Abstract
Background
Autophagy plays an important role in tumour cell growth and survival and also promotes resistance to chemotherapy. Hence, autophagy has been targeted for cancer therapy. We previously reported that macrolide antibiotics including azithromycin (AZM) inhibit autophagy in various types of cancer cells in vitro. However, the underlying molecular mechanism for autophagy inhibition remains unclear. Here, we aimed to identify the molecular target of AZM for inhibiting autophagy.
Methods
We identified the AZM-binding proteins using AZM-conjugated magnetic nanobeads for high-throughput affinity purification. Autophagy inhibitory mechanism of AZM was analysed by confocal microscopic and transmission electron microscopic observation. The anti-tumour effect with autophagy inhibition by oral AZM administration was assessed in the xenografted mice model.
Results
We elucidated that keratin-18 (KRT18) and α/β-tubulin specifically bind to AZM. Treatment of the cells with AZM disrupts intracellular KRT18 dynamics, and KRT18 knockdown resulted in autophagy inhibition. Additionally, AZM treatment suppresses intracellular lysosomal trafficking along the microtubules for blocking autophagic flux. Oral AZM administration suppressed tumour growth while inhibiting autophagy in tumour tissue.
Conclusions
As drug-repurposing, our results indicate that AZM is a potent autophagy inhibitor for cancer treatment, which acts by directly interacting with cytoskeletal proteins and perturbing their dynamics.
Similar content being viewed by others
Background
Autophagy, a lysosome-dependent system, degrades cellular components; it is involved in protein degradation to remove or recycle amino acids, thereby supplying energy under starvation conditions, and helps degrade damaged organelles for cellular homoeostasis [1]. Autophagy is involved in various aspects of cancer cell biology, e.g., carcinogenesis, tumour development, cancer stem cell maintenance, and resistance to chemotherapeutics [2,3,4,5]. Autophagy-deficient mice that are systematically mosaic for Atg5 deficiency, or are liver-specific Atg7 knockouts, develop liver adenomas, indicating that autophagy suppresses carcinogenesis [6]. In contrast, autophagy promotes tumorigenesis by supporting cancer cell proliferation and tumour growth. Hence, inhibiting autophagy suppresses tumour development [2]. Suppressing autophagy in non-malignant host cells, including those in the tumour microenvironment, suppresses tumour growth [7,8,9,10]. Small molecule inhibitors of autophagy can suppress tumour growth both in vitro and in vivo [11]. Thus, autophagy inhibitors may be suitable for cancer therapy; however, the only clinically available autophagy inhibitors are chloroquine (CQ) and hydroxychloroquine (HCQ). Several ongoing clinical trials involve HCQ administration in combination with other anti-cancer drugs. Although some prior trials showed a promising effect, not all patients were deemed fit to receive sufficient HCQ (1200 mg/day), owing to adverse events [12, 13]. Therefore, the development of an effective and feasible autophagy inhibitor with lower toxicity is desirable in the clinical setting.
Macrolide antibiotics, including azithromycin (AZM) and clarithromycin (CAM), inhibit autophagy [14,15,16]. Combined treatment with a proteasome inhibitor and macrolide resulted in pronounced cytotoxicity in myeloma and breast cancer cells, along with endoplasmic reticulum (ER) stress loading, owing to simultaneous inhibition of two major protein degradation systems: autophagy-lysosome system and ubiquitin-proteasomal system [17, 18]. Tyrosine kinase inhibitors (TKIs), including imatinib, dasatinib, gefitinib, erlotinib, and sorafenib, induce cytoprotective autophagy [19, 20]. Hence, co-treatment with these TKIs and macrolide for blocking autophagy has led to enhanced cytotoxic effects [21,22,23]. Since macrolide antibiotics exhibit almost no cytotoxicity alone, they appear to function as an adjuvant for TKIs in cancer treatment. Furthermore, the cytotoxic activities of DNA‐damaging drugs (e.g., doxorubicin, etoposide, and carboplatin) were enhanced in the presence of AZM in non-small cell lung cancer cell lines [24]. DNA-damaging drugs caused lysosomal damage and upregulated lysosomal biogenesis. Simultaneously, AZM treatment blocked autophagy to eliminate impaired lysosomes and accumulate lysosomes/autolysosomes. Thus, the effects were integrated into the marked increase in the damaged lysosomes/autolysosomes, leading to prominent lysosomal membrane permeabilization (LMP) for apoptosis induction.
Therefore, macrolide antibiotics can potentially be used as autophagy inhibitors in cancer therapy. However, the underlying molecular mechanism of AZM for autophagy inhibition is unclear. In the present study, we aimed to identify its molecular target during autophagy inhibition, using AZM-conjugated magnetic nanobeads for high-throughput affinity purification [25].
