Identification of an acetylation-dependant ku70/flip complex that regulates flip expression and hdac inhibitor-induced apoptosis

ABSTRACT FLIP is a potential anti-cancer therapeutic target that inhibits apoptosis by blocking caspase 8 activation by death receptors. We report a novel interaction between FLIP and the

DNA repair protein Ku70 that regulates FLIP protein stability by inhibiting its polyubiquitination. Furthermore, we found that the histone deacetylase (HDAC) inhibitor Vorinostat (SAHA)

enhances the acetylation of Ku70, thereby disrupting the FLIP/Ku70 complex and triggering FLIP polyubiquitination and degradation by the proteasome. Using _in vitro_ and _in vivo_ colorectal

cancer models, we further demonstrated that SAHA-induced apoptosis is dependant on FLIP downregulation and caspase 8 activation. In addition, an HDAC6-specific inhibitor Tubacin

recapitulated the effects of SAHA, suggesting that HDAC6 is a key regulator of Ku70 acetylation and FLIP protein stability. Thus, HDAC inhibitors with anti-HDAC6 activity act as efficient

post-transcriptional suppressors of FLIP expression and may, therefore, effectively act as ‘FLIP inhibitors’. SIMILAR CONTENT BEING VIEWED BY OTHERS CONVERSION OF KU80 K568 CROTONYLATION TO

SUMOYLATION FACILITATES DNA NON-HOMOLOGOUS END JOINING AND CANCER RADIORESISTANCE Article Open access 21 April 2025 SIRT1 DEACETYLATES WEE1 AND SENSITIZES CANCER CELLS TO WEE1 INHIBITION

Article 12 January 2023 DEUBIQUITINASE OTUD6A PROMOTES BREAST CANCER PROGRESSION BY INCREASING TOPBP1 STABILITY AND RENDERING TUMOR CELLS RESISTANT TO DNA-DAMAGING THERAPY Article 29 June

2022 MAIN FLIP is an anti-apoptotic protein that blocks the activation of apoptosis mediated by death receptors, such as Fas, TRAIL receptor 1 (TRAIL-R1/DR4) and TRAIL-R2 (DR5).1 By binding

to the adaptor protein FADD, FLIP inhibits apoptosis by blocking the processing and activation of procaspase 8 (FLICE) by death receptor complexes termed DISCs (death-inducing signalling

complexes).2 We previously reported that FLIP inhibits apoptosis induced by chemotherapeutic agents3 and that high FLIP expression is an independent adverse prognostic biomarker in

colorectal cancer (CRC).4 These and other studies have indicated that inhibition of FLIP constitutes a promising therapeutic strategy for the treatment of CRC. Ku70 and its binding partner

Ku80 are critical components of the non-homologous end joining (NHEJ) DNA repair machinery.5 Ku70 is regulated by acetylation, which is mediated by the histone acetyl transferases (HATs);

CREB-binding protein (CBP) and PCAF, and its acetylation can be enhanced by treating cells with histone deacetylase (HDAC) inhibitors.6 Ku70 acetylation disrupts its DNA-binding activity and

sensitises cells to DNA-damaging agents.7 In addition, cytoplasmic Ku70 binds to and regulates the pro-apoptotic Bcl-2 family member, Bax.6 Ku70 simultaneously inhibits Bax degradation via

the ubiquitin proteasome system (UPS) and prevents its translocation to the mitochondria.8 Moreover, it has been reported that Ku70 may have intrinsic de-ubiquitinating (DUB) activity.8 The

Ku70–Bax complex is disrupted by Ku70 acetylation, which promotes Bax translocation to mitochondria and apoptosis induction.6 Herein, we report a novel interaction between FLIP and Ku70 that

regulates FLIP stability. This interaction is acetylation-dependant and is disrupted by HDAC inhibitors with activity against HDAC6. Disruption of the Ku70–FLIP interaction subsequently

leads to FLIP degradation by the UPS and induction of caspase 8-dependant apoptosis. RESULTS FLIP INTERACTS WITH KU70 A yeast-2-hybrid screen was carried out to identify novel binding

partners for the long FLIP splice variant (FLIP(L)). One of the novel proteins identified was Ku70. The interaction between FLIP(L) and Ku70 was confirmed by re-transformation assay (Figure

