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Autophagy is an evolutionarily conserved process that degrades cellular components to restore energy homeostasis under limited nutrient conditions. How this starvation-induced autophagy is regulated at the whole-body level is not fully understood. Here, we show that the tumor suppressor Lkb1, which activates the key energy sensor AMPK, also regulates starvation-induced autophagy at the organismal level. Lkb1-deficient zebrafish larvae fail to activate autophagy in response to nutrient restriction upon yolk termination, shown by reduced levels of the autophagy-activating proteins Atg5, Lc3-II and Becn1, and aberrant accumulation of the cargo receptor and autophagy substrate p62. We demonstrate that the autophagy defect in lkb1 mutants can be partially rescued by inhibiting mTOR signaling but not by inhibiting the PI3K pathway. Interestingly, mTOR-independent activation of autophagy restores degradation of the aberrantly accumulated p62 in lkb1 mutants and prolongs their survival. Our data uncover a novel critical role for Lkb1 in regulating starvation-induced autophagy at the organismal level, providing mechanistic insight into metabolic adaptation during development.
Autophagy is a highly conserved, multi-step intracellular process of self-degradation. Under basal conditions, autophagy eliminates damaged proteins and organelles from cells, serving a housekeeping/recycling function. However, upon metabolic stress, starvation–induced autophagy serves to provide substrates for biosynthesis and energy production in order to maintain cellular homeostasis1, 2. The importance of autophagy for cellular and organismal health is showcased by the fact that defects in autophagy have been linked to neurodegeneration, cancer, aging and metabolic syndrome1.
Starvation-induced autophagy promotes survival in the Drosophila fat body3 and in Caenorhabditis elegans 4. A critical role for autophagy in surviving the metabolic stress at birth has also been demonstrated in mammals: mice deficient in Atg5 (autophagy protein 5, an E3 ubiquitin ligase necessary for autophagosomal elongation) survive foetal development, but die within one day after birth, exhibiting severe hypoglycaemia and hypolipidaemia2. However, the regulation of systemic starvation-induced autophagy is not well understood.
Autophagy-induction in response to energetic stress is triggered by the activation of AMPK-activated protein kinase (AMPK)5, 6, a key, evolutionarily conserved energy sensor. AMPK activation restores energy homeostasis at the cellular and organismal levels7 by many different pathways, including via inhibition of the mechanistic target of rapamycin (mTOR)8, a conserved serine-threonine kinase involved in nutrient sensing, growth and proliferation9, 10. AMPK itself is activated by multiple mechanisms including phosphorylation by the tumor suppressor LKB1/STK11 kinase in response to increased AMP or ADP levels in the cell11, 12. Because of the role of AMPK as a central energy checkpoint in the cell, these findings link LKB1 signaling to energy metabolism control, positioning LKB1 as a critical mediator of the effects of low energy on cell viability11, 13. Accordingly, cells lacking LKB1 undergo apoptosis under metabolic stress as they are unable to respond to energy deficiency and restore homeostasis11. LKB1/AMPK signaling is also important for long-term survival under nutrient-limiting conditions during C. elegans dauer (diapause) stage14. However, the early embryonic lethality of both Lkb1 mutant15 and Ampka1/a2 double mutant mice16 has precluded analysis of the in vivo role of LKB1/AMPK in physiological processes occurring at later developmental stages in vertebrates, such as during metabolic stress at birth.
The LKB1/AMPK axis is a negative regulator of mTOR signaling8 and mTOR signaling is a known inhibitor of autophagy17. However, LKB1 also activates 12 other AMPK-related kinases18, and many mTOR-dependent and mTOR-independent autophagy regulators exist19.
LKB1/AMPK regulation of mTOR has been linked to the regulation of autophagy in different settings, for example in autophagy stimulated by fluid flow over the primary cilium of epithelial cells20, and in cancer cells21. Furthermore, AMPK directly stimulates autophagy via the ULK1/Atg1 phosphorylation22, 23. And LKB1 may also stimulate autophagy by stabilizing p27, thereby linking nutrient sensing to cell-cycle progression13. However, whether and how LKB1 signaling regulates systemic starvation-induced autophagy in vertebrates is currently unknown.