Methods
We treated human lung cancer (A549), human multiple myeloma (IM-9), and adrenal cortex-derived human adenocarcinoma (SW13) cell lines with/without AZM, and performed autophagic flux assay through western blotting using anti-LC3B antibody. We also used A549 cells expressing GFP-LC3/RFP-LC3ΔG for autophagic flux assay with a real-time live-cell imaging system. AZM binding proteins were identified using high-throughput affinity purification with AZM-conjugated magnetic nanobeads followed by LC-MS/MS analysis. We also established cell lines stably expressing the fluorescent proteins: A549/AcGFP-KRT18, A549/LAMP1-EGFP, A549/mCherry-LC3, A549/AcGFP-αTubulin, A549/mCherry-EGFP-LC3, SW13/LAMP1-EGFP, and SW13/mCherry-EGFP-LC3. To analyse the autophagosome/autolysosome formation and lysosomal maturation process, we examined data from immunofluorescence staining, live-cell imaging, and transmission electron microscopy. In vivo tumour growth inhibitory effects of AZM were determined in a xenografted mice model. OligoDNA sequences used for shRNA construction are listed in Table S1, and their details are provided in Supplementary Materials and Methods.
Results
AZM inhibits both autophagy and tumour growth
Macrolide antibiotics have previously been shown to inhibit autophagy [15, 16, 21]. To determine the potential of macrolide antibiotics for treating cancer, we assessed the autophagy inhibitory effect of AZM and CAM in A549 cells. AZM (>5 μM) increased levels of both the autophagosomal marker LC3B-II and autophagic substrate p62 in a dose-dependent manner, indicating autophagy inhibition (Fig. 1a). AZM treatment was accompanied by a greater increase in LC3B-II and p62 levels, compared with CAM treatment (Fig. 1a). To study autophagic flux, we co-administered bafilomycin A1 (BafA1) with either AZM or CAM. There was no further increase in LC3B-II or p62 levels compared with BafA1 administration alone. Moreover, co-administration of BafA1 with AZM or CAM induces higher LC3B-II levels than AZM or CAM administration alone. This indicates that although AZM and CAM block autophagic flux, some residual autophagic flux remained when cells were treated with AZM or CAM alone (Fig. 1b) [26]. Since AZM was a more potent autophagy inhibitor than CAM, we used AZM in our experiments.
Next, we compared autophagy inhibitory activity and cell toxicity of AZM with those of other well-known autophagy inhibitors, HCQ and BafA1 [27, 28], using an autophagic flux probe (GFP-LC3/RFP-LC3ΔG) [29]; GFP-LC3 and RFP-LC3ΔG are expressed at equal levels in transfected cells, but GFP-LC3 is involved in isolation membrane growth to form autophagosomes, and fusion with lysosome quenches the GFP signal due to its acidic environment, and GFP-LC3 is subsequently degraded via autophagy. In contrast, RFP-LC3ΔG remains in the cytosol because it lacks the glycine residue involved in autophagosome formation and serves as an internal control. Therefore, GFP/RFP ratios represent autophagic flux [29]. We analysed the cell confluency, GFP, and RFP signals separately (Fig. S1).
AZM treatment increased the GFP/RFP ratio (>5 μM) meaning inhibition of autophagy, as same as immunoblotting data, and the GFP/RFP ratio increased in a dose-dependent manner; HCQ and BafA1 treatment yielded similar results (Fig. 1c). Cell growth inhibition upon AZM treatment was moderate, even at higher concentrations, compared with HCQ treatment (Fig. S1a). Although HCQ increased the GFP/RFP ratio in a dose-dependent manner, this ratio decreased after 6–12 h at higher concentrations. This decrease probably occurred due to strong cell toxicity because RFP signals increased as cells began to die at higher HCQ concentrations (Fig. 1c, Fig. S1). After 24 h of exposure, AZM treatment exhibited better autophagy inhibition than HCQ autophagy inhibition (GFP/RFP ratio = 5–25 μM). BafA1 (≤50 nM) exhibited similar inhibitory effects as AZM after 24 h (Fig. 1c, Fig. S1). Based on this assay system, AZM inhibits autophagy to a similar extent as HCQ, but with lower cytotoxicity at equivalent concentrations in A549 cells cultured in a complete medium.
Genetic disruption of autophagy has been reported to suppress tumour growth [2]. The role of autophagy in tumour progression is to support metabolic homoeostasis of cancer cells in a harsh microenvironment [30]. We previously reported that AZM induces cell death in head and neck squamous cancer cell lines under the amino acid-depleted condition but not in the complete culture medium [31]. Therefore, we assessed whether AZM can inhibit autophagy and tumour growth in vivo, using a tumour xenograft model. Daily oral administration of AZM suppressed xenograft tumour growth and reduced harvested tumour weight without any weight loss in recipient mice (Fig. 1d–f). To determine the in vivo autophagy inhibitory effect, we performed immunofluorescence staining for p62 on harvested tumour tissues. AZM treatment increased p62 expression, suggesting that autophagy is suppressed by AZM in vivo (Fig. 1g). Our results indicate that AZM inhibits autophagy in vitro and in vivo and suppresses xenograft tumour growth when administered orally.