1a). Immunoprecipitation experiments confirmed that FLIP(L) interacts with Ku70 in CRC cells (Figure 1b). Despite the predominant site of Ku70 expression being nuclear, the interaction

between FLIP(L) and Ku70 was more prominent in cytosolic fractions (Figure 1c), suggesting that the primary site of the interaction is cytosolic. Ku70 also interacted with the short FLIP

splice form, FLIP(S) (Supplementary Figure S1A). To map Ku70's interaction with FLIP, we generated a series of Flag-tagged Ku70 constructs. The region from 430 to 609 amino acids

interacted strongly with FLIP, however, neither the 496–609 nor the 535–609 fragments interacted (Figure 1d). These mapping experiments indicate that Ku70 binds FLIP via a region between

amino acids 430 and 496, which encompasses one of its sites of interaction with Ku80. KU70 BINDS TO DED2 OF FLIP To identify the regions of FLIP that are important for the FLIP–Ku70

interaction, we used a FLIP peptide array of overlapping 25-mer peptides, each shifted by four amino acids, encompassing the entire FLIP(S) sequence.9 Duplicate membranes were overlaid with

lysates from cells transfected with Flag-Ku70, and the Flag epitope detected by immunoblotting. Strong binding of Ku70 to the array was detected in four regions (Figure 2a and table). To map

the FLIP–Ku70 interaction to specific amino acids, alanine substitution arrays were constructed for peptides 17, 30, 41 and 46. Several alanine substitutions in peptide 30 (but not the

other 3 peptides) were found to disrupt the binding of Ku70 (Figure 2b). By using viral FLIP MC159 as a template,10 a homology model of human FLIP(S) was generated. The model predicted that

two of the candidate residues identified in the alanine substitution array, Y119 and R122, are prominently surface exposed and, therefore, available for making protein–protein interactions

(Figure 2c); the other candidate residues were predicted to be buried. Mutation of FLIP(S) R122, but not Y119, to alanine significantly diminished binding to Ku70 (Figure 2d). Thus, these

studies identify R122 as a critical site of interaction between FLIP and Ku70. This region of FLIP death effector domain 2 (DED2) is present in all FLIP splice forms and is adjacent to the

‘hydrophobic patch’ region reported to be important for binding to FADD.11 Binding of FADD and procaspase 8 to FLIP was unaffected by R122A mutation indicating that FADD/procaspase 8 and

Ku70 interact with distinct regions of FLIP (Figure 2d). SAHA DISRUPTS THE FLIP–KU70 INTERACTION AND INDUCES FLIP DEGRADATION Treatment with the HDAC inhibitor Vorinostat (SAHA,

suberoylanilide hydroxamic acid) for 2 h disrupted the interaction between endogenous FLIP and Ku70 (Figure 3a), and increased Ku70 acetylation after 1 h (Figure 3b). Increased Ku70

acetylation following SAHA treatment was also observed in three other CRC cell lines (Supplementary Figure S1B). Although Ku70 was primarily expressed in the nucleus, acetylated Ku70 was

detectable at similar levels in the nucleus and the cytosol, and increased in both sub-cellular locations following SAHA treatment (Supplementary Figure S1C). We were unable to detect the

acetylation of FLIP following SAHA treatment (Supplementary Figure S1D), suggesting that it is not directly modified by acetylation. Ku70 acetylation following SAHA treatment decreased its

capacity to bind to FLIP (Figure 3b). Cohen _et al._6 demonstrated that mimicking the acetylation of lysine residues K539 or K542 in Ku70 by mutating them to glutamine disrupted its ability

to inhibit Bax-mediated apoptosis. We found that mutation of either of these residues to glutamine impaired the ability of Ku70 to interact with FLIP (Figure 3c). Collectively, these results

indicate that Ku70 acetylation inhibits its ability to interact with FLIP. Disruption of FLIP–Ku70 binding following SAHA treatment correlated with increased polyubiquitination of FLIP(L)

and FLIP(S) (Figure 3d) and rapid downregulation of both splice forms from ∼4 h following treatment (Figure 3e). SAHA treatment also downregulated FLIP protein expression in three other CRC

cell lines after 6 h at sub-IC50 doses (Supplementary Figures S2C and E). In contrast to other studies, which have found that HDAC inhibitors downregulate FLIP at the transcriptional

level,12, 13 we found no evidence of transcriptional suppression of FLIP in CRC cells (Supplementary Figures S2A and D). Moreover, co-treatment with the proteasome inhibitor MG132 attenuated

SAHA-induced FLIP downregulation (Supplementary Figure S2B), providing further evidence that FLIP downregulation is mediated by the UPS. KU70 POST-TRANSCRIPTIONALLY REGULATES FLIP

