High-frequency relapse remains a clinical hurdle for complete remission of T-cell acute lymphoblastic leukemia (T-ALL) patients, with heterogeneous dysregulated signaling profiles—including of Raf-MEK-ERK and Akt-mTORC1-S6K signaling pathways—recently being implicated in disease outcomes. Here we report that GM-CSF/IL-3/IL-5 receptor common β-chain-associated protein (CBAP) is highly expressed in human T-ALL cell lines and many primary tumor tissues and is required to bolster leukemia cell proliferation in tissue culture and for in vivo leukemogenesis in a xenograft mouse model. Downregulation of CBAP markedly restrains expansion of leukemia cells and alleviates disease aggravation of leukemic mice. Transcriptomic profiling and molecular biological analyses suggest that CBAP acts upstream of Ras and Rac1, and functions as a modulator of both Raf-MEK–ERK and Akt-mTORC1 signaling pathways to control leukemia cell growth. Specifically, CBAP facilitated Akt-dependent TSC2 phosphorylation in cell-based assays and in vitro analysis, decreased lysosomal localization of TSC2, and elevated Rheb-GTP loading and subsequent activation of mTORC1 signaling. Taken together, our findings reveal a novel oncogenic contribution of CBAP in T-ALL leukemic cells, in addition to its original pro-apoptotic function in cytokine-dependent cell lines and primary hematopoietic cells, by demonstrating its functional role in the regulation of Akt-TSC2-mTORC1 signaling for leukemia cell proliferation. Thus, CBAP represents a novel therapeutic target for many types of cancers and metabolic diseases linked to PI3K-Akt-mTORC1 signaling.
T-cell acute lymphoblastic leukemia (T-ALL) is a high-risk leukemia subtype that accounts for 10–15% of pediatric and 25% of adult ALL cases . Although the remission rate has significantly improved over the past decade, T-ALL remains a therapeutic challenge due to the high frequency of induction failure  and early relapse, which is mostly resistant to further treatment . Molecular abnormalities that have frequently been reported in T-ALL include activation mutations of Notch1 and JAK1 and inactivation mutations of PTEN and FBXW7 . The PI3K-Akt-mTOR signaling axis is an important contributory pathway for T-cell leukemia [5, 6]. It is frequently upregulated in patients with T-ALL and its activation is correlated with poor prognosis, therapeutic resistance, and disease relapse [5, 7,8,9]. Deletion of mTOR complex-1 (mTORC1) in a T-ALL mouse model resulted in profound cell-cycle arrest and efficient eradication of T-ALL cells [10, 11], suggesting that mTORC1 can integrate signals from the PI3K-Akt and MEK–ERK signaling pathways to activate downstream components responsible for tumor cell growth and metabolism .
Tuberous sclerosis is a hereditary syndrome characterized by hamartoma formation in various tissues, which is caused by mutations in either TUBEROUS SCLEROSIS COMPLEX 1 (TSC1) or TSC2 genes . The tuberous sclerosis complex (TSC) is typically composed of TSC1, TSC2, and Tre2-Bub2-Cdc16 domain family member 7 (TBC1D7) subunits. It can be regulated through the PI3K-Akt, Ras-ERK-RSK1, LKB1-AMPK, IKKβ, GSK3β, and HIFα-REDD1 signaling pathways, all of which can be activated by several stimuli such as growth factors, inflammation, energy stress, hypoxia, and the Wnt pathway [14, 15]. Thus far, the TSC is the only known direct inhibitor for activity of the small GTPase Ras homolog enriched in brain (Rheb), which is a critical activator for mTORC1 signaling, i.e., the major promoter of cellular growth and metabolism [14, 16,17,18,19]. Therefore, the TSC represents a key controller of the Rheb-mTORC1 signaling network, which is commonly activated via upstream signaling dysregulation due to oncogenic mutation of genes or post-translational protein modifications in tumors. Suppression of Rheb-mTORC1 activation is dependent on translocation of the TSC to the lysosomal surface [20, 21].
CBAP, also known as TMEM102 (Gene ID:284114), was first identified as an interacting protein of the GM-CSF/IL-3/IL-5 receptor common β-chain and participates in cytokine deprivation-induced apoptosis . Bioinformatics analyses have revealed that CBAP is a member of the Mab21 subfamily that lies within the nucleotide transferase protein fold superfamily . Our previous studies have demonstrated that CBAP participates in chemokine-enhanced T-cell migration and adhesion  and in T-cell receptor engagement-induced phosphorylation of ZAP-70 and PLCγ1 . Since CBAP proteins are highly expressed in many established tumor cell lines, including T-cell leukemia, we examined whether CBAP is also involved in leukemia proliferation and tumorigenesis. By manipulating the expression of the gene encoding CBAP with knockdown/knockout strategies in T-ALL cells, we demonstrate that CBAP participates in tumor cell growth and leukemogenesis in mice. Importantly, we further reveal the underlying mechanism by which CBAP facilitates Akt-mediated suppression of TSC2, which is accompanied by an increase of Rheb-GTP loading and activation of the mTORC1-signaling pathway to promote leukemogenesis.