AZM interacts with KRT18
We attempted to identify the molecular target of AZM for autophagy inhibition. We generated AZM-conjugated magnetic nanobeads by crosslinking 3’-N,N-Di(desmethyl) azithromycin (NH2-AZM) and COOH beads (FG beads) (Fig. 2a). NH2-AZM is an AZM-derivative that inhibits autophagy (Fig. 2b). AZM-conjugated beads were incubated with A549 cell lysate, and proteins that bound to the beads were detected via silver staining and identified via LC-MS/MS analysis (Fig. 2c, Fig. S2, Table. S2). Notably, we identified intermediate filament protein keratin-7/8/18 (KRT7/8/18) and α/β-tubulin (TUBA1B/ TUBB) as major AZM-binding protein (Fig. 2c arrows). We found that both FLAG-tagged recombinant KRT7/8/18 and TUBA1B/TUBB and endogenous forms can bind to AZM-conjugated beads (Fig. 2d, e). Although valosin-containing protein (VCP) was previously reported as an AZM-binding protein [32], we found that only recombinant VCP can bind to AZM-conjugated beads. We used FLAG-LDH and another intermediate filament protein, vimentin (VIM), as negative controls (Fig. 2d, e). We focused on KRT18 because it was the protein most enriched by AZM-conjugated beads (Fig. 2d, e). AZM addition to our binding assay solution inhibited the interaction between FLAG-KRT18 and AZM-conjugated beads in a dose-dependent manner (Fig. 2f), indicating the specific interaction between AZM-conjugated beads and FLAG-KRT18.
KRT18 is composed of three major domains: the head, rod, and tail, arranged from the N- to C-terminus (Fig. 2g). The purified recombinant head domain expressed in Escherichia coli bound strongly to the AZM-conjugated beads, indicating that AZM binds directly to the N-terminal head domain of KRT18 (Fig. 2h). KRT18 is expressed in simple epithelial cells, and keratin filament networks are required for epithelial tissues to maintain their stiffness and integrity under mechanical stress [33]. We explored the effect of AZM on KRT18 networks to understand how AZM inhibits autophagy by interacting with KRT18. In untreated control cells, GFP-KRT18 forms keratin filaments and exhibits dynamic intracellular movements from the cell periphery toward the centre of the cell (Video 1) [34]. AZM treatment suppresses the dynamic movement of keratin, while keratin filaments became thicker than those in untreated cells (Fig. 2i, Video 2). Our findings indicate that AZM interacts directly with KRT18 and inhibits its movement in A549 cells.
KRT18 knockdown leads to autophagosome and lysosome accumulation along with autophagy inhibition
To determine whether KRT18 inhibition suppresses autophagy, we generated A549 cells expressing shRNA against KRT18 (shKRT18#1–3). KRT18 forms a heterodimer with either KRT7 or KRT8 [35], both of which were identified as AZM-binding proteins (Fig. 2c). KRT18 knockdown resulted in suppression of KRT7/8 expression, possibly due to the loss of a heterodimeric partner (Fig. 3a). LAMP2 and LC3B levels increased in KRT18 knockdown cells, suggesting the accumulation of either autophagosomes, lysosomes, and/or autolysosomes (Fig. 3a). Additionally, p62 levels were higher in shKRT18 cells, suggesting that KRT18 knockdown inhibits autophagic flux (Fig. 3a). This hypothesis is supported by the flux assay, which shows reduced LC3-II and p62 accumulation after BafA1 treatment compared to control cells (shNT) (Fig. S3). Immunofluorescence staining exhibited an increase in LC3B-positive autophagosomes and LAMP2-positive lysosomes in KRT18 knockdown cells (Fig. 3b). This accumulation of LC3B and LAMP2 in AZM-treated cells was elucidated via western blotting and immunofluorescence staining (Fig. 3c, d). Collectively, our results suggest that AZM suppresses autophagy by interacting directly with KRT18 and disrupting the keratin network.
AZM interacts with α/β-tubulin in non-epithelial cells
KRT18 is expressed in simple epithelial cells but not in cells derived from the mesoderm, such as IM-9 and keratin-deficient SW13 cells [36] (Fig. 4a); however, AZM treatment inhibited autophagy in both IM-9 and SW13 cells (Fig. 4b), suggesting the presence of AZM targets other than KRT18 during autophagy inhibition. Thus, we attempted to identify AZM-binding proteins expressed by IM-9 and SW13 cells using AZM-conjugated beads. We identified α/β-tubulin as a major band, as noted with A549 cells (Figs. 2a, 4c arrow, Tables S3, S4).
We assessed effect of AZM on tubulin polymerisation. SW13 cells were treated with AZM, and tubulin was separated into non-polymerised (Sup) and polymerised (Ppt) fractions. Paclitaxel (PTX), which stabilises tubulin, and vinorelbine (VNR), which inhibits tubulin polymerisation, were used as controls. PTX increased α-tubulin level in Ppt, but VNR reduced it. We did not observe any effect of AZM on polymerisation (Fig. 4d). Microtubules act as a scaffold for intracellular vesicle trafficking, as autophagosomes and lysosomes are transported by microtubule-based dynein and kinesin motor proteins [37]. Tubulin inhibitors inhibit autophagy; PTX or VNR treatment inhibited autophagy, as shown by flux assay (Fig. 4e). Conversely, tubulin acetylation is reported to be involved in autophagosome formation under starvation conditions [38], and SAHA, which inhibits activity of the tubulin deacetylation enzyme HDAC6, increased autophagic flux (Fig. 4e). Therefore, we determined the effect of AZM on cytoplasmic vesicle trafficking by measuring lysosomal movement in A549 cells expressing LAMP1-EGFP. Tracking analysis revealed that AZM treatment reduces the rate of lysosome migration along microtubules (Fig. 4f, Video 3, 4), suggesting that AZM can alter autophagic flux by modulating intracellular vesicle trafficking. The same result was noted for SW13 cells, suggesting that the effect of AZM on tubulin is independent of KRT18 (Fig. 4g). However, tubulin inhibitors disrupted KRT18 intracellular dynamics (Fig. S4a, Video 5–7). Additionally, KRT18 knockdown suppressed tubulin acetylation in A549 cells (Fig. S4b, c). Although we did not observe any change in α-tubulin acetylation in response to AZM treatment (Fig. S4d), these data indicate an interaction between KRT18 and microtubules. Thus, we concluded that AZM inhibits autophagic flux via interaction with these cytoskeletal proteins.
