International Journal of Cell Biology

International Journal of Cell Biology / 2013 / Article
Special Issue

Alternative Splicing: Role in Cancer Development and Progression

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Review Article | Open Access

Volume 2013 |Article ID 962038 | 17 pages |

Oncogenic Alternative Splicing Switches: Role in Cancer Progression and Prospects for Therapy

Academic Editor: Claudio Sette
Received30 May 2013
Accepted12 Aug 2013
Published27 Oct 2013


Alterations in the abundance or activities of alternative splicing regulators generate alternatively spliced variants that contribute to multiple aspects of tumor establishment, progression and resistance to therapeutic treatments. Notably, many cancer-associated genes are regulated through alternative splicing suggesting a significant role of this post-transcriptional regulatory mechanism in the production of oncogenes and tumor suppressors. Thus, the study of alternative splicing in cancer might provide a better understanding of the malignant transformation and identify novel pathways that are uniquely relevant to tumorigenesis. Understanding the molecular underpinnings of cancer-associated alternative splicing isoforms will not only help to explain many fundamental hallmarks of cancer, but will also offer unprecedented opportunities to improve the efficacy of anti-cancer treatments.

1. Introduction

Alternative splicing is the process by which splice sites in precursor messenger RNAs (pre-mRNAs) are differentially selected and paired to produce multiple mature mRNAs and protein isoforms with distinct structural and functional properties. The first example of alternative splicing was discovered almost 30 years ago, when membrane-bound and secreted antibodies were demonstrated to be encoded by the same gene [1, 2]. Now, we know that alternative splicing is a very accurate, efficient, and extraordinarily flexible process that regulates all major aspects of eukaryotic cell biology. Affecting approximately 94% of human genes [3, 4], it represents the major source of the human proteomic diversity.

Regulation of alternative splicing decisions involves the recognition of target sequences in the pre-mRNA by a number of splicing regulatory factors with antagonistic functions such as SR (serine-arginine-rich) and hnRNP (heterogeneous nuclear ribonucleoprotein) protein families [5]. Generally, SR proteins promote exon recognition by binding to exonic or intronic splicing enhancer sequences (ESEs and ISEs, resp.), while hnRNP factors typically interact with exonic or intronic splicing silencers (ESSs and ISEs) inhibiting splice sites recognition. The regulation of alternative splicing has been discussed in several excellent reviews [68].

Changes in alternative splicing patterns have an essential role in normal development, differentiation, and in response to physiological stimuli, but aberrant splicing generates variants that contribute to multiple aspects of tumor establishment and progression and in the resistance to therapeutic treatments [5, 9, 10]. Many cancer-associated splicing isoforms are expressed during embryonic development, but not in normal adult tissues, whereas others are entirely novel transcripts [11]. Central to the splicing oncogenic switch are changes in the expression, activity, or post-translational modification of splicing regulatory factors, such as SR and hnRNP proteins [5, 9]. Thus, modification of alternative splicing profiles contemporaneously affects multiple key aspects of cancer cell biology, including control of cell proliferation, cancer metabolism, angiogenesis, evasion from apoptosis, invasiveness, and metastasis [5, 9, 10].

Here, we discuss aberrant alternative splicing networks that contribute to the oncogenic phenotype and have a prominent role in important aspects of tumorigenesis process, including response to hypoxia and cancer cell invasion and metastasis. In addition, we also discuss important questions connected to the role of alternative splicing in cancer: what are the relevant splicing switches that are critical to malignant transformation? How the amounts/activity of the splicing regulatory factors modulate these splicing switches? What are the main functions of cancer-associated alternatively spliced variants? By illustrating specific examples, it will be clear how the production of cancer-related isoforms offers the potential to develop novel diagnostic, prognostic, and more specific anticancer therapies.

2. Alternative Splicing Changes of Cancer Cells in Response to Hypoxia

Through the activation of oncogenes and inactivation of tumor suppressor genes, cancer cells become able to proliferate, survive, and resist to apoptosis. Nevertheless, also microenvironmental signaling plays a crucial role in controlling cancer cell homeostasis, metabolism, growth, and differentiation [12]. The microenvironment in solid tumors is very distinct from that in normal tissues and the cross-talk between cancer and stromal cells contributes to the formation of a clinically relevant tumor and to response to antitumor therapy [13, 14]. Modifications of the microenvironment (most of these start early during tumor progression) result from metabolic alterations in cancer cells and from recruitment or activating of nontumoral cells, including blood and lymphatic endothelial cells, pericytes, carcinoma-associated fibroblasts, bone marrow-derived cells, and immune and inflammatory cells [15, 16]. In this altered microenvironment cancer cells are exposed to pro-proliferative growth factors. In addition, transformed cells often hijack the signaling circuits acting on normal cells in order to become independent from external stimulation to grow and proliferate [12, 13]. Due to deregulated cancer cell metabolism (the consequence of uncontrolled and rapid proliferation) and to an altered structure and functionality of tumor blood vessels, the tumor microenvironment is characterized by hypoxia and acidosis [15, 17, 18]. Hypoxic tumor microenvironments are now recognized as a selective pressures that promote tumor aggressiveness, inducing cancer cells to metastasize and making them refractory to radiotherapy and chemotherapy. Cells cope with hypoxia by activating transcription factor HIF-1 (hypoxia-inducible factor-1), a heterodimer formed by the constitutively expressed β subunit (HIF-1β) and the inducible α subunit (HIF-1α) [19]. The regulation of HIF-1 activity is mainly at the protein level [19]. Under non-hypoxic conditions, the HIF-1α subunit is rapidly ubiquitinylated and degraded by the pVHL (von Hippel-Lindau tumor suppressor protein) and the proteasome, thus preventing the dimerization with HIF-1β [19]. Under hypoxia, HIF-1α degradation is suppressed and its level increases rapidly. The HIF-1α/HIF-1β heterodimer translocates to the nucleus where it binds to hypoxia response elements (HRE) in the promoters of target genes. Through the activation of more than 150 genes, HIF-1 affects important biological processes such as angiogenesis, glucose metabolism, cell proliferation, survival, apoptosis, and invasion/metastasis [19]. Target genes include several enzymes involved in glycolysis (Glut-1 and PDK-1), angiogenesis, iron metabolism (transferrin), cell adhesion molecules (MIC2), fibronectin and matrix metalloproteinase (MMP-2), extracellular matrix (ECM) modifying enzymes such as lysyl oxidase, and pluripotency factors including OCT4, NANOG, and SOX2 [1921].