CBAP enhances the growth of leukemia cells
We first observed that CBAP protein expression was higher in a Jurkat T-ALL cell line than in purified human peripheral T lymphocytes (CD3+ T cells) (Fig. 1a), but these latter conversely expressed a higher level of CBAP mRNA than Jurkat T cells (Supplementary Fig. 1a). Interestingly, CBAP protein levels were elevated in all four T-ALL cell lines analyzed, but only in one of the acute myeloid leukemia cell lines we examined (HL60) (Fig. 1b). To confirm this overexpression of CBAP in leukemic cells, we further verified CBAP protein expression in bone marrow (BM) biopsy sections of T-ALL patients (Table 1) by immunohistochemical (IHC) staining. IHC staining for CD3 was positive and diffuse, confirming that most of the tumor cells in the BM sections are T cells (Fig. 1c, middle row), and only a few were positive in the BM sections from control patients (Fig. 1d, middle row). CBAP protein was diffusely overexpressed in T-ALL tumor cells (Fig. 1c, upper row) when compared with the control (anemia patients), with these latter showing no obvious CBAP expression in normal BM biopsy sections (Fig. 1d, upper row). We also assessed C-Myc protein expression as a downstream marker of mTORC1 activation and found strong nuclear C-Myc staining in two T-ALL patients but not in the control patients (Fig. 1c, bottom row). Therefore, we hypothesized that higher CBAP protein expression may confer a beneficial effect on T-ALL cells. To investigate this possibility, we generated a CBAP knockout (KO) Jurkat cell line using the CRISPR/Cas9 technique, and confirmed the absence of CBAP expression by immunoblotting (Supplementary Fig. 1b, left panel). These CBAP-KO Jurkat cells exhibited reduced chemokine-induced migratory activity (Supplementary Fig. 1c), which is consistent with our previous observation . Importantly, CBAP downregulation by either one of two different shRNA knockdown plasmids (sh-CBAP no. 1 and no. 2), or by CRISPR/Cas9 plasmid–mediated KO, caused a significant and consistent reduction in the proliferation rate of Jurkat cells (Fig. 1e), as well as in CCRF-CEM T-ALL cells (Supplementary Figs. 1b, right panel, and 1d). We compared control and CBAP-KO Jurkat cells in a cell-cycle analysis using a bromodeoxyuridine (BrdU) and 7-aminoactinomycin D (7-AAD) double-labeling method and found a significant increase in the number of cells undergoing G0/G1 in CBAP-KO Jurkat cells (Fig. 1f), but no significant difference in the percentages of cells undergoing sub-G0/G1 (i.e., apoptotic) stages (Supplementary Fig. S1e) or in the number of annexin V+ apoptotic cells (Supplementary Fig. S1f), suggesting that CBAP KO mainly affects the cell proliferation rate in Jurkat cells. This finding is consistent with our observation that levels of bcl-2 protein, a major anti-apoptotic protein in hematopoietic cells, increased in CBAP-KO Jurkat cells (Supplementary Fig. S1g).
CBAP is involved in leukemogenesis in vivo
We next investigated the impact of CBAP loss on the leukemogenic potential of Jurkat cells in vivo. We established a leukemic mouse model by transplanting five million Jurkat cells expressing a firefly luciferase reporter gene into NOD-SCID-IL2Rγc-deficient (NSG) mice. At 14 and 21 days after transplantation (D), luminescence was significantly lower in mice transplanted with sh-CBAP-expressing Jurkat cells compared with control (sh-Ctrl) Jurkat cells (Fig. 2a). One mouse died at D14 and another one died at D21 in the control group (Fig. 2a, upper row). However, transplanted mice could live up to D42 under conditions of reduced CBAP expression (Fig. 2a, lower row). At D18, representative proportions of human CD45+ cells were significantly higher in the BM, peripheral blood leukocytes (PBLs), and spleen of mice that received control (sh-Ctrl) Jurkat cell transplants (Supplementary Fig. S2a). Leukemic mice engrafted with sh-Ctrl Jurkat cells displayed a splenomegaly phenotype (Supplementary Fig. S2b), and became moribund with severe hind limb paralysis before death. Notably, although all mice eventually succumbed to T-ALL, the mice transplanted with sh-CBAP Jurkat cells developed leukemia over a much longer latency period than those transplanted with sh-Ctrl Jurkat cells (Fig. 2b and Supplementary Fig. S3a). Mice transplanted with CBAP-KO Jurkat cells also exhibited a significantly prolonged latency period compared to those transplanted with the control (cr-Ctrl) Jurkat cells (Fig. 2c and Supplementary Fig. S3b). Introduction of CBAP-GFP fusion protein into CBAP-KO cells could partially rescue cell proliferation in tissue culture (Supplementary Fig. S3c), and leukemogenesis in vivo (Fig. 2c, green line), further supporting the importance of CBAP in leukemic cell proliferation. Moreover, shRNA knockdown of CBAP in CCRF-CEM T-ALL cells also consistently produced cells that exhibited longer disease latency in this leukemic mouse model compared to the control (Fig. 2d and Supplementary Fig. S3d), suggesting that CBAP expression increases the oncogenic activity of leukemia cells in vivo.