AZM does not perturb autolysosome formation
We aimed to determine which steps of the autophagic process were affected by AZM. Immunofluorescence staining showed the accumulation of large, round LAMP2-positive vesicles in AZM-treated A549 cell cytoplasm, most of which contained LC3B-positive materials (Fig. S5), indicating the accumulation of enlarged autolysosomes. Similarly, the accumulation of autolysosomes was observed in mCherry-LC3B and LAMP1-EGFP-expressing A549 cells via confocal microscopy (Fig. 5a). In contrast, in BafA1-treated cells, most LAMP1-EGFP signals coincided with mCherry-LC3, but vesicle formation was perturbed (Fig. 5a). A similar result was obtained via immunofluorescence staining (Fig. S5), indicating impairment of autolysosome formation by BafA1 [28]. Furthermore, during transmission electron microscopy (TEM), we observed an increased number of enlarged autolysosomes engulfing incompletely digested material in AZM-treated cells (Fig. 5b). In BafA1-treated cells, we observed many deformed lysosomes adjacent to autophagosomes containing intact materials, probably due to the lack of fusion with lysosomes (Fig. 5b). These findings indicate that AZM treatment results in the accumulation of enlarged autolysosomes containing undigested debris. Unlike BafA1, AZM does not block autophagosome-lysosome fusion, but AZM appears to inhibit subsequent autolysosomal digestion.
AZM inhibits lysosomal maturation and proteolysis
We investigated lysosomal function following drug treatment to determine how AZM inhibits digestion of autolysosomal contents. As acidification is critical for lysosomal hydrolytic enzyme activity [39], A549 and SW13 cells were stained with LysoTracker Red to track lysosome acidity. Although AZM treatment weakened the signals slightly compared with control cells in A549, the signal increased in SW13 cells (Fig. 6a). The same result was noted for flow cytometry; BafA1-treatment exhibited inhibition of lysosomal acidification in both cell lines (Fig. 6b). We also used a mCherry-GFP-LC3 probe; GFP fluorescence is quenched at low pH that results from fusion with acidic lysosomes [40]. Treating A549 cells with AZM increased the number of GFP+/mCherry+ signals, indicating autolysosomes to not be acidified (Fig. S6). However, in SW13 cells, AZM treatment increased the abundance of GFP-/mCherry+ large vesicles, indicating an acidic environment of autolysosomes (Fig. S6). These results demonstrated that AZM-induced inhibition of lysosomal acidification is cell-type dependent.
Next, we determined lysosomal proteolytic activity by introducing DQ Red BSA into A549 or SW13 cells expressing LAMP1-EGFP. DQ Red BSA was incorporated into cells via endocytosis and delivered to lysosomes. Before proteolysis, fluorescence of DQ Red BSA was quenched, but once DQ Red BSA was exposed to proteolysis, it showed red fluorescence. We detected proteolytic activity in control cells 6 h after pulse-administration of DQ Red BSA. However, in the presence of AZM, proteolytic activity was almost undetectable (Fig. 6c). Endocytosis assessment using Dextran-Alexa488 indicated that AZM did not disrupt the endocytosis in A549 and SW13 cells (Fig. S7). These results demonstrated that AZM suppresses hydrolytic enzymatic activity in lysosomes, regardless of lysosomal acidity, and support the TEM findings showing the cytosolic accumulation of enlarged autolysosomes containing undigested debris (Fig. 5b). For further confirmation, we assessed the maturation of hydrolytic enzymes cathepsin D (CTSD), and α-glucosidase (GAA) via western blotting in KRT18-expressing A549 and MCF7 cells and KRT18-non-expressing 293 T and SW13 cells (Fig. 6d). CTSD and GAA mature via cleavage during lysosomal maturation [41, 42]. Notably, similar to A549 and SW13 cells, MCF7 cells showed a decrease in LysoTracker Red signals, whereas 293 T cells showed an increase in LysoTracker Red signals, in response to AZM treatment (Fig. S8). Since lysosomal acidity is an important condition for enzymatic maturation, BafA1 is used as a control to suppress lysosomal acidification (Fig. 6b, S8). In all cells, BafA1 treatment inhibited the maturation of CTSD and GAA, as indicated by repression of the active form of CTSD and mature-GAA (Fig. 6e). Similarly, AZM treatment decreased levels of the mature forms of CTSD and GAA, suggesting that AZM suppresses lysosomal enzymatic maturation, regardless of whether it inhibits lysosomal acidification. Finally, we assessed the involvement of KRT18 in maturation of CTSD and GAA. In KRT18 knockdown cells, the levels of proforms of these enzymes increased slightly without an apparent decrease in the levels of mature forms of these enzymes (Fig. 6f), suggesting that KRT18 is involved in lysosomal maturation.