The regulation of systemic metabolism and autophagy are often studied in zebrafish because of its small size and vertebrate physiology24, 25. Importantly, fundamental principles of energy homeostasis are highly conserved between humans and zebrafish26, 27. Autophagy has critical functions during zebrafish embryonic development28, with autophagy-defective animals displaying abnormal heart development29, which is also seen in mice30. Zebrafish are also a valuable model for studying tissue regeneration, and autophagy has been shown to be required for the regeneration of amputated caudal fins31. Like mammals, zebrafish also experience metabolic stress at birth, when the maternal nutrient supply (yolk) is depleted. The metabolic stress at birth in mammals is accompanied by induction of gluconeogenesis32, 33 and of autophagy2, 34. While induction of gluconeogenesis also serves as a mechanism to restore energy homeostasis in zebrafish35, a role for autophagy during this metabolic transition has not been investigated.
We previously used TILLING36 to generate zebrafish mutants that carried a point mutation leading to a stop codon in the kinase domain of Lkb1 (stk11 hu1968). These mutants survived gastrulation and early embryonic development but died prematurely from starvation at 7 to 8 days post-fertilization (dpf). Our experiments, impossible to conduct in mice due to the early embryonic lethality of Lkb1 knock-out mice15, established Lkb1 as a critical regulator of whole-body energy homeostasis37. Zebrafish lkb1 (stk11 hu1968) mutants are unable to cope with the energetic stress induced upon yolk depletion and fail to adapt their metabolism to lower nutrient levels. lkb1 mutants are indistinguishable from wild type (wt) siblings while their maternal nutrient supply is still present, until 5–6 dpf. However, they die within 1–2 days following yolk depletion whereas wt larvae can survive without food until 13–14 dpf38.
The zebrafish lkb1 mutant phenotype is reminiscent of the Atg5 knock-out mice that appear normal until birth but die soon after, due to their inability to cope with the metabolic stress at birth2. This resemblance prompted us to investigate the autophagy status in the lkb1 mutants to study the role of Lkb1 in regulation of systemic starvation-induced autophagy.
We show that Lkb1-deficient larvae fail to activate autophagy in response to nutrient restriction. Furthermore, we demonstrate aberrant accumulation of the autophagy adaptor and substrate p62 in lkb1 mutants, confirming impaired autophagy. Genetic or chemical induction of autophagy in lkb1 mutants prolongs their survival, while suppression of autophagy shortens it. Survival prolongation only occurs when degradation of p62 is restored. We therefore show that autophagy is essential to survive the feeding-fasting transition in zebrafish, and identify Lkb1 as a critical regulator of whole-body starvation-induced autophagy in vertebrates.
To determine if autophagy initiation and maintenance is affected in the lkb1 mutants we previously generated37, we analyzed wt and lkb1 larvae between 5–7 dpf during the metabolic transition following yolk depletion. lkb1 mutants are indistinguishable from wt larvae up to day 5–6 dpf37 (while there is still yolk). We chose this time window also because the morphological lkb1 phenotype of flattened intestine and darkened liver is apparent at 7 dpf37 and the majority of lkb1 mutants die at 8 dpf (Supplementary Fig. S1). Autophagic activity is commonly monitored by accumulation of the membrane-bound form of MAP1LC3B (microtubule-associated proteins 1A/1B light chain 3B, Atg8 in yeast; Lc3B in zebrafish), Lc3-II, which is a ubiquitin-like protein39 that localizes in autophagosomal membranes upon induction of autophagy. To enable visualization of Lc3-II accumulation in autophagosomes, we first blocked the fusion of autophagosomes with lysosomes by treating the larvae with 2.5μM chloroquine40 for 14 hours (h) before analysis.