EXPRESSION Transfection with three different Ku70-targeted siRNAs resulted in Ku70 depletion and significant decreases in FLIP expression (Figure 4a). Similar effects were observed in three

other CRC cell lines (Figure 4b). However, Ku70 depletion had no effect on FLIP mRNA expression (Figure 4c). siRNA-mediated Ku70 downregulation resulted in apoptosis as indicated by

poly(ADP-ribose) polymerase (PARP) cleavage (Figure 4d), flow cytometry (Figure 4e) and caspase 3/7 activation (Supplementary Figure S3A). The FLIP downregulation observed in Ku70-depleted

cells was not an indirect result of caspase activation, as inhibition of apoptosis with the pan-caspase inhibitor z-VAD-fmk failed to prevent FLIP downregulation in Ku70-depleted cells

(Figure 4d). Furthermore, the half-lives of both FLIP(L) and FLIP(S) were significantly reduced in Ku70-depleted cells, with almost undetectable levels of FLIP 1 h after treatment with the

protein synthesis inhibitor cycloheximide (Figure 4f). Importantly, Ku70 downregulation resulted in increased levels of polyubiquitinated FLIP(L) and FLIP(S) (Figure 4g), suggesting that

Ku70 enhances the half-life of FLIP by inhibiting its degradation via the UPS. SAHA- AND KU70 SIRNA-INDUCED APOPTOSIS IS CASPASE 8-DEPENDANT Analysis of other apoptotic proteins indicated

that unlike FLIP, none were significantly affected by SAHA treatment after 6 h, however, Bax was upregulated and XIAP downregulated 24 h following SAHA treatment (Figure 5a). Despite being

acetylated, total Ku70 expression was not affected by SAHA treatment (Figure 5a). Expression of several BH3-only proteins was also assessed: NOXA and BID were not significantly altered

following SAHA treatment, whereas PUMA was downregulated and BIM upregulated (Figure 5b). As the upregulation of Bax and BIM at 24 h coincided with the onset of apoptosis as determined by

PARP cleavage, we directly assessed the roles of the initiator caspases, caspase 8 and caspase 9 during SAHA-induced apoptosis. siRNA-mediated inhibition of caspase 8 significantly inhibited

SAHA-induced apoptosis in each CRC cell line as assessed by flow cytometry (Figure 5c), PARP cleavage (Supplementary Figure S4A) and analysis of caspase 3/7 activity (Supplementary Figure

S4C). In contrast, caspase 9 silencing failed to inhibit SAHA-induced apoptosis (Figure 5c). Furthermore, caspase 8 activity increased following SAHA treatment and correlated with increased

activity of the executioner caspases 3/7 (Figure 5d). SAHA treatment also resulted in significant increases in caspase 8 activity in other CRC cell lines (Supplementary Figure S4B). Notably,

increased caspase 8 activity was detected in Ku70-depleted HCT116 cells (Supplementary Figure S3A), and the apoptosis induced by Ku70 silencing was caspase 8-dependant (Figure 4e). Similar

results were observed in HT29 and RKO cells, although not in H630 cells, in which Ku70 silencing failed to activate either caspase 8 or caspase 3/7 (Supplementary Figures S3B and S3C); this

may be because FLIP downregulation following Ku70 depletion was less pronounced in this cell line (Figure 4b). Interestingly, given Ku70's role in regulating Bax-mediated apoptosis,6

Ku70 depletion still resulted in significant (albeit reduced) levels of apoptosis in Bax-null HCT116 cells, and this was again caspase 8-dependant (Figure 4e). SAHA- AND KU70 SIRNA-INDUCED

APOPTOSIS IS FLIP-DEPENDANT Using an HCT116 FLIP(L) overexpressing cell line (FL17), we obtained direct evidence for the importance of FLIP downregulation during SAHA-induced apoptosis. SAHA

failed to downregulate FLIP(L) in this cell line (Figure 6a) as it activated transcription of the exogenous transgene (unpublished observations). Lack of FLIP(L) downregulation in this cell

line correlated with significantly reduced levels of SAHA-induced apoptosis compared with the parental cell line as determined by PARP cleavage (Figure 6a) and flow cytometry (Figure 6b).