Discussion
In this study, we elucidated that AZM specifically interacts with keratin-18 and α/β-tubulin, in addition to disturbing their cytoskeletal dynamics. Thus, we concluded that these cytoskeletal proteins are molecular targets of the autophagy inhibitory effect of AZM via suppression of trafficking of lysosomes and inhibition of lysosomal functional maturation. Since BafA1, a well-known autophagy inhibitor, has been reported to target both V-ATPase-dependent acidification and Ca-P60A/SERCA-dependent autophagosome-lysosome fusion independently for autophagy inhibition [28], it is not surprising that there are two targets of AZM for autophagy inhibition. Indeed, we have not obtained any data indicating a correlation between KRT18 expression level and AZM-induced growth inhibition in several cancer cell lines used in this study (data not shown). We have demonstrated that KRT18 knockdown inhibits autophagic flux and partially suppresses lysosomal enzymatic maturation. Additionally, lysosomal trafficking on the microtubules was significantly repressed in the presence of AZM, which explains the autophagy inhibition in cells derived from mesoderm with no KRT18 expression. Since microtubules are critical for cellular physiology, including cell division, it was practically difficult to perform the experiments for α/β-tubulin knockdown. Thus, the involvement of α/β-tubulin in AZM-induced autophagy inhibition is still circumstantial. However, microtubules have a well-documented role in autophagy, which involves forming a scaffold for intracellular vesicle trafficking including autophagosomes and lysosomes [37].
In contrast to microtubules, the role of intermediate filaments, including keratin, in autophagic regulation is not well-documented. Our study showed that AZM disrupts intracellular dynamics of keratin filaments, thereby suppressing autophagy and accumulating autophagosomes, lysosomes, and autolysosomes (Figs. 2, 3, Video 2). Our findings indicate that KRT18 is a molecular target of AZM for autophagy inhibition (Figs. 3, 6). There are several reports supporting our findings, thereby suggesting keratin’s involvement in autophagy. In retinal pigment epithelium under paraquat-treated conditions, KRT8-knockdown suppressed autolysosome formation, but KRT8-overexpression promoted autolysosome formation [43]. In another study, KRT8 knockdown suppressed autophagy and overcame chemoresistance of chordoma cells [44]. These results indicate the involvement of keratin filaments in autophagy.
Currently, there is no concrete evidence for the interaction between keratin and microtubules for autophagy inhibition; both were identified as the targets of AZM in this study. Notably, keratin knockdown reduced α-tubulin acetylation (Fig. S4b, c), along with autophagy inhibition, implying that keratin interacts with microtubules to regulate autophagy. Conversely, tubulin inhibitors disrupt keratin networks (Fig. S4a, Video 5–7). Although keratin filaments are known to move from the cell periphery to the cell centre (Video 1), the molecular mechanisms underlying these dynamics remain unclear [34]. Microtubule-based such retrograde transport is used for endosomal trafficking and is carried out by dynein, which is involved in autophagy regulation [37, 38]. It is crucial to understand the molecular mechanism underlying the interaction between microtubules and intermediate filaments during autophagy.
AZM possesses weakly basic lipophilic compounds, which accumulate in acidic organelles, including lysosomes. CQ is one of the well-known lysosomotropic compounds. These compounds increase lysosomal pH and disrupt lysosomal function because an acidic environment is critical for lysosomal hydrolytic enzyme activity [39]. Additionally, lysosomal enzymatic maturation was disturbed under high lysosomal pH because lysosomal enzymes are proteolytically processed and maturated by other lysosomal enzymes. However, in this study, although AZM inhibited lysosomal enzymatic maturation (Fig. 6e), it appeared to be independent of lysosomal pH; A549 and MCF7 cells showed a decreased LysoTracker Red signal, whereas it increased in SW13 and 293 T cells (Fig. 6a, Fig. S7). Additionally, this impaired enzyme maturation was partially observed in KRT18 KD cells. Thus, further research should determine whether the lysosomal maturation inhibition is due to the repression of KRT18 movement or by the lysosomotropic compound itself.
Several ongoing clinical trials involving HCQ in cancer therapy involve the combination of HCQ with other anticancer drugs. Combination chemotherapy with HCQ has shown improved clinical outcomes in cases of glioblastoma and pancreatic ductal adenocarcinoma [45,46,47], but some trials did not show beneficial outcomes or sufficient benefit to warrant further study when compared with combination chemotherapies currently available [13, 48]. Throughout these trials, despite promising certain therapeutic effects, it has been difficult to demonstrate actual autophagy inhibition in response to HCQ in cancer patients. Additionally, some patients cannot receive an effective dose of HCQ due to its toxicity, which has led to an unsatisfactory outcome [2, 12, 13]. Thus, developing other effective and feasible autophagy inhibitors is an important clinical issue. AZM has been in daily clinical use for a long time; it has a long half-life (68 h), high tissue penetration, and 10–100 times higher concentration in human tissues compared with serum [49, 50]. Although AZM has a short measured half-life of 4 h in mice compared with humans [51], we still observed significant anti-tumour effects in mice following oral administration (Fig. 1). Furthermore, AZM showed less toxicity than HCQ in vitro (Fig. S1). These findings suggest the superiority of AZM for cancer therapy as an autophagy inhibitor. Genetically autophagy-deficient mice (atg5 or atg7 KO mice) are born normally but die within one day due to insufficient nutrition [52, 53]. In the case of induced whole-body atg7 deletion in adult mice, most mutant mice die within 2–3 months due to infection and neurodegeneration [8]. BafA1 cannot be clinically used due to toxicity [54]. These data demonstrate excessive autophagy inhibition may damage the whole body in clinical application. Supporting this notion, a new autophagic inhibitor Lys05, a dimeric CQ, strongly inhibits autophagy but also causes Paneth cell dysfunction and intestinal toxicity in mice. This outcome is identical to that reported in humans and in mice carrying mutations in the autophagy gene Atg16l1 [55]. Since AZM was less toxic to cultured cells than HCQ, and we have not observed any toxicity in orally-administrated mice at 100 μg/g/day; the risk of adverse events may be limited. We believe that the growth inhibitory effect and cell toxicity of AZM are dependent on how much the cancer cells rely on autophagy for their growth or survival, as we previously demonstrated [21, 31].