We found that Lc3-II protein levels were lower in lkb1 mutant larvae compared to their wt siblings after yolk depletion at 6 and 7 dpf (Fig. 1A). Note that the Lc3 antibody in zebrafish recognizes predominantly the cleaved Lc3B-II form, which still accurately reflects autophagic activity41 (Supplementary Fig. S2A), and we were only able to detect a faint signal for Lc3B-I in zebrafish lysates (Fig. 1A). To verify this result, we used an alternative marker of autophagy by analyzing the expression of Atg5-containing protein complexes during development. We found that while the expression of the common ~56 KD complex was unaffected, the ~47 KD complex, which is indicative of autophagy induction31 was undetectable in the lkb1 mutants (Fig. 1A). Finally, we also assessed the levels of Beclin 1 (Becn1), a protein involved in autophagosome nucleation30, 42 and also commonly used as an autophagy indicator. Becn1 expression was also strongly reduced in the lkb1 mutants (Supplementary Fig. S2B). While Lc3-II and Becn1 levels progressively increased in wt larvae between 5–7 dpf, indicating upregulation of autophagy upon yolk termination, lkb1 mutants did not show such an increase, suggesting they fail to activate autophagy under nutrient limiting conditions (Fig. 1A, and Supplementary Fig. S2B).
To examine the spatial distribution of autophagy, we performed immunofluorescence analysis with antibodies against Lc3B on transverse liver and intestine sections of lkb1 and wt larvae at 7 dpf. Lc3B expression was strongly reduced in lkb1 intestines and livers as compared to their wt counterparts (Fig. 1B–E and Supplementary Fig. S2E,F), confirming and supporting the immunoblotting results. Furthermore, immunohistochemistry (IHC) against Becn1 on transverse sections of wt and lkb1 mutants showed markedly reduced Becn1 staining in the lkb1 mutants compared to their wt counterparts (Supplementary Fig. S2C,D).
To further confirm that activation of autophagy is impaired in lkb1 mutants, we monitored expression levels of the p62 protein (also known as sequestosome 1, (SQSTM1). p62 is an adaptor protein that targets ubiquitinated proteins or organelles that bind to it for selective autophagy43. Accumulation of p62 has been observed in mouse AMPK-deficient fibroblasts44, and is associated with liver toxicity in autophagy-deficient mouse liver45. p62 itself is also an autophagy substrate, thus accumulation of p62 levels is a marker for impaired autophagy46. In agreement with our model that lkb1 mutants have impaired autophagy, Western blot analysis of p62 levels at 5, 6 and 7 dpf showed progressive accumulation of p62 specifically in the lkb1 mutants (Fig. 1A). IHC performed on transverse sections of lkb1 intestine and liver confirmed a marked accumulation of p62 in lkb1 larvae, whereas wt siblings were devoid of staining (Fig. 1F,G).
Collectively, these findings demonstrate that whole-body autophagy is impaired in lkb1 mutants during the feeding-fasting transition in zebrafish, which could contribute to their premature death.
To investigate the effect of inhibiting autophagy on lkb1 larvae survival prior to yolk depletion, we blocked autophagosome formation using an antisense morpholino oligonucleotide (MO), that targets the translational start-site of atg5 mRNA28, 47, atg5MO. We confirmed that injection of atg5MO abolishes Atg5 protein expression (Supplementary Fig. S3). Atg5-knockdown led to a reduction in Lc3-II levels compared to the negative control in both wt and lkb1 mutants at 4 dpf, before yolk depletion, confirming autophagy suppression upon atg5MO injection (Fig. 2A). While all un-injected wt and lkb1 larvae were alive at 4 dpf, a significant number of atg5MO-injected embryos were found dead at that time point. Genotyping all larvae at 4 dpf revealed that 75% of atg5MO-injected lkb1 larvae had died compared to only 25% of atg5MO-injected wt larvae (Fig. 2B). Thus, lkb1 mutants, which fail to induce autophagy at the metabolic transition, are also more sensitive to autophagy inhibition at earlier embryonic stages.