One of the primary targets of HIF-1 is VEGFA (Vascular Endothelial Growth Factor A), a cytokine that promotes blood vessel growth and stimulates angiogenesis [22]. VEGF, secreted by hypoxic cancer cells, diffuses through the tumor mass to neighbouring host normal vessels, where, upon binding to its receptor VEGFR2, it stimulates endothelial cells to proliferate, migrate toward the tumor, and form new capillaries [23]. Even though the angiogenesis process does not initiate malignancy, it promotes tumor growth by allowing oxygen and nutrients to reach proliferating cancer cells [23]. Alternative splicing occurs extensively within VEGF pre-mRNA, generating various isoforms with different C-terminal domains and distinct affinity for its receptors and with a non-redundant role in angiogenesis [24, 25]. VEGF isoforms are classified in two families, called VEGFxxx (pro-angiogenic) and VEGFxxxb (anti-angiogenic), where xxx denotes the position of the amino acid residue in the mature protein. Pro- or anti-angiogenic isoforms are generated through alternative splicing of the mutually exclusive terminal exons 8a and 8b. Selection of the proximal 5′ splice site (PSS) in exon 8a generates VEGFxxx whereas the distal 5′ splice site (DSS) in exon 8b results in VEGFxxxb isoforms. The two types of isoforms bind VEGFR2 (Vascular Endothelial Growth Factor Receptor 2) with equal affinity. However, VEGFxxx activates the downstream signaling pathways and induces angiogenesis, while VEGFxxxb blocks this process [26]. Given these characteristics, it is not surprising that VEGFxxxb is preferentially expressed in normal tissues and it is downregulated in cancer [25]. The choice between PSS or DSS depends upon the activity of the splicing factors of the SR family SRSF1 and SRSF6: SRSF6 preferentially selects the DSS and promotes the production of anti-angiogenic VEGF isoforms, whereas SRSF1 mainly activates the proximal PSS [27]. Thus, the altered expression of SRSF1 and SRSF6 in many types of tumors could impact malignant transformation by ensuring the proper balance of pro- and anti-angiogenic isoforms in cancer cells [28, 29]. Importantly, microenviromental factors can influence alternative splicing of VEGF. For example, treatment with TGF-β1 increases the anti-angiogenic VEGFxxxb isoforms via p38 MAPK signaling [27]. Conversely, Insulin-like Growth Factor 1 (IGF-1) decreases the expression of VEGFxxxb isoforms in retinal pigmented epithelial cells through PKC and SRPK1 [30]. SRPK1 is a protein kinase that specifically phosphorylates proteins containing SR domains and is upregulated in various types of cancer, like pancreatic, breast, and colon carcinoma [31].

Recently, a genome-wide analysis of hypoxia-induced alternative splicing changes in endothelial cells has identified target genes implicated in angiogenesis-mediated cytoskeleton remodeling (cask, itsn1, larp6, sptan1, tpm1, and robo1), in the synthesis of membrane anchors (pign) and in the regulation of gene expression (cugbp1 and max) [32]. These changes are likely part of the adaptation of endothelial cells to stressing conditions. The impact of hypoxia on post-transcriptional events is proven also by LAMA3-A (Laminin alpha 3), a splicing variant of the LAMA3 gene induced by reduction of oxygen supply which promotes cell invasion and is associated with a poor prognosis in head and neck cancer [33, 34].

As mentioned before, HIF is a heterodimer that acts as a dominant regulator of adaptive cellular responses to hypoxia. There are three principal isoforms of the HIF-α subunit encoded by distinct genes: HIF-1α, HIF-2α (EPAS1), and HIF-3α. HIF-3α gene consists of 19 exons and it is subjected to extensive alternative splicing leading to the production of at least six isoforms [35]. HIF-3α4 is one of the HIF-3α splicing variants whose functions have recently been linked the development of hypervascular malignant meningiomas [36]. Indeed, HIF-3α4 directly binds to HIF-1α and suppresses HRE dependent transcription of VEGF. Importantly, HIF-3α4 is able to inhibit proliferation and invasion, to reduce neovascularization and glucose metabolism in hypervascular meningiomas [36].