Downregulation of CBAP expression in T-ALL cells results in reduced aerobic glycolysis and energy metabolism
We next sought to examine CBAP-regulated gene expression signatures in leukemia using a next generation sequencing technique for RNA (RNA-seq). Total mRNA was isolated from two types of CBAP-expressing Jurkat cells (sh-Ctrl cells and CBAP-KO cells expressing CBAP-GFP, with these latter referred to as CBAP-reconstituted cells) and two types of CBAP-deficient Jurkat cells (sh-CBAP cells and CBAP-KO cells expressing GFP). We then generated genome-wide transcriptome profiles for these cell lines (for method, see supplementary information). The RNA-seq data have been deposited in NCBI Gene Expression Omnibus (GEO) database (accession number: GSE 69511). Gene sets that presented highly reduced expression in the CBAP-deficient cells were related to metabolism, as assessed by KEGG (Kyoto Encyclopedia of Genes and Genomes) categories (Supplementary Table S1), and these metabolic genes represented over 60% of the significantly enriched pathways (false discovery rate (FDR) q value < 0.25) (Fig. 3a). Of interest, among these downregulated metabolic pathways, most of the gene sets belonged to subgroups linked to carbohydrate metabolism (35.7%) or amino acid metabolism (32.1%) (Table S1). A gene set enrichment analysis (GSEA) showed that the gene expression pattern in CBAP-deficient leukemia cells was significantly correlated with signatures of TSC1/TSC2-dependent rapamycin-sensitive genes  (Fig. 3b). Furthermore, the most represented genes (P < 0.05), i.e., pertaining to the mTORC1-induced gene set, encoded proteins involved in the regulation of glycolysis (i.e. Aldoa, Pfkl, Pfkp, Pgm1, Glut1, and Tpi1) and lipid biosynthesis (i.e. Acly, Fasn, Gdpd1, Hsd17b12, and Slc25a1)  (Supplementary Table S2). To further validate the results of our transcriptomic analysis, qRT-PCR experiments on expression levels of the aforementioned genes also supported that mRNA levels of many enzymes involved in glycolysis and lipid biosynthesis pathways were significantly reduced (Fig. 3c). Protein levels of two critical transcriptional factors downstream of mTORC1—c-Myc, which is important for protein translation, and HIF1α, which is important for energy metabolism—were also reduced in the CBAP-deficient Jurkat cells (Fig. 3d). Finally, critical metabolites in glycolysis (lactate) and glutaminolysis (α-ketoglutarate) were also reduced in CBAP-KO cells (Fig. 3e), suggesting that indeed the activities of several catabolic pathways such as aerobic glycolysis and glutaminolysis are diminished in the absence of CBAP proteins, resulting in reduced cell growth. These biochemical evidences prompted us to investigate whether CBAP participates in the proliferation of leukemia cells via the mTORC1 pathway since mTORC1 signaling is a well-known master regulator of protein translation, cell growth, metabolism, and cancer cell proliferation . Treatment with rapamycin, a specific mTORC1 inhibitor, efficiently suppressed phosphorylation of p70S6K (a marker of mTORC1 activation, Fig. 3f) and cell growth (Fig. 3g) in both control and CBAP-KO Jurkat cell lines, demonstrating that activation of mTORC1 signaling is essential for Jurkat cell leukemic growth. Although p70S6K phosphorylation was almost completely inhibited in both control and CBAP-KO cells using 1 nM of rapamycin (Fig. 3f), loss of CBAP and rapamycin treatment had an additive effect in terms of growth suppression (Fig. 3g and Supplementary Fig. S5a). Therefore, apart from the mTORC1 signaling pathway, CBAP might act on another growth pathway (see below).
Loss of CBAP simultaneously attenuates both Raf-MEK-ERK–RSK and mTORC1-S6K signaling
Since both PI3K-Akt and Raf–MEK–ERK signaling are reported to be crucial for mTORC1 activation [12, 14], we investigated the potential involvement of CBAP in these signaling pathways. First, CBAP KO resulted in a drastic increase of Akt phosphorylation at residues T308 and S473, whereas downstream mTORC1-S6K-4E-BP1 signaling was downregulated in CBAP-KO cells, as demonstrated by the decreased phosphorylation of TSC2 (T1462, S939) and p70S6K (T389), but not 4EBP1 (T37/46) (Fig. 3h). The relative phosphorylation of residue S9 of GSK3β compared to total GSK3β levels was not altered (Fig. 3h). Notably, compared to CBAP-KO cells, phosphorylation of TSC2, p70S6K, and 4EBP1 was all significantly enhanced in CBAP-reconstituted cells (Fig. 3h and Fig. S4 for quantification data), whereas Akt phosphorylation in these CBAP-reconstituted cells had returned to the level of control cells (Fig. 3h and Fig. S4a). These data are consistent with the hypothesis proposed by Guertin and Sabatini [28, 29] that a negative feedback inhibition loop may exist to regulate PI3K/Akt activity as a result of increased p70S6K activity. CBAP deletion also downregulated Raf-MEK-ERK signaling, as judged by decreased phosphorylation of cRaf (at residue S338, but not S259), MEK1/2 (S217/221), ERK1/2 (T202/Y204), and p90RSK (S380) (Fig. 3i, lane 2, and Supplementary Fig. S4b). Restoration of CBAP expression partially restored the phosphorylation levels of these proteins (Fig. 3i, lane 4, and Supplementary Fig. S4b). These data suggest that CBAP plays a critical role in regulating both the Akt-mTORC1 and Raf-MEK-ERK signaling pathways.
To further investigate which signaling pathway is essential for T-ALL cell growth, we treated cells with the specific inhibitors MK2206 and U0126 that target the Akt and MEK signaling pathways, respectively. Both inhibitors effectively suppressed tumor growth in tissue cultures in a time- and dose-dependent manner (Fig. 3j, k), indicating that both pathways are important for cell growth. As for the effect of rapamycin treatment on mTORC1 activation, 1 μM MK2206 or 1 μM U0126 could almost completely inhibit Akt activity or MEK/ERK activity, respectively, in both control and CBAP-KO cells (see below, Fig. 4d, e), and loss of CBAP always had an additive effect to the inhibitor in terms of suppressing cell growth (Fig. 3j, k, see also Figs. S5b and S5c). Furthermore, suppression of leukemia cell growth in Jurkat cell-engrafted leukemic mice by either rapamycin or U0126 treatment or a combination of both further supports the importance of both the Raf-MEK-ERK and Akt-mTORC1 pathways in leukemia proliferation, especially since a combination of both inhibitors had an additive effect in vivo (Supplementary Fig. S6).
Crosstalk between the PI3K-Akt and ERK–RSK pathways in T-ALL cells
Next, we set out to investigate the effect of CBAP on other upstream components involved in the Akt/TSC2 and Raf-MEK-ERK pathways. We measured levels of GTP-loaded Ras and Rac1 by pull-down assays with the Ras-binding domain (RBD) of Raf1 and with the p21-binding domain (PBD) of Pak1 , respectively. Compared to GTPγS-bound Ras (Fig. 4a) and GTPγS-bound Rac1 (Fig. 4b), only small amounts of Ras and Rac1 were GTP-loaded (lane 1 vs. lane 3). However, we found that these amounts were further reduced in CBAP-deficient cells compared to cr-Ctrl cells (lane 2 vs. lane 1). Conversely, in accordance with the effect of CBAP deficiency on Akt activity, we found that loss of CBAP increased phosphorylation of the p85 subunit of PI3K (Fig. 4c). However, it remains to be explored whether these two signaling pathways have a common upstream regulator.