We next investigated the mechanism behind the impaired autophagy observed in the lkb1 mutants. Signaling through mTOR is known to inhibit autophagy, and we and others have previously reported that mTOR activity is high in wt larvae between 2 and 5 dpf and is downregulated at later stages of larval development37, 47, 48. This suggests that at the time of yolk depletion, mTOR activity is switched off, enabling the activation of autophagy. It has also been shown in mice that suppression of mTOR activity at birth enables activation of autophagy49. We hypothesized that mTOR inactivation was defective in the absence of Lkb1. Therefore, we first assessed the status of mTOR signaling in lkb1 mutants at the metabolic transition (6 dpf) by analyzing phosphorylation of the mTOR-substrate ribosomal protein S6 (RS6) by Western blot. Total RS6 levels were almost undetectable in wt larvae at this stage, consistent with our previous report37. However, both total and phospho- RS6 levels were high in lkb1 mutants (Fig. 3A), indicating active mTOR signaling, which was inhibited by rapamycin treatment. In comparison, in rapamycin-treated 6 dpf wt larvae, we observed increased phospho-RS6 expression (Fig. 3A). This could be explained by a known developmental delay caused by chronic mTOR inhibition during development50. Consistent with this, rapamycin-treated wt larvae retained significant amounts of yolk at 7 dpf, demonstrating a delay in larval development (Supplementary Fig. S4C).
To determine whether mTOR signaling mediates the inhibition of autophagy seen in the lkb1 mutants at 6 dpf, we examined whether rapamycin treatment could restore autophagy in these mutants. We treated wt and lkb1 embryos with rapamycin from 1 dpf onwards. We have previously reported that rapamycin-treated lkb1 larvae survive until 9 dpf, but still have a considerable amount of yolk, demonstrating a developmental delay37. Rapamycin-treatment resulted in elevated Lc3-II levels in both wt and lkb1 larvae, at 6 dpf (Fig. 3B), indicating that autophagy in the lkb1 mutants is inhibited, at least in part, by mTOR signaling. The same was also observed when blocking autophagosome-lysosome fusion by chloroquine, which prevents degradation of autophagosome-associated Lc3, allowing monitoring of the autophagic flux51 (Supplementary Fig. S4A,B). However, rapamycin-treatment led to only slight upregulation of Atg5 and complexed Atg5 in lkb1 mutants (Fig. 3C), and was not sufficient to decrease the marked p62 accumulation (Fig. 3B). These results suggest that while mTOR inhibition can at least partially restore autophagy in lkb1 mutant larvae, it cannot entirely alleviate the observed phenotype.
We next analyzed the pro-survival PI3K pathway, which in response to external stimuli (growth factors, insulin) also suppresses autophagy, acting upstream of mTOR signaling52. To this end, we used the small molecule AR-12, an inhibitor of phosphoinositide-dependent kinase (PDK)-1, a component of the PI3K pathway53, which has been shown to activate autophagy in zebrafish54. Treatment of wt and lkb1 siblings with AR-12 from 1 dpf onwards, led to accumulation of Lc3-II protein levels in wt but not in lkb1 larvae at 6 dpf (Fig. 4A). Interestingly, AR-12 treatment resulted in upregulation of Atg5 expression and formation of Atg5/12 complexes in wt larvae indicating autophagy induction, but no changes in Atg5 expression were observed in lkb1 larvae (Fig. 4B). Furthermore, while p62 protein expression was diminished in wt larvae upon AR-12-mediated activation of autophagy, accumulation of p62 remained unchanged in AR-12-treated lkb1 larvae (Fig. 4A). This indicates that inhibition of the PI3K pathway fails to induce autophagy in mutant larvae. We next assessed phosphorylation of the mTOR-substrate RS6 upon AR-12 treatment in wt and lkb1 larvae at 6 dpf. RS6 and phosphorylated RS6 (P-RS6) were not detectable in wt larvae at 6 dpf (Fig. 4C), consistent with downregulation of mTOR activity at later developmental stages (here and refs 37, 47 and 48). AR-12 treatment did not affect the high protein levels of RS6 or P-RS6 seen in the lkb1 mutants, indicating that they are unsusceptible to PI3K pathway inhibition. In line with the lack of autophagy induction, AR-12 treatment did not enhance lkb1 survival, as no statistically significant differences were observed in the percentage of AR-12-treated lkb1 larvae alive at 9 dpf compared to DMSO-treated controls (Fig. 4D).