Another gene induced by hypoxia is Cyr61 (cysteine rich 61) encoding for a secrete protein that functions as a proangiogenic factor promoting adhesion, migration, and survival of vascular endothelial cells [37]. Cyr61 is supposed to be a promoter of tumor progression since its high expression levels were detected in various cancer types [38, 39]. Notably, in addition to transcriptional level, the expression of Cyr61 can be also regulated through an alternative splicing event that stimulates the retention of intron 3 in Cyr61 mRNA leading to the production of a nonsense-mediated decay (NMD) sensible transcript [40]. Importantly, this alternative splicing event coupled with NMD pathway (called AS-NMD) was reported to be altered in breast cancer and associated with a shift from an intron 3 retained transcript (IR) toward an intron 3 spliced mRNA (IS) encoding for the biological active Cyr61 protein. Moreover, in several breast cancer cell lines under hypoxic conditions AS-NMD of Cyr61 was reported to enhance the expression of the IS transcript, suggesting that hypoxia-mediated alternative splicing changes could be a central mechanism regulating the Cyr61 expression and its tumor-promoting activity [40].

The CD44 glycoprotein provides another attractive example of hypoxia-induced alternative splicing changes. CD44 is a transmembrane molecule able to bind several ligands, including important components of ECM, such as hyaluronic acid, collagen, fibronectin, laminin, and matrix metalloproteinases (MMPs), and involved in cell-cell and cell-matrix interactions, migration, and invasion [41]. CD44 pre-mRNA consists of 20 exons, 10 of which (v1–v10) undergo alternative splicing events, thus generating multiple CD44 isoforms with different molecular sizes and with diverse extracellular domains [41, 42]. The predominant CD44 isoform, the low-molecular-weight CD44s (90 kDa standard form), is expressed by several tissues, including hematopoietic, fibroblast, and glial cells, whereas high-molecular-weight CD44v variants (140–230 kDa) are restricted to epithelial cells and abundant in epithelial-type carcinomas [41, 42]. The physiological/pathological functions of most CD44v variants remain still poorly understood. However, it has been observed that some variants are over-expressed in various tumors and implicated in cancer cell invasion and metastasis [41, 43, 44]. In particular, CD44v6 and CD44v8 variants are associated with tumor progression and poor diagnosis in several types of carcinoma including breast and colorectal cancers [4547]. Interestingly, HIF-1α is able to increase the expression of the CD44 mRNA and to upregulate CD44 variants containing exons v6 and v7/8 [48]. In line with this, Krishnamachary and collaborators have reported that hypoxic regions of breast cancer specimens contain cells with elevated expression of CD44 [48]. Additional studies are necessary to identify the molecular mechanisms and signaling pathways regulating CD44 alternative splicing in response to hypoxia.

Hypoxia-induced alternative splicing changes were also recently investigated in the study of Hirschfeld and colleagues [49]. The YT521 (YTH domain containing 1) is a ubiquitously expressed nuclear splicing factor containing a novel RNA-binding domain (YTH domain) necessary for YT521 to directly influence splice site selection. Importantly, low YT521 expression was associated with clinical outcome in patients with type I endometrial cancer, suggesting its potential role as a tumor suppressor [50]. Furthermore, YT521 alternative splicing targets are well-known cancer-associated genes such as BRCA2, ESR1, MDM2, VEGF, and CD44 [49, 5155]. Similar to other proteins involved in mRNA processing, the expression of YT521 is regulated by alternative splicing. Interestingly, it was reported that under hypoxic conditions the alternative splicing of YT521 pre-mRNA containing exons 8 and 9 generates two transcripts that are subjected to degradation through NMD, suggesting that these AS-NMD events of YT521 could simultaneously affect the processing of several cancer-associated genes.

Further functional investigations on hypoxia and its impact in regard to alternative splicing of target genes may contribute to better understanding of a key regulatory epiphenomenon in tumor growth involved in the development of an aggressive cancer phenotype.

3. Invasion and Metastases

The term metastasization is currently used to indicate the ability of tumor cells to invade adjacent tissues and disseminate toward distant organs [56]. This is a multistep process that involves (i) local invasion of tumor cells through the basement membrane and endothelial walls into the host stroma, (ii) intravasation within the blood and the lymphatic circulatory systems; (iii) extravasation into distant tissues, and (iv) proliferation of tumor cells allowing growth and efficient metastatic colonization [56].

As observed for other hallmarks of cancer, gene expression programs implicated in the metastatic process are the same that participate in embryonic development, morphogenesis, and wound healing [57, 58]. One of these programs that physiologically pertain to embryogenesis is the epithelial-to-mesenchymal transition (EMT). The EMT process involves dedifferentiation steps in which cells lose their epithelial phenotype to acquire mesenchymal traits [58, 59]. The epithelial cell layer consists of polarized cells with cohesive cell-cell junctions. Through EMT cells undergo an extensive reorganization of the cytoskeletal architecture with the loss of intercellular junctions and cell polarity and the acquisition of an elongated, fibroblast-like shape. During tumor progression, EMT is one of the major routes through which cancer cells acquire invasive capabilities and spread throughout the body as single cells [58, 59]. Importantly, tumor EMT is a transient process that occurs in a subset of cells at the invasive front of the metastasizing primary carcinoma and is reversed at the final metastatic sites, where cells undergo the reverse process, namely, the mesenchymal-to-epithelial transition (MET) [58, 59]. This plasticity and the redifferentiation of metastatic cells to an epithelial identity help in organ colonization, ensuring metastasis formation. Moreover, it clearly indicates that EMT is not driven by stable genetic mutations but by activation of gene expression programs in response to external cues in the tumor microenvironment.