ERK  and RSK  have been shown to directly act on TSC2 and mTORC1 phosphorylation, respectively, in other cancer types, and that crosstalk exists between these pathways has been demonstrated . As this crosstalk may bias our interpretation of the effect of CBAP KO, we investigated the potential crosstalk between these pathways in T-ALL leukemia cells using pathway-specific inhibitors. When control cells were treated with the Akt inhibitor, MK2206, Akt phosphorylation was significantly reduced and phosphorylation levels of TSC2 and p70S6K also decreased, whereas ERK1/2 phosphorylation was not altered (Fig. 4d and Supplementary Fig. S4c for quantification data). However, when we inhibited MEK1/2 in control cells using U0126, ERK1/2 and p90RSK phosphorylation was significantly abrogated and Akt phosphorylation was increased (Fig. 4e), probably due to relief of the hypothetical cross-inhibitory signal from the Raf-MEK-ERK pathway . This upregulated Akt phosphorylation in turn led to increased phosphorylation of TSC2 and p70S6K, which was especially evident when cells were treated with 0.1 μM U0126 (Fig. 4e and Supplementary Fig. S4d). Notably, increased phosphorylation of TSC2 and p70S6K was not observed in the absence of CBAP (Fig. 4e, comparing lanes 4 and 5, and Supplementary Fig. S4d) or in the co-treatment with MK2206 (Fig. 4f, comparing lane 2 to lane 5), suggesting that the crosstalk between the Raf-MEK-ERK and Akt-mTORC1 pathways occurs mainly through the Akt protein or its upstream regulator PI3-K in Jurkat cells (see Fig. 4g), but does not directly affect TSC2 or mTORC1 proteins [31, 32]. Taken together, Akt appears to be the predominant kinase controlling both TSC2 phosphorylation and downstream mTORC1 activation in leukemic Jurkat cells.
CBAP facilitates TSC2 phosphorylation by Akt according to cell-based assays and in vitro analysis
Our aforementioned data suggest that CBAP is involved in the Akt-mTORC1 signaling pathway by controlling Akt-mediated TSC2 phosphorylation. We further investigated this dependency of Akt-mediated TSC2 phosphorylation on the presence of CBAP in HEK293T cells. We knocked out the CBAP gene in HEK293T cells using a CRISPR/Cas9-mediated strategy and then transiently expressed myc-Akt1 and Flag-TSC2/myc-TSC1 plasmids in this cell background (Fig. 5a, lower panel). We found the phosphorylated level of exogenously expressed Flag-TSC2 to be significantly elevated in the presence of CBAP and exogenous Akt, whereas it was not increased in HEK293T cells lacking either Akt (Fig. 5a, upper panel, lane 1) or CBAP (Fig. 5a, upper panel, lane 5), suggesting that CBAP-mediated facilitation of Akt-dependent TSC2 phosphorylation could be recapitulated in HEK293T cells using exogenous proteins. Additionally, we explored whether CBAP directly facilitates Akt-mediated TSC2 phosphorylation using an in vitro kinase assay. As shown in Fig. 5b, immunoprecipitated phospho-Akt from CBAP-KO cells possessed a limited ability to phosphorylate recombinant Flag-TSC2 protein that had been produced using an in vitro transcription/translation (IVT) system. When bacterially-derived recombinant GST-CBAP protein was added to the system, levels of phosphorylated TSC2 increased in a dose-dependent manner in vitro (Fig. 5b, lanes 4 and 5). However, when non-phosphorylated Akt was used in the in vitro kinase assay, the enhancing effect of CBAP disappeared (compare lane 4 and lane 6 in Fig. 5b), suggesting that CBAP directly activates Akt to phosphorylate TSC2. We also monitored the changing GTP-loadings of the small G protein Rheb as an independent measure of TSC2 complex inactivation by upstream Akt signals. Using an antibody that can specifically recognize GTP-loaded Rheb , we directly measured the nucleotide-binding states of Rheb in total cell lysates of leukemic Jurkat cells. As shown in Fig. 5c, under steady state conditions, the levels of Rheb-GTP (i.e., active Rheb) were decreased in CBAP-KO cells (lane 2) compared to both control cells (lane 1) and CBAP-reconstituted cells (CG5, lane 3). We further explored whether CBAP can regulate the levels of Rheb-GTP in the reconstituted HEK293T cells with exogenous proteins. After transfection with the Akt plasmids shown in Fig. 5d, cell lysates were immunoprecipitated with the anti-Rheb-GTP antibody and the immunoprecipitates were subjected to immunoblotting with an anti-Flag antibody. We found that there was an increase in the level of the active, GTP-bound, exogenous Flag-Rheb in control HEK293T cells (Fig. 5d, compare lanes 1 and 2). In contrast, Akt did not increase the levels of Rheb-GTP in the absence of CBAP (Fig. 5d, compare lanes 3 and 4). Thus, our data strongly suggest that CBAP can directly act on the Akt/TSC/Rheb axis to regulate downstream activation of mTORC1 signaling.