Activation of autophagy by an mTOR-independent pathway can be achieved using calpeptin, which inhibits the autophagy inhibitors calpain proteases55. Calpeptin treatment of lkb1 and wt embryos from 1 dpf onwards, in the presence or absence of chloroquine, enhanced Lc3-II levels in both wt and lkb1 larvae at 6 dpf (Fig. 5A and Supplementary Fig. S5) without any effects on development or yolk absorption. Calpeptin treatment also resulted in upregulation of the amounts of Atg5 and complexed-Atg5 in both wt and lkb1 mutants (Fig. 5B). In contrast to rapamycin treatment, treatment with calpeptin restored p62 degradation in lkb1 mutants (Fig. 5A). Calpeptin treatment had no effect on RS6 phosphorylation in lkb1 mutants (Fig. 5C), consistent with calpeptin being an mTOR-independent autophagy activator55. Moreover, calpeptin-mediated activation of autophagy prolonged survival in 70% of the treated lkb1 larvae. Specifically, 17.5% of calpeptin-treated lkb1 larvae survived until 9 dpf, whereas only 1% of vehicle-treated lkb1 larvae were alive at this point (Fig. 5D). Therefore, we conclude that induction of mTOR-independent autophagy results in a more complete restoration of the lkb1 mutant phenotypes compared to that obtained upon inhibition of mTOR signaling.
Aberrant p62 accumulation appeared as a hallmark of impaired autophagy in lkb1 mutants, and strongly correlated with survival. While p62 is primarily thought of as a receptor delivering cargo proteins to autophagosomes for degradation, it has also been implicated in enhancing mTOR activity56, thereby regulating autophagy as well. Loss of p62 function led to increased autophagy in mammalian cells and in C. elegans 56. We thus set out to determine whether reducing p62 levels in larvae would affect autophagy and survival. To this end, we injected a sqstm1/p62 MO, targeting splicing of sqstm1/p62 mRNA54, into 1–2-cell stage embryos. RT-PCR confirmed that the sqstm1/p62 MO blocked sqstm1/p62 mRNA splicing until at least 5 dpf (Supplementary Fig. S6). Western blot analysis of 6 dpf larvae showed decreased p62 expression compared to un-injected controls in both wt and lkb1 lysates (Fig. 6A). This was coupled with increased Lc3-II protein levels, suggestive of autophagy induction. Knockdown of p62 significantly prolonged lkb1 survival up to 9 dpf: Approximately 70% of sqstm1/p62 MO-injected lkb1 mutants survived to 9 dpf, whereas less than 5% of un-injected lkb1 larvae were alive at this time-point (Fig. 6B). Thus, depleting p62 is sufficient to activate impaired autophagy in lkb1 mutants and extend survival.
Organisms adapt their metabolism in response to nutrient limitation to restore energy homeostasis and ensure survival. Here, we identify a novel link between metabolic adaptation during development and induction and maintenance of autophagy, mediated by the tumor suppressor Lkb1. Specifically, we use metabolically compromised Lkb1-deficient zebrafish larvae to show that Lkb1 is crucial in the induction of autophagy in response to the metabolic challenge accompanying depletion of the maternal nutrient supply. Our data therefore reveal an essential function for Lkb1 in controlling starvation-induced autophagy at the organismal level in vertebrates.
Overall autophagy levels in lkb1 mutants are lower compared to those of wt siblings: while expression of autophagy–related proteins is progressively upregulated following yolk depletion in wt larvae, induction of autophagy in lkb1 mutants is strongly attenuated. Importantly, we demonstrate that genetic and chemical manipulation of autophagy levels significantly impacts lkb1 larvae survival: inducing autophagy by mTOR-dependent and –independent mechanisms prolongs survival, and suppressing autophagy by Atg5 depletion leads to premature death selectively of the mutants. The increased susceptibility of lkb1 larvae to Atg5 depletion during development occurred even while the yolk is not yet consumed, suggesting that even though the larvae do not show a morphological phenotype at this embryonic stage, the loss of Lkb1 appears to sensitize them to additional stress. This stress may be specifically autophagy inhibition, or related to alternative mechanisms, as autophagy-independent functions have been reported for several of the autophagy-related genes57, 58, including Atg559.