Several relevant players involved in EMT/MET cycles have been identified including transcription factors, growth factors, cytokines and chemokines, pro-angiogenic factors, cell adhesion molecules, modifiers of cytoskeletal organization, and extracellular matrix-remodeling enzymes [60]. The prevailing models propose that these regulators act largely at transcriptional level. Indeed, several pathways activate a network of transcription factors that promote the expression of mesenchymal markers, such as N-cadherin and vimentin, while inhibiting E-cadherin production, not only a key component of adherent junctions but also a tumor suppressor frequently repressed, mutated or degraded during tumor transformation [58, 59]. However, in the last few years, several studies have highlighted additional layers of EMT control, including epigenetic reprogramming, small noncoding RNAs, translational and post-translational regulations, and alternative splicing changes [10, 57, 61, 62]. In particular, an increasing body of evidence indicates that splicing regulation alone can drive critical aspects of EMT-associated phenotypic changes [10]. Below, we discuss some interesting examples of specific alternative splicing events that are implicated not just in the EMT/MET program but also in the different stages of the metastatic cascade.

3.1. Ron

Alternative splicing of the Ron proto-oncogene (also known as MST1R) has provided the first example of an alternative splicing variant linked to the activation of tumor EMT. Ron encodes for a tyrosine kinase receptor involved in control of cell dissociation, migration, and matrix invasion. The activity of the Ron receptor is regulated through alternative splicing. In particular, a constitutively active isoform (called ΔRon), which confers increased motility to expressing cells and accumulates during tumor progression of epithelial cancers [63, 64], is generated through skipping of exon 11. The oncoprotein SRSF1 deeply impacts cell physiology since its upregulation stimulates skipping of exon 11, thus promoting the production of ΔRon isoform that in turn triggers activation of the EMT program increasing the invasive properties of the cells [64]. Interestingly, SRSF1 expression levels are dynamically controlled in epithelial and mesenchymal cells through an AS-NMD event [65]. AS-NMD of SRSF1, which involves an intron in the 3′UTR region of the gene, decreases mRNA stability and SRSF1 protein levels and, notably, it is altered in colon cancer. This scenario is further complicated by the involvement of another splicing regulator, Sam68. Sam68, the 68 kD Src-associated protein in mitosis, is a member of the STAR (signal transduction and activation of RNA) family of RNA-binding proteins [66]. It contains a single KH-type RNA-binding domain and several protein-protein interaction motifs including potential binding sites for SH2, SH3, and WW domains, which are characteristic of signaling transducers [67]. Sam68 has been recognized as a substrate of several kinases, such as members of the Src family, ERK1/2 and BRK (Breast Tumor Kinase) [65, 6870]. As such, Sam68 is the first identified “hub factor” able to communicate extracellular stimuli to specific RNA splicing decisions. In particular, directed by ERK1/2 signaling, Sam68 controls AS-NMD of SRSF1 transcript, thus modulating its protein level. Notably, epithelial cell-derived soluble factors are able to inhibit ERK1/2 signaling thereby repressing Sam68 phosphorylation, which increases the production of the NMD-sensitive transcript of SRSF1.

3.2. Rac1

The matrix metalloproteinases (MMPs) are the most important family of proteinases of the tumor microenvironment that degrade structural components of the extracellular matrix (ECM), thus regulating proliferation, cell-cell adhesion, angiogenesis, invasion, and metastases [71]. In line with this, MMPs are upregulated in almost all types of human cancer and associated with poor survival [71]. Notably, over-expression of MMP-3 in mammary and lung epithelial cells triggers a cascade of events that determine activation of EMT process [72, 73]. Notably, these events, which induce tumorigenesis process in transgenic mice, are dependent on the expression of a constitutively active alternatively spliced isoform of the Rac1 gene, encoding for a small GTPase of the mammalian Rho family involved in actin cytoskeleton organization, cell growth, cell-cell adhesion, and migration [74]. This splice variant (known as Rac1b) is produced by inclusion of the exon 3b that contains the encoding region for a 19-amino acid domain involved in the interaction with regulator and effector molecules [75]. Since Rac1b shows increased expression during progression of several cancer types [72, 75, 76], it is tempting to speculate that the exon 3b (or the 19-amino acid insertion) could offer the opportunity for a selective targeting to develop anticancer therapies that block EMT-associated progression towards advanced tumor stages.