In this study, we found that keratin-7/8/18 and α/β-tubulin are novel targets of AZM for autophagy inhibition. Several questions remain unanswered; it is unknown how KRT7/8/18 regulates autophagy and what molecule(s) are involved in lysosomal trafficking and maturation after the interaction between AZM and these cytoskeletal proteins. However, the identification of molecular targets of AZM and assessment of its antitumor effect in an orally administrated xenograft mice model lays the foundation for further clinical application of AZM as an autophagy inhibitor in cancer therapy.
Data availability
The datasets used and/or analysed during the current study are available from the corresponding author on reasonable request.
References
Mizushima N, Komatsu M. Autophagy: renovation of cells and tissues. Cell. 2011;147:728–41.
Amaravadi R, Kimmelman AC, White E. Recent insights into the function of autophagy in cancer. Genes Dev. 2016;30:1913–30.
Sbrana FV, Cortini M, Avnet S, Perut F, Columbaro M, De Milito A, et al. The role of autophagy in the maintenance of stemness and differentiation of mesenchymal stem cells. Stem Cell Rev Rep. 2016;12:621–33.
Rehman SK, Haynes J, Collignon E, Brown KR, Wang Y, Nixon AML, et al. Colorectal cancer cells enter a Diapause-like DTP state to survive chemotherapy. Cell. 2021;184:226–242:e221.
Vera-Ramirez L, Vodnala SK, Nini R, Hunter KW, Green JE. Autophagy promotes the survival of dormant breast cancer cells and metastatic tumour recurrence. Nat Commun. 2018;9:1944.
Takamura A, Komatsu M, Hara T, Sakamoto A, Kishi C, Waguri S, et al. Autophagy-deficient mice develop multiple liver tumors. Genes Dev. 2011;25:795–800.
Poillet-Perez L, Xie X, Zhan L, Yang Y, Sharp DW, Hu ZS, et al. Autophagy maintains tumour growth through circulating arginine. Nature. 2018;563:569–73.
Karsli-Uzunbas G, Guo JY, Price S, Teng X, Laddha SV, Khor S, et al. Autophagy is required for glucose homeostasis and lung tumor maintenance. Cancer Discov. 2014;4:914–27.
Yang A, Herter-Sprie G, Zhang H, Lin EY, Biancur D, Wang X, et al. Autophagy sustains pancreatic cancer growth through both cell-autonomous and nonautonomous mechanisms. Cancer Discov. 2018;8:276–87.
Katheder NS, Khezri R, O’Farrell F, Schultz SW, Jain A, Rahman MM, et al. Microenvironmental autophagy promotes tumour growth. Nature. 2017;541:417–20.
Amaravadi RK, Kimmelman AC, Debnath J. Targeting autophagy in cancer: recent advances and future directions. Cancer Discov. 2019;9:1167–81.
Onorati AV, Dyczynski M, Ojha R, Amaravadi RK. Targeting autophagy in cancer. Cancer. 2018;124:3307–18.
Rosenfeld MR, Ye X, Supko JG, Desideri S, Grossman SA, Brem S, et al. A Phase I/II trial of hydroxychloroquine in conjunction with radiation therapy and concurrent and adjuvant temozolomide in patients with newly diagnosed glioblastoma multiforme. Autophagy. 2014;10:1359–68.
Mukai S, Moriya S, Hiramoto M, Kazama H, Kokuba H, Che XF, et al. Macrolides sensitize EGFR-TKI-induced non-apoptotic cell death via blocking autophagy flux in pancreatic cancer cell lines. Int J Oncol. 2016;48:45–54.
Moriya S, Che XF, Komatsu S, Abe A, Kawaguchi T, Gotoh A, et al. Macrolide antibiotics block autophagy flux and sensitize to bortezomib via endoplasmic reticulum stress-mediated CHOP induction in myeloma cells. Int J Oncol. 2013;42:1541–50.
Renna M, Schaffner C, Brown K, Shang S, Tamayo MH, Hegyi K, et al. Azithromycin blocks autophagy and may predispose cystic fibrosis patients to mycobacterial infection. J Clin Invest. 2011;121:3554–63.
Miyahara K, Kazama H, Kokuba H, Komatsu S, Hirota A, Takemura J, et al. Targeting bortezomib-induced aggresome formation using vinorelbine enhances the cytotoxic effect along with ER stress loading in breast cancer cell lines. Int J Oncol. 2016;49:1848–58.