Various mechanisms, including mTOR and PI3K signaling, as well as calpains, are known to regulate autophagy19, and likely interact at multiple levels. Indeed, our results, together with published work, indicate that all these influence the energy-sensing defect we observe in lkb1 mutants. We show that activating autophagy by calpeptin, which inhibits the action of the general autophagy inhibitors calpains55, led to robust upregulation of Atg5 expression and restored degradation of p62 in lkb1 mutants. Thus, calpeptin fully rescued the autophagy defect of the lkb1 larvae and prolonged their survival. In contrast, while the mTOR-inhibitor rapamycin increased Lc3-II accumulation in lkb1 larvae, autophagy was not completely restored since p62 still accumulated. This may be due to the high mTOR activity in the mutants that could not be fully blocked by rapamycin treatment under these experimental conditions. In addition, although rapamycin treatment also prolonged lkb1 survival, we believe this was likely due to a generalized growth delay, evidenced by the presence of a considerable amount of yolk at 7 dpf (this study and refs 37 and 50), rather than due to partial restoration of autophagy. A developmental delay caused by rapamycin is further supported by the persistence of RS6 expression in rapamycin-treated wt larvae at 7 dpf when mTOR would normally be suppressed (mTOR signaling is suppressed in wt larvae upon yolk depletion at 5–6 dpf37, 47, 48).
The autophagy receptor and substrate p62 aberrantly accumulates in lkb1 mutants indicating deficient autophagy. p62 is also a regulator of autophagy, as it participates in a feed-forward loop in which p62 enhances mTOR activity resulting in reduced autophagy, in turn leading to higher p62 levels in mice60. Here we also show that depletion of p62 in lkb1 larvae leads to activation of autophagy and prolonged survival. This implies that as the amount of p62 decreases due to autophagosomal clearance, its effect on mTOR activity is also reduced, and thus autophagy can be maintained. Furthermore, the aberrant accumulation of p62 in lkb1 larvae may in itself contribute to their premature lethality, as it has been shown that increased levels of p62 in autophagy-deficient mouse livers cause hepatotoxicity (reviewed in ref. 60). Further supporting our hypothesis, in apoptosis-impaired tumor cells with deficient autophagy, p62 accumulation triggers a positive feedback loop for the generation of reactive oxygen species (ROS) leading to enhanced genomic instability and tumorigenesis61.
PI3K signaling is a nutrient-sensing pathway that is also implicated in starvation-induced autophagy. Inhibition of the PI3K pathway activated autophagy in wt larvae, but not in lkb1 mutants, and did not prolong their survival. This is consistent with our previous findings that PI3K signaling is compromised in lkb1 mutants37. We postulate that defective PI3K signaling may contribute to the autophagy defect seen in these mutants. While AMPK is considered a major regulator of metabolism and has an important role in induction of autophagy under energetic stress23, 44, it is not overtly activated in wt larvae at 7 dpf37; in agreement with these data, studies in mice have also reported that 24hours of fasting did not lead to significant AMPK activation62, 63. Thus, the autophagy defect we describe in lkb1 mutants is unlikely to be solely attributable to impaired AMPK signaling, and deregulation of additional pathways, such as PI3K signaling and AMPK/mTOR-independent pathways may also be involved. Hence, nutrient-sensing pathways (like the PI3K pathway) and energy-sensing pathways (like the AMPK pathway) are likely in close cross-talk with each other, not only through their convergence on mTOR signaling but also through different, mTOR-independent mechanisms.
Together, our data indicate that Lkb1 plays an important role in the regulation of autophagy at the whole-organism level, and confirm that autophagy is critical for survival during the metabolic transition in development. Since defects in autophagy are implicated in a plethora of diseases, a better understanding of the upstream regulatory pathways could provide new insights into their pathophysiology.
Zebrafish were handled in compliance with the local animal welfare regulations and were maintained according to standard protocols (zfin.org). Their culture was approved by the local animal welfare committee (DEC) of the University of Leiden and all protocols adhered to the international guidelines specified by the EU Animal Protection Directive 2010/63/EU. Genotype analysis for lkb1 mutants embryos was performed as previously described37.
Larvae obtained from single matings of heterozygous lkb1 adults were analyzed over time. 48–95 larvae were genotyped on 6, 7, 8, 9, 10 and 11 dpf to assess the numbers of lkb1 mutants alive.