3.3. KLF6

The complexity of networks regulating the EMT program makes it very difficult to identify early inducers and a unifying molecular basis for this transition. Many transcription factors have been extensively studied for their involvement in activation of EMT. Among these are Slug (referred also to as SNAI2) and Twist, two repressors of E-cadherin promoter activity [57]. Recent studies have revealed important roles for specific alternatively spliced variants of upstream regulators of Slug and Twist activity. This is the case of oncogenic splice variant 1 of KLF6 (KLF6-SV1), a tumor suppressor gene belonging to the Krüppel-like family of transcription factors, able to act as functional driver of the entire metastatic cascade through Twist induction [77, 78]. Notably, KLF6-SV1 antagonizes the tumor suppressive activity of the full-length KLF6 protein and sustains tumor growth and dissemination in ovarian and prostate cancer models [7981]. Interestingly, increased expression of KLF6-SV1 occurs in many tumors and is associated with poor prognosis in prostate, lung, and ovarian cancers [82]. KLF6-SV1 has been recently shown to induce EMT and to drive aggressive multiorgan metastasis formation in both subcutaneous and orthotopic mouse models of breast cancer [78]. In this process, it acts through a Twist-dependent mechanism and Twist downregulation reverts the phenotype of KLF6-SV1 over-expressing cells, restoring the expression of epithelial markers [78]. Finally, high levels of KLF6-SV1 were found associated with increase in EMT markers in a large cohort of primary breast cancer patients [78].

3.4. FAM3B

FAM3B is a member of the novel FAM3 family of cytokine-like genes, predicted to produce at least 7 alternatively spliced isoforms [83, 84]. The most studied variant is the secreted form PANDER, so called for its robust expression and activity in the pancreatic cells [85, 86]. In addition, lower PANDER levels have been observed in human gastric cancers in respect to the corresponding normal tissues [87]. Recently, Li and colleagues have identified FAM3B-258, a 258-amino acids non-secretory protein, as a novel splicing variant of FAM3B up-regulated in colon adenocarcinoma cell lines as well as in human colorectal tumors [84]. FAM3B-258 is able to induce changes typical of an activated EMT program, stimulating cell migration and invasion in vitro and promoting metastases formation in nude mice. The oncogenic abilities of FAM3B-258 require a Slug-mediated transcriptional repression of E-cadherin and JAM (Junctional Adhesion Molecule). Knock-down of Slug in FAM3B-258 over-expressing cells restores higher levels of E-cadherin and JAM and prevents the FAM3B-258-dependent cell invasion [84]. Whether Slug is a direct target of FAM3B-258 or whether other signaling effectors are involved remains to be investigated.

3.5. Cortactin

To become migratory and invasive, cells must extend plasma membrane protrusions (such as lamellipodia and filopodia) forward and overcome the epithelial basement layer as a first barrier [56, 88]. The formation of invadopodia has been recently characterized as another important step of the EMT program [8991]. Invadopodia are enriched with a variety of proteins, including actin and actin regulatory proteins [92, 93]. The filamentous actin (F-actin) binding protein cortactin is one of the regulators of actin polymerization/branching involved in invadopodia assembly and maturation [92, 94]. Three splicing products of cortactin have been characterized until now [95]. Unlike the full-length protein (FL), the SV1 and SV2 variants lack, respectively, one and two of the six “cortactin repeats” that mediate the interaction with F-actin [95]. As a consequence of their reduced capabilities in F-acting binding and polymerization, over-expression of SV1- or SV2-cortactin shows reduced cell migration when compared with FL-cortactin over-expressing cells [95]. One of the factors that control alternative splicing of cortactin transcripts is SPF45 [96]. Initially characterized as a component of the spliceosome, SPF45 has been also implicated in the regulation of Fas and fibronectin alternative splicing [97, 98]. In their interesting article, Liu and coworkers have demonstrated that SPF45 mediates cell migration and invasion in ovarian cancer cells by promoting the formation of the FL-cortactin isoform. SPF45 activity appears to be controlled via phosphorylation by Clk1 (Cdc2-like kinase). Finally, SPF45 over-expression correlates also with increased cortactin phosphorylation by ERK, which enhances cortactin-mediated actin polymerization [96, 99].

3.6. MENA

As for invadopodia, filopodia nucleation and extension require actin cytoskeleton remodeling and involve several regulators of actin dynamics, such as the Ena/VASP protein family that in mammals includes three members: MENA (also called ENAH), VASP, and EVL [88]. Up-regulation of MENA has been detected in several human cancers, including breast cancer and melanoma and correlates with invasiveness of breast tumors [100, 101]. MENA pre-mRNA is alternatively spliced to generate different isoforms, expressed in a tissue-specific manner [102]. Importantly, the alternative splicing profile of MENA in invasive tumor cells is different from non-migratory resident cancer cells. Non-invasive tumor cells as well as poorly invasive breast cancer cells with epithelial morphology express MENA11a, the epithelial-associated variant generated from inclusion of exon 11a [102, 103]. This exon is inserted within the EVH2 domain, very close to the F-actin binding motif and the tetramerization site. This insertion has been predicted to affect the ability of MENA tetramers to interact with F-actin and thus to drive filopodia and lamellipodia maturation [103]. In agreement with this, the increment of MENA11a reduces both the number and the length of filopodia in a 3D culture assay [104]. On the contrary, invasive cancer cells lack MENA11a and express MENAINV, an isoform containing an additional exon, also referred to as exon +++ [103, 105]. The relative abundance of MENAINV and MENA11a seems to be important to regulate key stages of the metastatic cascade in breast cancer cells. Thus, high levels of MENAINV enhance coordinated motility, transendothelial migration, and intravasation of tumor cells, promoting spontaneous lung metastases in a murine model of breast cancer [105, 106]. In contrast, increased expression of MENA11a correlates with decreased invasion, intravasation, and dissemination of cancer cells [106]. Recently, Di Modugno and coworkers have identified another splice variant of human MENA lacking exon 6 and called hMENAΔv6 [104]. Contrary to MENA11a, hMENAΔv6 is expressed selectively in invasive cancer cells with mesenchymal phenotype and is able to enhance invasiveness of breast cancer cells but only in the absence of MENA11a [104]. This evidence suggests that MENA11a behaves as dominant anti-invasive player, making alternative splicing of this gene a potential target for anticancer therapies. Furthermore, MENA splicing occurs also in primary breast tumors and in particular MENA11a-negative tumors display lower level of E-cadherin when compared to MENA11a-positive samples [104], supporting the anti-migratory functions of this splicing isoform [104].