CBAP is also required for insulin-induced TSC2 phosphorylation and translocation
Since TSC2 functions as a signaling hub for many converging stimuli (including growth factors, stress, and metabolites, among others) and regulates downstream mTORC1-mediated cell metabolism, we wondered whether CBAP can also modulate Akt-dependent TSC2 phosphorylation and translocation via growth factors such as insulin. In CRISPR/Cas9-mediated CBAP-KO Hela cells, we found that insulin-stimulated phosphorylation of TSC2 and p70S6K was diminished but phosphorylation of Akt (S473 and T308) was elevated compared to control cells, suggesting that CBAP is also crucial for mediating insulin-stimulated Akt-mTORC1 signaling (Fig. 6a). Given that TSC2 phosphorylation has been reported to functionally inactivate the TSC by triggering its translocation into the cytosol and away from Rheb and mTORC1 at the lysosomal membrane [20, 34, 35], we investigated whether loss of CBAP affects TSC2 protein docking on and off the lysosomal surface in response to insulin stimulation. Through an immunostaining approach, we found that co-localization of endogenous TSC2 and LAMP2 (a well-characterized lysosomal marker) was obvious upon serum starvation and that levels of co-localization were reduced upon re-stimulation with insulin (1 μM, 15 min) in Hela (Fig. 6b, upper panel) and CBAP-KO Hela cells (Fig. 6b, lower panel). However, insulin treatment stimulated less lysosomal dissociation of TSC2 in CBAP-KO cells (Fig. 6e, left panel). Similar insulin-stimulated dissociation of TSC2 from lysosomal compartments, stained with LysoView, was also detected in CBAP-KO cells (Fig. 6c). Notably, TSC2 cycling off lysosomal compartments was profoundly restored in HA-CBAP-expressing cells in response to insulin signal (Fig. 6d, Fig. 6e, right panel). These findings show that CBAP is an integral part of the mechanism by which Akt regulates TSC2 function and localization upon growth factor stimulation.
This study highlights the critical role of CBAP in regulating the proliferation of T-ALL, and proposes a CBAP-dependent mode of action for Akt-mediated TSC inactivation. Our model proposes direct involvement of CBAP in Akt-dependent TSC2 phosphorylation, which facilitates dissociation of TSC2 from lysosomal surfaces, thereby relieving the Rheb-mTORC1 signaling axis from suppression by the TSC. Furthermore, loss of CBAP impairs both Rheb-mTORC1 and Raf–MEK–ERK signaling activities, resulting in reductions of leukemia cell migration and growth. Consistently, CBAP-KO T-ALL cells exhibited reduced leukemogenicity and spleen invasiveness when transplanted into immunocompromised mice. Although we cannot completely exclude the possibility of a common mechanism involving CBAP acting upstream of both the Raf-MEK-ERK and Akt-mTORC1 signaling pathways (Fig. 4g), in this study we have nevertheless clearly demonstrated that CBAP has a direct role in promoting Akt-dependent TSC2 phosphorylation, driving Rheb-mTORC1 signaling and leukemic cell growth.
Our previous studies have reported the pro-apoptotic functions of CBAP in cytokine-dependent cell lines  or in primary hematopoietic cells [24, 25]. However, in the current study, we have discovered an important oncogenic and pro-proliferative role of CBAP in malignant hematological cells, such as T-ALL cells. That two seemingly opposing roles for one protein occur in different cellular microenvironments is not unprecedented. The oncogene c-Myc is a well-known oncoprotein, being overexpressed in B-cell leukemia and other human cancers. However, until very recently, its apparently intrinsic apoptotic properties were not fully appreciated (Prendergast, 1999). The myeloid ecotropic viral integration site 1 (Meis1) protein coordinates with HoxA9 in vivo to drive murine myeloid leukemogenesis. However, Meis1 has an obviously pro-apoptotic function in hematopoietic cell cultures when it is expressed alone, whereas co-expression of Meis1 with HoxA9 completely suppresses cell death . Similarly, Tribbles homolog 2 functions as an oncogene in inducing murine acute myelogenous leukemia (AML) and cooperates with HoxA9 to accelerate the onset of AML in vivo, which is consistent with the fact that Trib2 is highly expressed in a particular subset of human AML patients . However, ectopic expression of Trib2 alone in 32D cells (an IL-3-dependent myeloid leukemia cell line) , or in TF-1 cells , induces a strong apoptotic response. Therefore, the two seemingly opposing roles of CBAP may be influenced by a “missing factor” that cooperates with CBAP to control the cellular microenvironment of host cells and determines the biological function of CBAP. This possibility warrants further investigation.
The exact mechanism of CBAP-mediated TSC2 phosphorylation remains undetermined. Previous studies have shown that CBAP is involved in ZAP70-dependent Vav1 phosphorylation and β1 integrin signalosome activation in chemokine-induced inside-out signaling . It is also involved in LAT-PLCγ2-ZAP70 signalosome formation during TCR engagement . We have previously mapped two discrete binding sites for Vav1 and Zap70 in the N-terminus of CBAP, as well as a β1 integrin binding site in the C-terminal half of the CBAP protein , but their functions remain unknown. Here we have uncovered a similar role for CBAP in facilitating TSC2 phosphorylation by Akt. Since CBAP deficiency results in a reduction of the GTP loading of multiple small G proteins such as Rac1 , cdc42 , Ras and Rheb (this report), we suspect that multiple guanine nucleotide exchange factors (GEFs) and GTPase-activating proteins (GAPs) may be regulated by CBAP. It has been reported that CBAP is a member of the Mab21 subfamily in the nucleotidyl-transferase (NTase) fold protein superfamily . Proteins of this subfamily are characterized by sharing a common Mab21 core structure composed of an N-terminal NTase domain followed by a C-terminal polyA polymerase/2′−5′-oligoadenylate synthase1 (PAP/OAS1) substrate binding domain . A crystallographic study of CBAP protein structure would greatly enhance our understanding of how CBAP is involved in the activation of multiple small G proteins, as well as how its structure and function diverge from those of other NTase fold protein superfamily members [23, 40].
As a therapeutic strategy targeting the mTORC1 pathway, several studies have developed single or dual inhibitors targeting components of the PI3K-Akt-mTORC1 signaling cascade and have showed profound anti-leukemic effects on T-ALL cell lines or in vivo T-ALL models, suggesting the presence of a dominant oncogenic driver in this pathway [41, 42]. The advantage of targeting CBAP as a therapeutic intervention in the PI3K-Akt-mTORC1 axis is that knockout of the CBAP gene in mice resulted in almost no significant acute phenotype and CBAP plays no essential role in cell metabolism or proliferation in primary cells. However, the high metabolic demands of cancer cells apparently require more efficient enzymatic complexes, which may be facilitated by overexpression of CBAP protein. Consequently, a CBAP blocker should effectively suppress cancer cell growth that is dependent on the PI3K-Akt-mTORC1 signaling axis, while leaving other primary normal cells unaffected by systemic therapy.