Of note, FLIP(L) overexpression did not prevent SAHA-induced cell cycle arrest in G2/M phase (Figure 6b), indicating that FLIP regulates the cytotoxic rather than the cytostatic effects of

SAHA. SAHA also sensitised CRC cells to apoptosis induced by rTRAIL and chemotherapeutic agents in a FLIP-dependant manner (Supplementary Figures S5A-D). These results establish direct

evidence for FLIP downregulation as a major mechanism of apoptosis induction by SAHA alone and in combination with other anti-cancer agents. Ku70 siRNA-induced apoptosis was also

significantly reduced in FLIP(L)-overexpressing cells (Figure 6c). To assess the importance of FLIP downregulation for the _in vivo_ effects of SAHA, we used the FL17 FLIP(L)-overexpressing

model. In both parental and FL17 xenografts, treatment with SAHA resulted in increased acetylation of histone H4, a marker of HDAC inhibition (Figure 6d). SAHA treatment resulted in potent

FLIP(L) downregulation in the parental xenografts and also decreased FLIP(L) expression in the FL17 xenografts. However, the levels of FLIP(L) expression that were maintained in SAHA-treated

FL17 tumours were comparable to those in vehicle-treated parental xenografts. Notably, SAHA treatment failed to inhibit the growth of FL17 xenografts, whereas the growth of the parental

xenografts was significantly inhibited by SAHA (Figure 6e). These results are the first to demonstrate that SAHA downregulates FLIP _in vivo_ and that FLIP downregulation is important for

its anti-tumour activity. INHIBITORS WITH ANTI-HDAC6 ACTIVITY REGULATE FLIP EXPRESSION AND KU70 ACETYLATION To identify the HDACs involved in regulating Ku70 acetylation, we used the HDAC

inhibitor Droxinostat,14 which, although less potent, has a more restricted activity than SAHA: Droxinostat is an inhibitor of HDACs 6 and 8, and (to a lesser extent) HDAC3;14 SAHA inhibits

HDACs 1, 2, 3, 6 and (to a lesser extent) 8.15 In agreement with earlier studies,16 we found that Droxinostat potently downregulated FLIP expression and did so at early (6 h) time points

post-treatment (Supplementary Figure S6A). However, unlike these earlier studies, we found that this downregulation was post-transcriptional, as this agent had no effect on FLIP mRNA

expression (Supplementary Figure S6B). Droxinostat-induced apoptosis correlated with FLIP downregulation (Supplementary Figure S6C), and FLIP downregulation was not caspase dependant

(Supplementary Figure S6D). Like SAHA, Droxinostat-induced apoptosis was caspase 8-dependant (Supplementary Figures S6D and 7A). Using a ‘caspase-trap’ assay,17 we demonstrated that caspase

8 rather than caspase 9 was the first caspase activated in HCT116 cells in response to treatment with both SAHA and Droxinostat for 4 h (Figure 7b). In addition, Droxinostat-induced

apoptosis was inhibited in FL17 cells (Figures 7c and d). Given the reported importance of Bax for HDAC inhibitor-induced apoptosis,6 it was notable that the inhibitory effects of caspase 8

silencing or FLIP overexpression on HDAC inhibitor-induced apoptosis were more profound than loss of Bax (Figures 7a and d). Furthermore, in contrast to a previous study,18 we found that

HDAC inhibitor-induced apoptosis was not p53-dependant in HCT116 cells (Figure 7d). We previously reported that apoptosis induction following siRNA-mediated FLIP silencing is primarily

driven by the TRAIL receptor DR5.3 In agreement with this, SAHA- and Droxinostat-induced cell death were both significantly attenuated when DR5 was silenced, and this effect was further

enhanced when DR4 was co-silenced with DR5 (Figure 7e). As Droxinostat and SAHA both inhibit HDAC6, we hypothesised that HDAC6 may be involved in regulating FLIP expression. To test this, we

used an HDAC6-selective inhibitor Tubacin.19 Both Tubacin and Droxinostat increased Ku70 acetylation to the same extent as SAHA (Figure 8a). By comparison, acetylation of Ku70 in response

to Entinostat, which inhibits HDACs 1–3, but not HDAC6,15 was significantly less than that induced by the other HDAC inhibitors (Figure 8a). In addition, siRNA-mediated depletion of HDAC6

resulted in significantly increased Ku70 acetylation (Figure 8b). Like SAHA and Droxinostat, Tubacin treatment resulted in rapid FLIP protein downregulation (Figure 8c), but had no

significant effect on FLIP mRNA expression (Figure 8d). Tubacin also caused an increase in acetylation of _α_-tubulin, a marker of HDAC6 inhibition, whereas acetylation of histone H4, a

marker of nuclear HDAC inhibition, was significantly lower following Tubacin treatment than following SAHA treatment (Figure 8c). In contrast, Entinostat failed to downregulate FLIP

expression in HCT116 cells after 6 h at a concentration that potently increased acetylation of histone H4, but had no effect on acetylation of _α_-tubulin (Figure 8e). In addition,