Splicing of MENA exon 11a is regulated by the expression levels of epithelial-specific alternative splicing factors ESRP1 and 2 (Epithelial Splicing Regulatory Proteins 1 and 2), two important regulators of the mesenchymal and epithelial splicing signatures [107]. In particular, ESRP proteins, by promoting inclusion of exon 11a and the production of MENA11a isoform, cause a drastic reorganization of actin cytoskeleton as well as cell morphology and a reduction of invasive properties [107]. In addition to MENA, ESRPs control the alternative splicing of several genes involved in different aspects of the metastatic cascade, such as cell-cell and cell-matrix adhesion, actin cytoskeleton organization, cell polarity, and migration [108, 109]. In line with this, modification of ESRPs expression levels results in alternative splicing changes of CD44 and p120-Catenin, a protein found at cell-cell junctions and also involved in signal transduction [108, 109].

3.7. L1CAM

The penetration of migrating cancer cells into tissue barriers, including the basement membrane, is supported by the proteolytic degradation of the extracellular matrix (ECM) through the activity of secreted enzymes, such as matrix metalloproteinases MMP-2 and MMP-9 [110]. The expression and activity of MMPs are regulated through several signals, mainly induced by growth factors and chemokines, as well as through integrin and extracellular matrix-mediated signals [110]. Recently, the alternative splicing of the cell adhesion molecule L1 (L1CAM) has been found to control the invasive capabilities of tumor cells by regulating MMP-2 and MMP-9 expression and activity [111]. More specifically, although initially the splicing variant considered as cancer-associated was SV-L1CAM (lacking of exons 2 and 27), only the full-length FL-L1CAM has been found up-regulated upon exposure of tumor cells to the pro-metastatic factors TGF-β and HGF. Importantly, the over-expression of FL-L1CAM but not of the SV isoform is able to induce metastasis formation in mice [111].

3.8. SVEP1

Invasion and colonization of a secondary organ by disseminating cancer cells are influenced by the microenvironment and the cross-talk between cancer populations and cells in the niche of the receiving tissue [56, 112]. The cell adhesion molecule SVEP1 has been recently involved in the interactive network that affects breast cancer cells homing to bone niches [113]. SVEP1 expression is stimulated by TNFα, a pro-inflammatory cytokine able to affect adhesion and migration, and to induce EMT [114, 115]. Recently, Glait-Santar and colleagues have investigated the alternative splicing of SVEP1 transcripts in a co-culture model of pre-osteoblastic MDA-15 and mammary adenocarcinoma DA3 cells, which mimic the molecular interactions in the bone niche after invasion of breast carcinoma cells [116]. Similar to what observed after TNFα treatment, several splicing isoforms of SVEP1, such as the full-length isoform a and isoform e, are up-regulated in both cell lines upon co-culture conditions. In parallel embryonic variants g and f are silenced in adenocarcinoma DA3 cells, whereas no effect is observed in pre-osteoblastoma cells [116]. The same authors also observed that the ratio between splicing isoforms of SVEP1 is perturbed after treatment with epigenetic drugs such as DNA demethylating or histone deacetylase inhibitors, supporting a link between the epigenetic organization and splicing of SVEP1 pre-mRNA. However, further studies are needed to establish the pathological role of the different SVEP1 isoforms in the metastatic process.

3.9. CD44

Several microenvironmental stressors, including nutrient deficiency, low pH, mediators of inflammatory responses, and reactive oxygen species (ROS), can affect successful colonization by disseminating cells at the final metastatic tissues [117]. Disseminating cancer cells can take advantage of antioxidant systems to counteract the exposure to oxidative stress. The synthesis of reduced glutathione (GSH), a reducing thiol peptide, protects cancer cells against ROS-mediated damage and confers resistance to anticancer therapies [118, 119]. A rate-limiting factor for GSH synthesis is the availability of cysteine and the cystine transporter system xc- (composed by two subunits, xCT and CD98hc) is essential in the GSH antioxidant mechanism [119, 120]. Recently, a link between the GSH-dependent evasion from oxidative stress and alternative splicing of CD44 has been identified [121, 122]. As mentioned before, CD44 has an important role in cell-cell and cell-matrix interactions, migration, and invasion [41]. Through alternative splicing, CD44 pre-mRNA generates multiple CD44 high-molecular-weight isoforms with different extracellular domains [41, 42]. Intriguingly, CD44v8-10 has been demonstrated to interact with the cystine transporter xCT, increasing the levels of GSH and, as a consequence, the ability of cancer cells to avoid ROS damage [122]. In line with this, CD44v-positive 4T1 mouse breast cancer cells display high levels of GSH and xCT and enhanced ROS defense compared to CD44v-negative 4T1 cells [123]. Thus, CD44v-positive 4T1 are able to establish lung metastatic lesions in mouse models with an incidence higher than CD44v-negative cells [123]. Interestingly, down-regulation of the splicing regulator ESRP1 in metastatic 4T1 cells shifts the splicing pattern toward the production of CD44s and results in suppression of lung metastasis [123]. On the contrary, forced expression of CD44v8-10 in ESRP1-depleted cells is sufficient to restore high content of GSH and lung colonization potential [123].