Moriya S, Komatsu S, Yamasaki K, Kawai Y, Kokuba H, Hirota A, et al. Targeting the integrated networks of aggresome formation, proteasome, and autophagy potentiates ER stress‑mediated cell death in multiple myeloma cells. Int J Oncol. 2015;46:474–86.
Han W, Pan H, Chen Y, Sun J, Wang Y, Li J, et al. EGFR tyrosine kinase inhibitors activate autophagy as a cytoprotective response in human lung cancer cells. PLoS One. 2011;6:e18691.
Bellodi C, Lidonnici MR, Hamilton A, Helgason GV, Soliera AR, Ronchetti M, et al. Targeting autophagy potentiates tyrosine kinase inhibitor-induced cell death in Philadelphia chromosome-positive cells, including primary CML stem cells. J Clin Invest. 2009;119:1109–23.
Tanaka H, Hino H, Moriya S, Kazama H, Miyazaki M, Takano N, et al. Comparison of autophagy inducibility in various tyrosine kinase inhibitors and their enhanced cytotoxicity via inhibition of autophagy in cancer cells in combined treatment with azithromycin. Biochem Biophys Rep. 2020;22:100750.
Sugita S, Ito K, Yamashiro Y, Moriya S, Che XF, Yokoyama T, et al. EGFR-independent autophagy induction with gefitinib and enhancement of its cytotoxic effect by targeting autophagy with clarithromycin in non-small cell lung cancer cells. Biochem Biophys Res Commun. 2015;461:28–34.
Ohtomo T, Miyazawa K, Naito M, Moriya S, Kuroda M, Itoh M, et al. Cytoprotective effect of imatinib mesylate in non-BCR-ABL-expressing cells along with autophagosome formation. Biochem Biophys Res Commun. 2010;391:310–5.
Toriyama K, Takano N, Kokuba H, Kazama H, Moriya S, Hiramoto M, et al. Azithromycin enhances the cytotoxicity of DNA-damaging drugs via lysosomal membrane permeabilization in lung cancer cells. Cancer Sci. 2021;112:3324–37.
Ito T, Ando H, Suzuki T, Ogura T, Hotta K, Imamura Y, et al. Identification of a primary target of thalidomide teratogenicity. Science. 2010;327:1345–50.
Mizushima N, Murphy LO. Autophagy assays for biological discovery and therapeutic development. Trends Biochem Sci. 2020;45:1080–93.
Mauthe M, Orhon I, Rocchi C, Zhou X, Luhr M, Hijlkema KJ, et al. Chloroquine inhibits autophagic flux by decreasing autophagosome-lysosome fusion. Autophagy. 2018;14:1435–55.
Mauvezin C, Nagy P, Juhász G, Neufeld TP. Autophagosome-lysosome fusion is independent of V-ATPase-mediated acidification. Nat Commun. 2015;6:7007.
Kaizuka T, Morishita H, Hama Y, Tsukamoto S, Matsui T, Toyota Y, et al. An autophagic flux probe that releases an internal control. Mol Cell. 2016;64:835–49.
Perera RM, Stoykova S, Nicolay BN, Ross KN, Fitamant J, Boukhali M, et al. Transcriptional control of autophagy-lysosome function drives pancreatic cancer metabolism. Nature. 2015;524:361–5.
Hirasawa K, Moriya S, Miyahara K, Kazama H, Hirota A, Takemura J, et al. Macrolide antibiotics exhibit cytotoxic effect under amino acid-depleted culture condition by blocking autophagy flux in head and neck squamous cell carcinoma cell lines. PLoS One. 2016;11:e0164529.
Nujic K, Smith M, Lee M, Belamaric D, Tomaskovic L, Alihodzic S, et al. Valosin containing protein (VCP) interacts with macrolide antibiotics without mediating their anti-inflammatory activities. Eur J Pharmacol. 2012;677:163–72.
Loschke F, Seltmann K, Bouameur JE, Magin TM. Regulation of keratin network organization. Curr Opin Cell Biol. 2015;32:56–64.
Windoffer R, Beil M, Magin TM, Leube RE. Cytoskeleton in motion: the dynamics of keratin intermediate filaments in epithelia. J Cell Biol. 2011;194:669–78.
Kim HJ, Choi WJ, Lee CH. Phosphorylation and reorganization of keratin networks: Implications for carcinogenesis and epithelial mesenchymal transition. Biomol Ther (Seoul). 2015;23:301–12.
Hedberg KK, Chen LB. Absence of intermediate filaments in a human adrenal cortex carcinoma-derived cell line. Exp Cell Res. 1986;163:509–17.
Mackeh R, Perdiz D, Lorin S, Codogno P, Pous C. Autophagy and microtubules—new story, old players. J Cell Sci. 2013;126:1071–80.
Geeraert C, Ratier A, Pfisterer SG, Perdiz D, Cantaloube I, Rouault A, et al. Starvation-induced hyperacetylation of tubulin is required for the stimulation of autophagy by nutrient deprivation. J Biol Chem. 2010;285:24184–94.
Mindell JA. Lysosomal acidification mechanisms. Annu Rev Physiol. 2012;74:69–86.
N’Diaye EN, Kajihara KK, Hsieh I, Morisaki H, Debnath J, Brown EJ. PLIC proteins or ubiquilins regulate autophagy-dependent cell survival during nutrient starvation. EMBO Rep. 2009;10:173–9.