Tubacin-induced apoptosis was highly FLIP-dependant as determined by flow cytometry (Figure 8f), consistent with FLIP downregulation being a primary mechanism of apoptosis induction in

response to this agent. DISCUSSION We previously demonstrated that FLIP is an important regulator of apoptosis induction and drug resistance in CRC. 3, 20 We carried out a yeast-2-hybrid

screen to identify novel FLIP-interacting proteins, with the aim of identifying novel regulators of FLIP expression or function. This screen identified Ku70, a DNA repair protein that was

initially characterised as being critical for NHEJ.21 Ku70 was subsequently shown to have an apoptosis-regulating function through its ability to bind to and sequester Bax.6 Both the DNA-

and Bax-binding activities of Ku70 are acetylation dependant.6, 7 Acetylation of Ku70 at residues K539 and K542 in its C-terminus by CBP and PCAF disrupt its ability to inhibit Bax-mediated

apoptosis.6 Moreover, Ku70 was reported to have intrinsic DUB activity that inhibits Bax degradation via the UPS.8 We found that FLIP interacts with Ku70 via a region in the DED2, using a

site (R122) adjacent to the region that is functionally important for FLIP binding to FADD.11 Binding of FADD and procaspase 8 to FLIP was unaffected by mutation of R122, indicating that

Ku70 interacts with a region of FLIP that is distinct from the region with which it interacts with these DISC components. Furthermore, Ku70 did not bind to FLIP via the same region it binds

Bax, but rather via a region previously shown to be important for dimerisation with Ku80 (amino acids 430–496).22 Therefore, FLIP interacts with the same region of Ku70 with which it engages

Ku80 and does so using a region in DED2 not involved in its DISC recruitment. In addition, fractionation experiments suggested that similar to Bax, the primary sub-cellular location of the

FLIP–Ku70 interaction is cytoplasmic. Ku70 depletion resulted in significant decreases in FLIP expression. Furthermore, the decrease in FLIP expression following Ku70 silencing was because

of a decrease in protein stability. Treatment with the HDAC inhibitor SAHA resulted in the acetylation of Ku70 and disrupted its interaction with FLIP. Moreover, mimicking Ku70 acetylation

by mutating the residues K539 and K542 to glutamine resulted in reduced Ku70–FLIP binding. These lysine residues are present in the flexible C-terminal linker region adjacent to the region

of Ku70, which binds FLIP (amino acids 430–496). It is possible that acetylation of this flexible linker region causes a conformational change of Ku70 that disrupts binding of FLIP in the

adjacent 430–496 region, or that acetylation disrupts binding of an as yet unidentified binding partner (or partners) that is important for maintaining the Ku70–FLIP complex. Although we

found no evidence of FLIP acetylation following SAHA treatment, polyubiquitination of both FLIP(L) and FLIP(S) was increased, and both splice forms were rapidly downregulated in a

proteasome-dependant manner. A direct link between Ku70 and FLIP ubiquitination status was indicated by the increased levels of polyubiquitinated FLIP(L) and FLIP(S) in Ku70-silenced cells.

In contrast to numerous other studies,12, 13 we found no evidence that SAHA downregulated FLIP expression at the transcriptional level. However, our findings agree with a recent study in

breast cancer models, which also found that SAHA-induced FLIP downregulation was post-transcriptional.23 In addition, a related pan-HDAC inhibitor Panobinostat (LBH589) was recently reported

to cause FLIP polyubiquitination and proteasomal degradation in pancreatic cancer cells.24 Collectively, these findings suggest that SAHA causes Ku70 acetylation, resulting in the

disruption of its interaction with FLIP leading to degradation of FLIP by the UPS. Although Ku70 is a substrate for the HATs CBP and PCAF,6 the HDACs that regulate Ku70 acetylation have not

been previously characterised. In this study, we provide evidence that HDAC6 is a key deacetylase for Ku70 as, in addition to Vorinostat (inhibitor of HDAC1-3, 6 and 8)15 and Droxinostat

(inhibitor of HDAC3, 6 and 8),14 the HDAC6-specific inhibitor Tubacin19 potently increased the acetylation of Ku70. Moreover, both Droxinostat and Tubacin also caused rapid FLIP

downregulation. In contrast, Entinostat, which inhibits HDAC1–3, but has no activity against HDAC6,15 failed to downregulate FLIP at early time points and had less impact on Ku70

acetylation. During revision of this manuscript, another study was published that also found that HDAC6 deacetylates Ku70.25 HDAC6 is a unique HDAC that has key roles in regulating protein

turnover by the proteasome through its regulation of HSP90 and by the aggresome through its ability to recruit polyubiquitinated proteins to the tubulin cytoskeleton.26 Thus, this study

identifies a further potential role for HDAC6 in regulating protein stability through its ability to deacetylate Ku70, thereby stabilising FLIP. By deacetylating Ku70, HDAC6 may also