4. Diagnostic, Prognostic, and Anticancer Therapy Potentials of Alternative Splicing

Cancer chemotherapy relies on the expectation that anticancer drugs will preferentially kill rapidly dividing tumor cells, rather than normal cells. Unfortunately, most pharmacological approaches for the treatment of solid tumors suffer from poor selectivity, which limits the overall dose of drug that can be administered because of unacceptable toxicities to normal tissues.

As shown in previous sections, alternative splicing variants of many cancer-related genes can directly contribute to the oncogenic phenotype and to the acquisition of resistance to therapeutic treatments [5, 9, 10]. Alternative splicing isoforms selectively expressed by tumors and not by normal tissues may represent suitable targets for new therapeutical approaches [11]. In this section, we discuss some significant examples to illustrate how cancer-specific splicing events can be a powerful source of new diagnostic, prognostic, and therapeutic tools.

Several highly sensitive methods allowed the identification of cancer-specific splicing isoforms [124128]. For example, the splicing profile of ABCC1, Mdm2, and fibronectin transcripts has been used to distinguish normal ovary from epithelial ovarian cancer [127], whereas altered splicing of MED24, MFI2, SRRT, CD44, and CLK1 has been associated with metastatic phenotype in breast cancer and poor prognosis in patients [128]. Notably, splicing of hMENA may improve the early diagnosis of breast cancer and clinical decision [104], whereas the balance between splicing variants of KLF6 and caspase-9 genes could be useful to predict the susceptibility of cancer cells to chemotherapy [129, 130].

Along this line, a SpliceDisease database (, which provides information for relationships among gene mutations, splicing defects, and disease, has been recently developed [131]. A list of cancer-specific alternative splicing isoforms is shown in Table 1.

GeneSplice variantCancer typeFunctionReference

ABCC1 Various internal deletionsOvarian cancerDrug resistance[127]
Mdm2 Various internal deletionsOvarian cancerLoss of p53 binding[127]
Fibronectin Exclusion of EDB exonOvarian cancerTumor angiogenesis[127]
MENA Exclusion of exon 6Breast cancerIncrease invasiveness and drug resistance[104]
MENA Skipping of exon 11ABreast cancerEnhance EMT[103, 106]
Ron Skipping of exon 11Colon and gastric breast cancerIncrease motility and invasion[64]
HDMX Exclusion of exon 6Soft-tissue sarcomaIncrease tumor aggressiveness[132]
p73 Inclusion of exon 13Prostate cancerProstate hyperplasia and malignancy[133]
CASP9 Exclusion of a four-exon cassetteNon–small cell lung cancerSusceptibility to chemotherapy[134]
CASP8 Retained intronBreast cancerInhibition of caspase[135]
APC Skipping of exon 4Colon cancerCause familial adenomatous polyposis (FAP)[136]
BRCA1 Skipping of exon 18Breast cancerBreast cancer susceptibility[137]
PTEN Retained introns 3 and 5Breast cancerPathogenesis of sporadic breast cancers with p53[137]
p53 Retained intronBreast cancerTumorigenesis[137]
KLF6 Alternative 5′ ssProstate cancerTumor cell proliferation[82]
NF1 Inclusion of exon 23aNeurofibromatosis type IInactive tumor suppressor[138]
ASIP Alternative 3′ ssHepatocellular carcinomaBlocks Fas-mediated apoptosis[139]
Bcl-X Alternative 5′ ssHepatocellular carcinomaRegulation of apoptosis[140]
TACC1 Exon inclusionGastric cancerAltered centrosome functions[141]
TERT Alternative 3′ ssAstrocytic gliomasRescue of telomerase activity[142]
CDH17 Exclusion of exon 13Hepatocellular carcinomaIncidence of tumor recurrence[143]

Cancer-specific splice variants may not only serve as diagnostic and prognostic tumor biomarkers but also provide potential targets for the development of new therapeutic strategies. Promising avenues towards the development of more selective anticancer drugs are (i) antibodies against tumor-associated markers, (ii) small molecules targeting the spliceosome or trans-acting splicing regulatory factors, and (iii) antisense oligonucleotides that prevent the production of specific aberrant alternative splicing variants.

4.1. Monoclonal Antibodies Targeting Splicing Isoforms

Alternative splicing in cancer can generate unique epitopes in the extracellular domain of cell membrane proteins. Indeed, many receptors involved in cell-cell and cell-matrix interactions undergo alternative splicing and specific splicing isoforms are associated with human malignancies [152]. These novel, or embryo-restricted, epitopes seem to be ideally suited for tumor-targeting strategies consisting in the delivery of bioactive compounds, for example, monoclonal antibodies (mAbs). Binding of mAbs to tumor-associated biomarkers can determine down-regulation or inhibit the function of the target (Figure 1(a)). Moreover, when conjugated with radioemitters or chemotherapics, the mAbs can efficiently ensure in situ delivery of the bioactive molecule to cancer cells, sparing normal tissues.

