medicine, and 5T32GM007067-43 (NIH); LBS was supported by Siteman Cancer Center Cancer Pathway Program (P30 CA091842 and T32CA113275). BLP by Washington University Biology Summer Undergraduate Research Fellowship Program (BioSURF) and the Children’s Discovery Institute of Washington University and St. Louis Children’s Hospital; JWB was supported by the Department of Defense, through the PRCRP program under Award No. W81XWH2010630 (USAMRAA), T32-DK007130 (NIH NIDDK), the Digestive Disease Research Core Centers Pilot and Feasibility Grant as part of P30 DK05257, NIH R21 AI156236, and the American Gastroenterological Association AGA2021-5101; J.B. was supported by National Institutes of Health (NIH) training grant (GM007067) and the Philip and Sima Needleman Student Fellowship in Regenerative Medicine; CJC by T32-CA009547 (NIH NCI); JCM by the National Institute of Diabetes and Digestive and Kidney Diseases (R21 DK111369, R01DK094989, R01DK105129, R01DK110406 R01120680), The National Institutes of Health National Cancer Institute (P30 CA09182, R01 CA239645, R01 CA246208), and the BETRNet (U54 CA163060).
MDR designed and performed experiments, analyzed and interpreted data, performed statistical analyses, and drafted and revised the manuscript; LBS and BLP designed and performed experiments, analyzed and interpreted data, performed statistical analyses, and drafted the manuscript; JWB, JB, CJC, and YK designed and performed experiments. C-CS and JAJF designed the experiments. JCM designed the experiments, provided funding for the study, generated data, performed bioinformatics analyses, and drafted and revised the manuscript.
Conflict of interest
The authors declare that they have no conflict of interest.
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