Materials and methods
Patient samples and primary cells
Human samples used in this study were approved by the Institutional Review Board (IRB; AS-IRB01-11153 and AS-IRB01-16055) of Academia Sinica (AS). Paraffin-embedded specimens of patient bone marrow were provided by Tri-Service General Hospital (Taipei, Taiwan). Informed consent has been obtained from all subjects. All cases of T-ALL and anemia non-tumor specimens were diagnosed clinically and pathologically and are detailed in Table 1. Human blood cells were separated using a Ficoll gradient and CD3+ T cells were sorted using a FACSAria flow cytometer (Becton Dickinson, Franklin Lakes, NJ).
Plasmids expressing Flag-tagged TSC2 (#14129) and Myc-tagged TSC1 (#12133) were obtained from Addgene (Cambridge, MA). The mammalian Myc-tagged Akt1 expressing vector was generated from the pcDNA3-Akt1 plasmid by standard PCR-assisted cloning. The full-length Rheb gene was cloned from the cDNA of Jurkat cells and was subclonned to generate Flag-tagged Rheb plasmid.
Human cell lines and transplantation of NSG mice
Jurkat, MOLT-4, CCRF-CEM, HSB-2 and HL-60 cell lines were purchased from the American Type Culture Collection (ATCC, Manassas, VA). Kasumi-1 cell line was a gift from Dr. LT Hsiao obtaining from Bioresource Collection and Research Center, Taiwan. KG-1 cell line was obtained from Dr. PM Chen’s collection. For insulin stimulation, Hela cells were treated as described previously [20, 35]. NOD-scid-IL2RγKO (NSG) mice  were purchased from Jackson Laboratory (Bar Harbor, ME) and maintained in the specific pathogen-free animal facility of the Institute of Biomedical Sciences, AS. Animal experiments were approved by the Institutional Animal Care and Utilization Committee (IACUC) of AS (protocol number: 12-12-443). For tumor transplantation, five millions cells were transplanted by tail vein injection into 6–8-week-old male NSG recipients to generate cohorts of T-ALL leukemic mice for analyses.
Immunohistochemistry (IHC) of patient bone marrow sections
IHC of paraffin-embedded bone marrow biopsy specimens was performed with the Cell and Tissue Staining Kit HRP-DAB System (#CTS002, CTS005, Abingdon, UK) and SignalStain Antibody Diluent (8112, Cell signaling, Danvers, MA) following the vender’s instructions.
CRISPR/Cas9-mediated knockout and shRNA knockdown of CBAP
A CRISPR/Cas9 target site for CBAP co-expression with GFP was designed by Zgenebio Biotech Inc. (Taipei, Taiwan) (http://crispr.mit.edu). The target sequence used for CBAP was 5ʹ-GGCCCCAGCTCGGCCGCTCA-3ʹ. GFP+-sorted single cells were cultured to establish single-cell clones. Knockout and control (cr-Ctrl) clones were identified by immunoblot.
For shRNA-mediated knockdown of CBAP, lentiviral particles bearing specific shRNAs were provided by the National RNAi Core Facility of AS. Two different CBAP shRNAs were used: one targeting the 5′-ACCGAACGGAGAGCGAAGAAA-3′ sequence to produce the sh-CBAP (no. 1) clone, and another targeting 5′-CTGGACCTGGAATCCTGTTAC-3′ to produce the sh-CBAP (no. 2) clone. One non-targeted control shRNA (pLKO TRC025) was used to generate sh-Ctrl. Puromycin was used for selection of stable clones.
Leukemia xenograft bioluminescent imaging
Bioluminescent imaging was performed for all animals in the cohort by intraperitoneal injection of D-Luciferin potassium salt (BioVision, Milpitas, CA) at 150 mg/kg in conscious mice. After 7 min, mice were anesthetized (1% isofluorane) for image acquisition (IVIS 200, Caliper Life Sciences, Hopkinton, MA) with a 15 s exposure. The total photon flux−1 for bioluminescent imaging was determined using Living Image 4.5 software (Caliper Life Sciences, Hopkinton, MA).
Proliferation and cell-cycle analysis
Cell proliferation was evaluated using an automated cell counter (Countess, Invitrogen, Grand Island, NY) and the trypan blue exclusion method. For cell-cycle profile analysis, a BrdU/7-ADD staining kit (552598; BD Pharmingen, San Jose, CA) was used.
Cell immuno-fluorescence, confocal microscopy and quantification of co-localization
The immuno-fluorescence experiments and calculation of Manders’ co-localization coefficient (MCC) were performed according to a previous report  using a Zeiss LSM 700 confocal microscope (Oberkochen, Germany). For each condition, 3–6 representative confocal images from three independent experiments were used. For calculation of Manders’ co-localization coefficient (MCC), automatic Costes thresholding was applied to analyze a total of 45–95 individual cells per condition. Statistical significance was calculated using unpaired Student’s t test.
Measurement of cellular Rheb-GTP levels
To measure Rheb-GTP levels, we used a Rheb activation assay kit (81201; New East Biosciences, Malvern, PA) according to the manufacturer’s instructions.
In vitro akt kinase assay
Akt kinase assays were carried out using a non-radioactive Akt kinase assay kit (9840; Cell Signaling Technology, Danvers, MA) according to the manufacturer’s instructions. In vitro transcription/translation (IVT; L5010, Madison, WI) Flag-TSC2 protein was synthesized and used as the substrate.
Animal survival was assessed with Kaplan–Meier plots. The equality of the Kaplan–Meier survival distributions was assessed using the Mantel–Cox log-rank test for statistical significance. For other statistical analyses, P values were calculated with a two-tailed Student’s t test for two-group comparisons using Prism (GraphPad, La Jolla, CA). Differences were considered significant if the P value was < 0.05. *P < 0.05; **P < 0.01; ***P < 0.001; ****P < 0.0005.