Approximately 20 larvae/sample were lysed (3μl per larva) in cold lysis buffer (50mM Hepes, pH 7.6, 50mM KCl, 50mM NaF, 5mM NaPPi, 1mM EGTA, 1mM EDTA, 1mM beta-Glycerophosphate, 1mM DTT, 1mM Vanadate, 1% NP40) containing phosphatase and proteinase inhibitors. Lysates were pestled for 5min, sonicated for 30seconds at 30seconds intervals for 5min and centrifuged at 13.000rpm for 15min at 4°C to pellet nuclei and cell debris. Protein lysates were boiled for 10min and BCA assay was performed to measure protein concentration. Samples containing 12–30μg of protein were heated at 95°C for 5min with 4× Bolt LDS sample buffer (Thermofisher, #B0007), supplemented with 5% beta-mercaptoethanol, and loaded onto a 12% Bis-Tris plus gel (Thermofisher, #NW00122). The protein marker used was Precision Plus ProteinTM Dual Color Standards, #1610374 (BioRad). Proteins were transferred onto a nitrocellulose membrane (Thermofisher, #88018) using a wet transfer system (Bio-Rad) according to manufacturer’s instructions. Subsequent blocking and antibody incubation were performed in 5% skimmed milk powder (#115363, Merck Millipore) in PBS containing 0.1% Tween-20. For the anti-p62 antibody, blocking was performed in 10% milk powder and antibody incubation in 1% milk powder in PBS containing 0.1% Tween-20. Antibodies used were: rabbit anti-LC3B (1:1000, Abcam, #ab51520), rabbit anti-p62 (1:1000, MBL, #PM045), rabbit anti-BECN1 (1:500, Santa Cruz, #sc-11427), rabbit anti-H3 (1:5000, Santa Cruz, #sc-10809), mouse anti-beta-actin (1:5000, Sigma, #A5441), mouse anti-Tubulin (1:500, Sigma, #T9026), rabbit anti-Atg5 (1:500, Novus, #NB110-53818). Secondary antibodies used were goat Anti-Mouse IgG (H+L)-HRP (1:10.000, BioRad, #1721011) and Goat Anti-Rabbit IgG (H+L)-HRP Conjugate (1:10.000, BioRad, #17210191). Membranes were developed using ECL (BioRad, #1705060), followed by chemiluminescence detection with a gel doc system (BioRad).
For transverse sections, larvae were fixed in 40% ethanol, 5% acetic acid and 10% formalin for 3h at room temperature followed by three washes in 70% ethanol before being dehydrated following serial washes in Histoclear and reducing ethanol concentrations. Larvae were then sectioned at 5 μm intervals using a Reichert-Jung 2050 microtome (Leica). Sections were deparaffinized and hydrated following by 20min of antigen retrieval in sodium citrate buffer pH 6.0 at 100°C. Sections were blocked in 5% BSA in PBS−0.1% Tween-20 for 1h at room temperature and incubated overnight with sheep anti-p62 (1:200, Abcam, #ab31545) and rabbit anti-BECN1 (1:150, Santa Cruz, #sc-11427). Endogenous peroxidase activity was blocked in 0.3% H2O2 for 20min at room temperature followed by incubation with rabbit anti-sheep antibody (1:800, Abcam, #ab6747) for 1h at room temperature. Sections were incubated with 0.1M imidazole prior to detection with 3,3′-diaminobenzidine (DAB) substrate and counterstaining with hematoxylin.
For immunofluorescence, larvae were fixed in 4% PFA overnight at 4°C, embedded vertically in a 0.5% gelatin/30% albumin mixture and sectioned at 120 μm intervals using a VT1000S vibratome (Leica). Sections were transferred to the wells of a 24-well plate containing PBD (PBS+0.1% Tween-20 and 0.5% Triton-X-100), which was then replaced with blocking solution (PBD+1% BSA) for 1h at RT. Sections were incubated with rabbit anti-LC3B (1:1000, Abcam, #ab51520) in blocking solution overnight at 4°C. Sections were washed three times for 15min in PBS-0.1% Tween-20 and incubated with secondary anti-rabbit 488 green fluorescent antibody (1:100, Thermofisher, #A11008) for 2h at room temperature. Sections were then washed three times for 15min in PBS-0.1% Tween-20 prior to be incubated with phalloidin-Alexa 588 (1:25, Thermofisher, #A12380) and DAPI (1:200, Thermofisher, #62248) for 30min at room temperature in the dark and rinsed three times for 5min with dH2O. Sections were then imaged using the Zeiss LSM5 Exciter confocal laser-scanning microscope.