regulate Bax and possibly other as yet unidentified Ku70-binding partners. Although a number of studies have shown that HDAC inhibitor-mediated downregulation of FLIP sensitises various

cancer cell lines to death ligands, such as TRAIL,23, 27, 28 to our knowledge, no previous studies have directly examined whether FLIP downregulation is a sufficient death signal for

apoptosis induction when these agents are administered as single agents. We found that FLIP downregulation in response to HDAC inhibitors results in caspase 8- and DR5-mediated apoptosis,

phenocopying the mechanism of apoptosis that we previously observed in CRC cells following siRNA-mediated downregulation of FLIP.3 We also demonstrate for the first time that SAHA

downregulates FLIP _in vivo_ and that FLIP(L) overexpression abrogates SAHA's _in vivo_ anti-tumour activity. FLIP(L) overexpression or caspase 8 downregulation had a greater inhibitory

effect on HDAC inhibitor-induced apoptosis than loss of Bax, suggesting that the extrinsic apoptotic pathway is at least as important as the intrinsic pathway in mediating the effects of

HDAC inhibitors in CRC cells. From a cancer therapeutics perspective, these results suggest that HDAC inhibitors with anti-HDAC6 activity act as efficient post-transcriptional suppressors of

FLIP expression in CRC. HDAC inhibitors are promising anti-cancer therapeutics that have demonstrated pre-clinical and clinical activities in haematological and solid cancers, and SAHA was

the first of this class of compound to be FDA approved.29, 30, 31, 32, 33 There have been several early phase clinical trials in advanced, chemotherapy-resistant CRC examining SAHA in

combination with standard 5-Fluorouracil (5-FU)-based chemotherapy.34, 35, 36 In one of these studies, 21/38 5-FU-refractory patients had stable disease and 1 had a partial response.34 The

plasma concentrations of SAHA achieved in these patients were similar to the concentrations that we find are sufficient to downregulate FLIP. Of note, we found that SAHA synergized with both

5-FU and oxaliplatin to induce apoptosis in CRC cells; however, this synergy was abolished in cells overexpressing FLIP(L). Thus, FLIP and components of the extrinsic pathway, such as

caspase 8, may be useful predictive biomarkers for the targeted use of HDAC inhibitors in CRC. In conclusion, we provide evidence that Ku70 regulates FLIP ubiquitination and that HDAC

inhibitor-mediated acetylation of Ku70 disrupts the interaction between FLIP and Ku70 resulting in degradation of FLIP via the UPS and induction of caspase 8-dependant apoptosis (summarised

in Figure 9). MATERIALS AND METHODS REAGENTS The following reagents were used: Vorinostat (Zolinza, SAHA; Selleck Chemicals, Suffolk, UK); Droxinostat

(4-(4-chloro-2-methylphenoxy)-N-hydroxybutanamide, compound #5809354) and its inactive analogue 4-(4-chloro-2-methylphenoxy)-N-(3-ethoxypropyl)butanamide (compound #7271570, ChemBridge

Corporation, San Diego, CA, USA). Tubacin was a kind gift from Dr. Ralph Mazitschek and Dr Stuart Schreiber (Howard Hughes Medical Institute, Broad Institute of Harvard and MIT). Entinostat

(MS-275) was synthesised in the laboratory as previously described.37, 38 Cycloheximide and MG132 (Sigma-Aldrich, Dorset, UK). Biotinylated z-VAD-fmk (Val-Ala-Asp-CH2F) and immobilised

Streptavidin slurry were purchased from MP Biomedicals (Cambridge, UK) and Thermo Fisher Scientific (Leicestershire, UK), respectively. CELL CULTURE HCT116, H630, HT29 and RKO human CRC cell

lines were used as previously described.3, 39 Matched isogenic p53 and Bax-null HCT116 cell lines were kindly provided by Professor B Vogelstein (Johns Hopkins University School of

Medicine, Baltimore). FL17 cells were generated and cultured as previously described.20 EXPRESSION CONSTRUCTS Flag-tagged FLIP(L), FLIP(S) and Ku70 expression constructswere generated in the

pCMV-3Tag-6 vector (Agilent Technologies, Berkshire, UK). The GST-tagged FLIP(S) expression construct was generated in the pGEX6P-3 vector (GE Healthcare, Herts, UK). Mutagenesis was

carried out using the KOD Extreme polymerase (Novagen, Nottingham, UK), with the template plasmid digested using _DpnI_ (New England Biolabs, Herts, UK). WESTERN BLOTTING AND SUB-CELLULAR