Cell lysis, immunoprecipitation and immunoblots
All methods for total cell lysis, immunoprecipitation, and Western blotting were described previously . All antibodies used for this purpose are detailed in supplementary Table 3. The ImageJ software (Wayne Rasband, NIH) was used to quantify band intensities on the blots.
Quantitative reverse transcription PCR
Quantitative reverse transcription PCR and cDNA synthesis were performed as described . The primer sequences used for quantitative reverse transcription PCR of human CBAP were 5′-TGGCAAAGCTCTGTAGACCA-3′ (forward) and 5′-CTGGGCGGAACATAATGTGG-3′ (reverse). Relative fold expression was calculated by the 2−ΔΔCT method .
Roti G, Stegmaier K. New approaches to target T-ALL. Front Oncol. 2014;4:170.
Silverman LB, Gelber RD, Young ML, Dalton VK, Barr RD, Sallan SE. Induction failure in acute lymphoblastic leukemia of childhood. Cancer. 1999;85:1395–404.
Gokbuget N, Stanze D, Beck J, Diedrich H, Horst HA, Huttmann A, et al. Outcome of relapsed adult lymphoblastic leukemia depends on response to salvage chemotherapy, prognostic factors, and performance of stem cell transplantation. Blood. 2012;120:2032–41.
You MJ, Medeiros LJ, Hsi ED. T-lymphoblastic leukemia/lymphoma. Am J Clin Pathol. 2015;144:411–22.
Palomero T, Sulis ML, Cortina M, Real PJ, Barnes K, Ciofani M, et al. Mutational loss of PTEN induces resistance to NOTCH1 inhibition in T-cell leukemia. Nat Med. 2007;13:1203–10.
Blackburn JS, Liu S, Wilder JL, Dobrinski KP, Lobbardi R, Moore FE, et al. Clonal evolution enhances leukemia-propagating cell frequency in T cell acute lymphoblastic leukemia through Akt/mTORC1 pathway activation. Cancer Cell. 2014;25:366–78.
Jotta PY, Ganazza MA, Silva A, Viana MB, da Silva MJ, Zambaldi LJ, et al. Negative prognostic impact of PTEN mutation in pediatric T-cell acute lymphoblastic leukemia. Leukemia. 2010;24:239–42.
Silva A, Yunes JA, Cardoso BA, Martins LR, Jotta PY, Abecasis M, et al. PTEN posttranslational inactivation and hyperactivation of the PI3K/Akt pathway sustain primary T cell leukemia viability. J Clin Invest. 2008;118:3762–74.
Gutierrez A, Sanda T, Grebliunaite R, Carracedo A, Salmena L, Ahn Y, et al. High frequency of PTEN, PI3K, and AKT abnormalities in T-cell acute lymphoblastic leukemia. Blood. 2009;114:647–50.
Hoshii T, Matsuda S, Hirao A. Pleiotropic roles of mTOR complexes in haemato-lymphopoiesis and leukemogenesis. J Biochem. 2014;156:73–83.
Laplante M, Sabatini DM. mTOR signaling in growth control and disease. Cell. 2012;149:274–93.
Mendoza MC, Er EE, Blenis J. The Ras-ERK and PI3K-mTOR pathways: cross-talk and compensation. Trends Biochem Sci. 2011;36:320–8.
Crino PB, Nathanson KL, Henske EP. The tuberous sclerosis complex. N Engl J Med. 2006;355:1345–56.
Dibble CC, Manning BD. Signal integration by mTORC1 coordinates nutrient input with biosynthetic output. Nat Cell Biol. 2013;15:555–64.
Zoncu R, Efeyan A, Sabatini DM. mTOR: from growth signal integration to cancer, diabetes and ageing. Nat Rev Mol Cell Biol. 2011;12:21–35.
Tee AR, Fingar DC, Manning BD, Kwiatkowski DJ, Cantley LC, Blenis J. Tuberous sclerosis complex-1 and -2 gene products function together to inhibit mammalian target of rapamycin (mTOR)-mediated downstream signaling. Proc Natl Acad Sci USA. 2002;99:13571–6.
Dibble CC, Elis W, Menon S, Qin W, Klekota J, Asara JM, et al. TBC1D7 is a third subunit of the TSC1-TSC2 complex upstream of mTORC1. Mol Cell. 2012;47:535–46.
Huang J, Manning BD. The TSC1-TSC2 complex: a molecular switchboard controlling cell growth. Biochem J. 2008;412:179–90.
Inoki K, Li Y, Xu T, Guan KL. Rheb GTPase is a direct target of TSC2 GAP activity and regulates mTOR signaling. Genes Dev. 2003;17:1829–34.
Menon S, Dibble CC, Talbott G, Hoxhaj G, Valvezan AJ, Takahashi H, et al. Spatial control of the TSC complex integrates insulin and nutrient regulation of mTORC1 at the lysosome. Cell. 2014;156:771–85.
Demetriades C, Doumpas N, Teleman AA. Regulation of TORC1 in response to amino acid starvation via lysosomal recruitment of TSC2. Cell. 2014;156:786–99.
Kao CJ, Chiang YJ, Chen PH, Lin KR, Hwang PI, Yang-Yen HF, et al. CBAP interacts with the un-liganded common beta-subunit of the GM-CSF/IL-3/IL-5 receptor and induces apoptosis via mitochondrial dysfunction. Oncogene. 2008;27:1397–403.
Kuchta K, Knizewski L, Wyrwicz LS, Rychlewski L, Ginalski K. Comprehensive classification of nucleotidyltransferase fold proteins: identification of novel families and their representatives in human. Nucleic Acids Res. 2009;37:7701–14.