For immunohistochemistry, the sections were imaged on an upright compound Nikon Eclipse E800 microscope. The images were captured using a Nikon Digital Sight camera unit, equipped with a DS-Fi1 digital camera head and a DS-L2 camera controller. Pixel dimensions of the acquired images were W2584 X H1936 pixels, at 150 pixels/inch.
The images were processed using Photoshop CS6 software. The original images were scaled-down constraining proportions, and cropped to the area of interest. Adjustment of Image Levels was applied on whole images. Assembly of the composite figures and labeling was done on Illustrator CC2015.
Confocal images were obtained in a sequential manner using a Zeiss LSM5 Exciter Confocal Laser Scanning Microscope equipped with Argon (458, 488, 514nm), and 405, 450 and 635 diode excitation lasers and a 40× water immersion objective (C-APOCHROMAT 40×/1.2 Water). Emission ranges were set at 420–480, 505–550 and 560–615nm in separate channels to prevent bleeding. Images were obtained using the Leica application X software (Leica, Wetzlar, Germany) and post-acquisition data analysis was performed using ImageJ software.
Translation-blocking morpholino (MO) directed against atg5 (CATCCTTGTCATCTGCCATTATCAT) was obtained from Gene-Tools. The splice-blocking MO against Sqstm1/p62 (CTTCATCTAGAGACAAAGTTCAGGA) was a kind gift from Prof. AM Meijer. Splice efficiency of sqstm1 mRNA was tested in RT-PCR using a specific primer-set (Forward primer: 5′ ATTTGCAGCGAAAAGTGCTC 3′; Reverse primer:
5′ AGTGAACGGAAACCCAGGAA 3′). Embryos were injected at the 1–2-cell stage with either 2 ng (atg5) or 4 ng (Sqstm1/p62) of MO.
Wild type or lkb1 mutant zebrafish embryos were treated from 1 dpf in embryo-medium at 28°C with either of the following treatments: 50μM calpeptin (Abcam, #4ab120804), 1μM AR-12 (Medkoo Biosciences, #200272), or 10μM rapamycin (Sigma, #R0395). Stock solutions of AR-12, rapamycin and calpeptin were prepared in DMSO and diluted in embryo medium for treatment (final concentration of DMSO, 0.2%). Other treatments were prepared in embryo medium. All treatments were refreshed every 2–3 days, larvae collected at the specified time points and genotyped for the lkb1 gene. For Western Blotting, embryos were exposed to 2,5μM chloroquine (Sigma, #C6628) for 14h prior to lysing.
Statistical significance was determined using Fisher’s exact test in GraphPad software. Error bars represent the means±standard errors of the means (SEM) and are pooled from a minimum of two independent experiments. A p-value of <0.05 was used to define statistical significance.
We thank Prof. Annemarie Meijer (IBL) for the sqstm1/p62 morpholino and critical advice on the manuscript, Gerda Lamers (IBL) for advice with confocal microscopy, the DNA-Markerpoint facility (IBL) for genotyping, and the animal caretakers for excellent care of the fish. We also thank Dr. Anastassis Perrakis (NKI) for critical reading of the manuscript and the Life Science Editors for editorial assistance. The work was supported by a grant from the Dutch Cancer Society (KWF UL 2012–5395) to A.-P.G.H.
Conceived and designed the experiments: A.-P.G.H., L.A.M. and L.Q.C. Performed the experiments and collected data: L.A.M., L.Q.C., J.v.P., P.G. Analyzed the data: L.Q.C., L.A.M., W.-J.K., A.-P.G.H. Wrote the manuscript L.Q.C., A.-P.G.H. Reviewed and edited the manuscript: L.A.M., L.Q.C., W.-J.K., A.-P.G.H.
The authors declare that they have no competing interests.
Laurie A. Mans and Laia Querol Cano contributed equally to this work.
Electronic supplementary material
Supplementary information accompanies this paper at doi:10.1038/s41598-017-07116-9
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