FRACTIONATION Western blots were carried out as previously described.3 Isolation of nuclear and cytosolic fractions was carried out by lysing the cells for 10 min on ice in buffer A (10 mM

HEPES, 1.5 mM MgCl2, 10 mM KCL, 0.5 mM DTT, 0.5% NP40, pH7.9) followed by centrifugation at 3000 r.p.m. for 10 min. The supernatants were retained as the cytosolic fractions, and the pellets

were subjected to further lysis in buffer B (5 mM HEPES, 1.5 mM MgCl2, 0.2 mM EDTA, 0.5 mM DTT, 26% glycerol (v/v), pH 7.9). NaCl was added to a final concentration of 300 mM, and the

samples were homogenized using a Dounce homogenizer (VWR, Dublin, Ireland). After a 30-min incubation on ice, the lysates were centrifuged for 20 min at 24 000 _g_, and the resulting

supernatants collected as the nuclear fractions. ANTIBODIES _Mouse monoclonal (Western)_: FLIP (NF6; Alexis, San Diego, CA, USA), Caspase 8 (12F5; Alexis) and PARP (eBioscience, San Diego,

CA, USA), _β_-Actin and Flag-HRP (Sigma, Dorset, UK), Ku70, ITCH (both BD Transduction Laboratories, Oxfordshire, UK) and Noxa (Abcam, Cambridge, UK). _Rabbit polyclonal (Western and IP):_

Caspase 9, caspase 3, acetylated lysine, acetylated-_α_-tubulin, XIAP, Bcl-2, Bcl-XL, Mcl-1, Bax, Bak, Bid, Bim, PUMA (Cell Signaling Technology, Beverly, MA, USA), c-FLIP (H202), Ku70

(Santa Cruz Biotechnology, Santa Cruz, CA, USA) and Hyperacetylated Histone H4 (Millipore, Watford, UK). Horseradish peroxidase-conjugated sheep anti-mouse and sheep anti-rabbit secondary

antibodies were used as appropriate (Amersham, Buckinghamshire, UK). YEAST-2-HYBRID The Matchmaker GAL4-based yeast-two-hybrid system was used (Clontech, Saint Germain en Laye, France).

Human FLIP(L) was used as the bait protein and expressed as a fusion to the GAL4 DNA-binding domain in pGBKT7 vector. A cDNA library generated from HCT116 cells was cloned into pGADT7 prey

vector. The yeast-two-hybrid screen for FLIP(L)-interacting proteins was carried out according to the manufacturer's instructions. IMMUNOPRECIPITATION (IP) REACTIONS Protein lysates

were prepared using CHAPS (10 mM HEPES, 150 mM NaCl, 1% CHAPS, pH 7.4) or NP-40 (0.2% NP-40, 20 mM Tris-HCL (pH 7.4), 150 mM NaCl, 10% glycerol) buffers. Lysates (0.5–2 mg) were pre-cleared

overnight with sheep anti-rabbit IgG Dynalbeads (Invitrogen, Paisley, UK). Antibodies (1–2 _μ_g) were conjugated with sheep anti-rabbit IgG Dynal beads for at least 1 h and then washed

before incubation with pre-cleared lysates for at least 4 h. After several washes, Dynal beads were resuspended in Laemmli loading buffer and heated at 95 °C for 5 min before immunoblot

analysis. Ubiquitin IP experiments were carried out using the Ubiquitin Enrichment kit (Thermo Scientific, Surrey, UK) according to the manufacturer's instructions. RECOMBINANT PROTEIN

PURIFICATION AND GST PULL-DOWNS GST and GST-tagged FLIP(S) were expressed in IPTG-stimulated BL21 bacteria. Bacterial cell lysates were purified using Glutathione-Sepharose beads (GE

Healthcare Bio-Sciences AB, Uppsala, Sweden) and dialysed using Slide-A-Lyzer Dialysis Cassettes (Thermo Scientific). For pull-downs, GST-tagged proteins (10 _μ_g) were conjugated to

Glutathione-Sepharose beads and incubated with pre-cleared protein lysates (500 _μ_g) for 2 h at 4 °C with constant mixing. Beads were washed several times and resuspended in Laemmli loading

buffer before western blot analysis. FLIP PEPTIDE ARRAY ANALYSIS FLIP peptide arrays were generated as previously described9 using the Genbank sequence U97074.1. The arrays were blocked in

5% milk/PBS/0.5% Tween-20 for 1 h and then overlaid with lysates prepared from the cells transfected with Flag-tagged Ku70 or EV. Following several washes (PBS/0.5% Tween-20), bound