Chiang YJ, Ho KC, Sun CT, Chiu JJ, Lee FJ, Liao F, et al. CBAP functions as a novel component in chemokine-induced ZAP70-mediated T-cell adhesion and migration. PLoS ONE. 2013;8:e61761.
Ho KC, Chiang YJ, Lai AC, Liao NS, Chang YJ, Yang-Yen HF, et al. CBAP promotes thymocyte negative selection by facilitating T-cell receptor proximal signaling. Cell Death Dis. 2014;5:e1518.
Bilanges B, Argonza-Barrett R, Kolesnichenko M, Skinner C, Nair M, Chen M, et al. Tuberous sclerosis complex proteins 1 and 2 control serum-dependent translation in a TOP-dependent and -independent manner. Mol Cell Biol. 2007;27:5746–64.
Duvel K, Yecies JL, Menon S, Raman P, Lipovsky AI, Souza AL, et al. Activation of a metabolic gene regulatory network downstream of mTOR complex 1. Mol Cell. 2010;39:171–83.
Guertin DA, Sabatini DM. Defining the role of mTOR in cancer. Cancer Cell. 2007;12:9–22.
Huang J, Dibble CC, Matsuzaki M, Manning BD. The TSC1-TSC2 complex is required for proper activation of mTOR complex 2. Mol Cell Biol. 2008;28:4104–15.
Stofega M, DerMardirossian C, Bokoch GM. Affinity-based assay of Rho guanosine triphosphatase activation. Methods Mol Biol. 2006;332:269–79.
Ma L, Chen Z, Erdjument-Bromage H, Tempst P, Pandolfi PP. Phosphorylation and functional inactivation of TSC2 by Erk implications for tuberous sclerosis and cancer pathogenesis. Cell. 2005;121:179–93.
Roux PP, Ballif BA, Anjum R, Gygi SP, Blenis J. Tumor-promoting phorbol esters and activated Ras inactivate the tuberous sclerosis tumor suppressor complex via p90 ribosomal S6 kinase. Proc Natl Acad Sci USA. 2004;101:13489–94.
Dennis MD, Coleman CS, Berg A, Jefferson LS, Kimball SR. REDD1 enhances protein phosphatase 2A-mediated dephosphorylation of Akt to repress mTORC1 signaling. Sci Signal. 2014;7:ra68.
Cai SL, Tee AR, Short JD, Bergeron JM, Kim J, Shen J, et al. Activity of TSC2 is inhibited by AKT-mediated phosphorylation and membrane partitioning. J Cell Biol. 2006;173:279–89.
Demetriades C, Plescher M, Teleman AA. Lysosomal recruitment of TSC2 is a universal response to cellular stress. Nat Commun. 2016;7:10662.
Wermuth PJ, Buchberg AM. Meis1-mediated apoptosis is caspase dependent and can be suppressed by coexpression of HoxA9 in murine and human cell lines. Blood. 2005;105:1222–30.
Keeshan K, He Y, Wouters BJ, Shestova O, Xu L, Sai H, et al. Tribbles homolog 2 inactivates C/EBPalpha and causes acute myelogenous leukemia. Cancer Cell. 2006;10:401–11.
Keeshan K, Bailis W, Dedhia PH, Vega ME, Shestova O, Xu L, et al. Transformation by Tribbles homolog 2 (Trib2) requires both the Trib2 kinase domain and COP1 binding. Blood. 2010;116:4948–57.
Lin KR, Lee SF, Hung CM, Li CL, Yang-Yen HF, Yen JJ. Survival factor withdrawal-induced apoptosis of TF-1 cells involves a TRB2-Mcl-1 axis-dependent pathway. J Biol Chem. 2007;282:21962–72.
Nikolaidis N, Chalkia D, Watkins DN, Barrow RK, Snyder SH, van Rossum DB, et al. Ancient origin of the new developmental superfamily DANGER. PLoS ONE. 2007;2:e204.
Lonetti A, Cappellini A, Sparta AM, Chiarini F, Buontempo F, Evangelisti C, et al. PI3K pan-inhibition impairs more efficiently proliferation and survival of T-cell acute lymphoblastic leukemia cell lines when compared to isoform-selective PI3K inhibitors. Oncotarget. 2015;6:10399–414.
Chiarini F, Grimaldi C, Ricci F, Tazzari PL, Evangelisti C, Ognibene A, et al. Activity of the novel dual phosphatidylinositol 3-kinase/mammalian target of rapamycin inhibitor NVP-BEZ235 against T-cell acute lymphoblastic leukemia. Cancer Res. 2010;70:8097–107.
Ito M, Hiramatsu H, Kobayashi K, Suzue K, Kawahata M, Hioki K, et al. NOD/SCID/gamma(c)(null) mouse: an excellent recipient mouse model for engraftment of human cells. Blood. 2002;100:3175–82.
Livak KJ, Schmittgen TD. Analysis of relative gene expression data using real-time quantitative PCR and the 2(-Delta Delta C(T)) Method. Methods. 2001;25:402–8.
We thank Dr. Richard Lin at Stony Brook University Medical Center for his careful reading of the manuscript and his suggestions. We thank the National Center for Genome Medicine, National RNAi Core Facility, and the Molecular and Genetic Imaging Core of the Taiwan Mouse Clinic for their technical support. This work was supported by grants from the Ministry of Science and Technology, Taiwan to JJYY (NSC102-2320-B001-007-MY3 and MOST105-2320-B-001-012-MY3), and was partly supported by Tri-Service General Hospital (TSGH-106-01-34). YJC is supported by postdoctoral fellowships MOST103-2811-B-001-090 and MOST105-2811-B-001-044.
Conflict of interest
The authors declare that they have no conflict of interest.
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Chiang, YJ., Liao, WT., Ho, KC. et al. CBAP modulates Akt-dependent TSC2 phosphorylation to promote Rheb-mTORC1 signaling and growth of T-cell acute lymphoblastic leukemia. Oncogene 38, 1432–1447 (2019). https://doi.org/10.1038/s41388-018-0507-6
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