Moreland RJ, Jin X, Zhang XK, Decker RW, Albee KL, Lee KL, et al. Lysosomal acid alpha-glucosidase consists of four different peptides processed from a single chain precursor. J Biol Chem. 2005;280:6780–91.
Zaidi N, Maurer A, Nieke S, Kalbacher H. Cathepsin D: a cellular roadmap. Biochem Biophys Res Commun. 2008;376:5–9.
Baek A, Yoon S, Kim J, Baek YM, Park H, Lim D, et al. Autophagy and KRT8/keratin 8 protect degeneration of retinal pigment epithelium under oxidative stress. Autophagy. 2017;13:248–63.
Wang D, Zhang P, Xu X, Wang J, Wang D, Peng P, et al. Knockdown of cytokeratin 8 overcomes chemoresistance of chordoma cells by aggravating endoplasmic reticulum stress through PERK/eIF2α arm of unfolded protein response and blocking autophagy. Cell Death Dis. 2019;10:887.
Briceño E, Reyes S, Sotelo J. Therapy of glioblastoma multiforme improved by the antimutagenic chloroquine. Neurosurg Focus. 2003;14:e3.
Sotelo J, Briceño E, López-González MA. Adding chloroquine to conventional treatment for glioblastoma multiforme: a randomized, double-blind, placebo-controlled trial. Ann Intern Med. 2006;144:337–43.
Boone BA, Bahary N, Zureikat AH, Moser AJ, Normolle DP, Wu WC, et al. Safety and biologic response of pre-operative autophagy inhibition in combination with gemcitabine in patients with pancreatic adenocarcinoma. Ann Surg Oncol. 2015;22:4402–10.
Haas NB, Appleman LJ, Stein M, Redlinger M, Wilks M, Xu X, et al. Autophagy inhibition to augment mTOR inhibition: a Phase I/II trial of everolimus and hydroxychloroquine in patients with previously treated renal cell carcinoma. Clin Cancer Res. 2019;25:2080–7.
Kong FYS, Horner P, Unemo M, Hocking JS. Pharmacokinetic considerations regarding the treatment of bacterial sexually transmitted infections with azithromycin: a review. J Antimicrob Chemother. 2019;74:1157–66.
Foulds G, Shepard RM, Johnson RB. The pharmacokinetics of azithromycin in human serum and tissues. J Antimicrob Chemother. 1990;25:73–82.
Azoulay-Dupuis E, Vallée E, Bedos JP, Muffat-Joly M, Pocidalo JJ. Prophylactic and therapeutic activities of azithromycin in a mouse model of pneumococcal pneumonia. Antimicrob Agents Chemother. 1991;35:1024–8.
Komatsu M, Waguri S, Ueno T, Iwata J, Murata S, Tanida I, et al. Impairment of starvation-induced and constitutive autophagy in Atg7-deficient mice. J Cell Biol. 2005;169:425–34.
Kuma A, Hatano M, Matsui M, Yamamoto A, Nakaya H, Yoshimori T, et al. The role of autophagy during the early neonatal starvation period. Nature. 2004;432:1032–6.
Dröse S, Altendorf K. Bafilomycins and concanamycins as inhibitors of V-ATPases and P-ATPases. J Exp Biol. 1997;200:1–8.
McAfee Q, Zhang Z, Samanta A, Levi SM, Ma XH, Piao S, et al. Autophagy inhibitor Lys05 has single-agent antitumor activity and reproduces the phenotype of a genetic autophagy deficiency. Proc Natl Acad Sci USA. 2012;109:8253–8.
Acknowledgements
We thank Ms. Ayako Hirota to help for preparing manuscript.
Funding
This study was supported by the Ministry of Education, Culture, Sports, Science and Technology (MEXT)-supported programme of the Strategic Research Foundation at Private Universities (S1411011, 2014-2018) (to KM), by JSPS KAKENHI Grant Numbers 17K15031 and 20K07298 (to NT), by a Grant-in-Aid from Tokyo Medical University Cancer Research (to KM and NT), and by AMED under Grant Number JP18lm0203004 (to NT).
Author information
Authors and Affiliations
Contributions
NT, MH, YY, HK, MT, HH: Performed research and analysed data. NT, KM: Conceptualisation. NT, MH, KM: Writing -original draft. NT, KM: Writing -review and editing.
Corresponding authors
Ethics declarations
Competing interests
The authors declare no competing interests.
Ethics approval and consent to participate
Animal protocols were in accordance with the Regulations and Guidelines on Scientific and Ethical Care and Use of Laboratory Animals by Science Council of Japan and were approved by the Tokyo Medical University Animal Care and Use Committee.
Additional information
Publisher’s note Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Rights and permissions
Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The images or other third party material in this article are included in the article’s Creative Commons license, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons license and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this license, visit http://creativecommons.org/licenses/by/4.0/.
About this article
Cite this article
Takano, N., Hiramoto, M., Yamada, Y. et al. Azithromycin, a potent autophagy inhibitor for cancer therapy, perturbs cytoskeletal protein dynamics. Br J Cancer 128, 1838–1849 (2023). https://doi.org/10.1038/s41416-023-02210-4
Received:
Revised:
Accepted:
Published:
Issue Date:
DOI: https://doi.org/10.1038/s41416-023-02210-4