Flag-tagged Ku70 was detected by immunoblotting. CASPASE ‘TRAP’ ASSAY This assay was performed as previously described.17 FLOW CYTOMETRY Apoptosis was determined using propidium iodide (PI)

staining to evaluate the percentage of cells with DNA content <2N as previously described.3 For annexin V/PI analysis, cells were harvested and analysed according to the

manufacturer's instructions (BD Biosciences, Oxford, UK). SIRNA TRANSFECTIONS The non-silencing control (SC) siRNA, FLIP-, caspase 8-, caspase 9, DR4- and DR5-targeted siRNAs were

obtained from Dharmacon (Chicago, IL, USA) and were the same as those previously described.3, 40 siRNAs targeting Ku70 and HDAC6 were obtained from Qiagen (West Sussex, UK). siRNA

transfections were carried out using OligofectAMINE (Invitrogen). QUANTITATIVE PCR (Q-PCR) RNA was isolated using the RNA STAT-60 reagent (Biogenesis, Poole, UK) and reverse transcribed

using Moloney murine leukemia virus-based reverse transcriptase kit (Invitrogen). Q-PCR analysis of the _FLIP_ gene expression was performed using the SYBR Green method or TaqMan Gene

Expression Assays (Applied Biosystems, Foster City, CA, USA). ANIMAL MODEL EXPERIMENTS Female BALB/c nude mice were maintained as previously described.3 All experiments were carried out in

accordance with the Animals (Scientific Procedures) Act, 1986 under a Project Licence (PPL 2590b) approved by the Department of Health, Social Services and Public Safety, Northern Ireland.

Mice were implanted sub-cutaneously on each flank with 2 × 106 HCT116 or FL17 cells using Matrigel (BD, Oxford, UK). After the tumours reached ∼100 mm3, mice were randomised to receive

vehicle control (10% DMSO/45% PEG400) or 100 mg/kg Vorinostat delivered IP on a 5-day on/2-day off schedule for 2 weeks. Tumour volumes were determined as previously described.3 To extract

protein, xenografts were homogenized in RIPA buffer. CASPASE ACTIVITY ASSAY Caspase-8 or caspase-3/7-GLO reagents (25 _μ_l) (Promega, Southampton, UK) were incubated with 1–10 _μ_g of

protein lysate diluted in cell culture medium in a total volume of 50 _μ_l for 1–2 h at room temperature. Luciferase activity was then determined using a luminometer. STATISTICAL ANALYSIS

Student's _t_-test was used for the statistical analysis; *denotes _P_<0.05;. **denotes _P_<0.01; ***denotes _P_<0.001; and ns denotes not significant compared with control.

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apoptosis in type II colorectal cancer cells. _Oncogene_ 2009; 28: 63–72. Article  CAS  Google Scholar  Download references ACKNOWLEDGEMENTS This work was supported by a grant from Cancer

Research UK. EK was supported by a studentship from the Department for Employment and Learning, NI. AUTHOR INFORMATION Author notes * E Kerr and C Holohan: These authors contributed equally

to this work. * P G Johnston and D B Longley: These authors contributed equally to this work. AUTHORS AND AFFILIATIONS * Centre for Cancer Research and Cell Biology, School of Medicine,

Dentistry and Biomedical Science, Queen's University Belfast, 97 Lisburn Road, Belfast BT9 7BL, Northern Ireland, UK, E Kerr, C Holohan, K M McLaughlin, J Majkut, S Dolan, K Redmond, J

Riley, K McLaughlin, I Stasik, M Crudden, S Van Schaeybroeck, C Fenning, M Sgobba, D Haigh, P G Johnston & D B Longley * Department of Biochemistry, Cell Biology Laboratory, University

College Cork, Cork, Republic of Ireland R O'Connor & P Kiely Authors * E Kerr View author publications You can also search for this author inPubMed Google Scholar * C Holohan View

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permissions ABOUT THIS ARTICLE CITE THIS ARTICLE Kerr, E., Holohan, C., McLaughlin, K. _et al._ Identification of an acetylation-dependant Ku70/FLIP complex that regulates FLIP expression

and HDAC inhibitor-induced apoptosis. _Cell Death Differ_ 19, 1317–1327 (2012). https://doi.org/10.1038/cdd.2012.8 Download citation * Received: 15 July 2011 * Revised: 21 December 2011 *

Accepted: 21 December 2011 * Published: 10 February 2012 * Issue Date: August 2012 * DOI: https://doi.org/10.1038/cdd.2012.8 SHARE THIS ARTICLE Anyone you share the following link with will

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content-sharing initiative KEYWORDS * Ku70 * FLIP * caspase 8 * HDAC inhibitors * colorectal cancer * apoptosis