A very well studied target for the mAbs-mediated therapy is the Epidermal Growth Factor Receptor (EGFR), which is over-expressed in several tumors [153]. Two antibodies directed against the EGFR, cetuximab (C225) and panitumumab, are currently used in therapy [154]. Unfortunately, since EGFR is expressed also in normal tissue, this therapy may have severe side effects. Interestingly, several tumor-specific splice variants of EGFR have been identified. One of this is the EGFRvIII variant, and two mAbs (Ch806 and CH12), targeting the unique extramembrane epitope of EGFRvIII, are used in clinical trial [155, 156]. Another cancer-specific EGFR isoform, de4 EGFR, is also recognized by mAb CH12 [157, 158]. Treatment with CH12, but not with cetuximab, of mice over-expressing the de4 EGFR variant significantly suppresses tumor proliferation and angiogenesis, leading to tumor apoptosis [158].

An important correlation between aberrant alternative splicing and tumor progression has been shown for CD44. In particular, CD44 isoforms containing the variant exon v6 and v8 (CD44v6 or CD44v8) are commonly over-expressed in epithelial tumors [159]. Unfortunately, the expression of these isoforms is not confined to cancer cells, but it occurs also in normal tissues, as skin keratinocytes [160]. Various mAbs targeting CD44v6 have been evaluated in clinical trials [152]. Anti-v6 mAbs are effective in treatment of patients with head and neck squamous cell carcinoma but they show severe skin toxicity [161, 162]. Recently, Masuko and collaborators have developed a mAb (GV5) against CD44R1, a CD44 isoform containing exons v8, v9, and v10 [163]. GV5 exhibited therapeutic effects in xenografts models, probably by inducing antibody-dependent cellular cytotoxicity, with undetectable reactivity with skin keratinocytes. However, despite these promising developments, solid tumors are frequently resistant to antibody-based therapies probably for the poor penetration of antibodies into the tumor tissue. Neo-vascularization (or angiogenesis) is needed for growth of cancer cells and for the metastatic process [22]. Tumor endothelial cells have a central role in this process because they are readily accessible to drugs via the blood circulation. Exploiting this feature, new cancer therapies have been developed to target the tumor vasculature with the aim to deprive the tumor of oxygen and nutrients and induce its regression [164]. Endothelial cells of tumor vessels express splicing isoforms of matrix proteins such as the fibronectin (FN) [165, 166]. For example, the oncofetal isoform containing the extra domain EDB of FN is exclusively expressed around newly developing tumor vasculature, whereas it is absent in adult tissue [165]. Notably, EDB-specific radiolabeled antibodies are used in clinical trial for antiangiogenic cancer treatment [167].

4.2. Small Molecules Targeting Splicing Components

The first drugs used to target the spliceosome machinery, FR901464 and herboxidiene, are natural compounds extracted from bacteria [168, 169]. Subsequently, synthetic analogues, with less complex structure, therefore with minor synthesis costs, but with higher stability, solubility, and activity, have been obtained [168]. All these molecules have been demonstrated to have selective toxicity and anti-cancer properties in human tumor xenografts [168]. Their molecular mechanism has been recently elucidated [170]. They bind to the splicing factor 3b (SF3b), destabilizing the U2 snRNP-pre-mRNA complex and altering the conformation of the branch site sequence. As a consequence, the correct selection of the 3′ splice acceptor site fails to occur and alternatively spliced mRNAs are generated [170]. One more promising antitumor agent characterized for its anti-proliferative activity is the biflavonoid isoginkgetin, a natural product found in a variety of plants [171]. Interestingly, isoginkgetin inhibits the transition from pre-spliceosomal complex A to complex B, probably by preventing stable recruitment of the U4/U5/U6 nuclear ribonucleoproteins [171].

SR proteins are targets of extensive phosphorylation that influences protein interactions and regulates their activity and sub-cellular localization [5] (Figure 1(b)). The benzothiazole compound TG003 has been described as a potent inhibitory of Clk1/Sty able to affect SFSR1-depending alternative splicing events [172]. Interestingly, the exposure of human colon carcinoma cells to TG003 has been described to determine accumulation of the tumor suppressor p53 [173], the most commonly mutated gene in human cancers. Activation of p53 is promoted by down-regulation of MdmX and decreased stability of Mdm2, two key repressors of p53. Interestingly, TG003 seems to contribute to their degradation rather than to change their pre-mRNA splicing. Further studies are required to elucidate the role of p53 pathway as a sensor of alterations in the splicing machinery.

As mentioned before, SRSF1 and SRSF6 control the choice between VEGFxxx (angiogenic) and VEGFxxxb (anti-angiogenic) isoforms. Interestingly, phosphorylation of SRSF1 by SRPK1 promotes the use of the proximal splice site within exon 8 of VEGF pre-mRNA and thus the production of the angiogenic isoform, while phosphorylation of SRSF6 activates the distal splice site in exon 8 [30]. Along this line, inhibitors of SRPK1 and Clk functions, as SRPIN340 or TG003, have been shown to block SRSF1 activation and to inhibit angiogenesis process both in vitro and in vivo [30, 174].

Indole derivatives represent a new class of strong splicing inhibitors able to interact with SR proteins and prevent their phosphorylation [175]. Some of them show anti-proliferative activity, with an acceptable toxicity [175]. In our recent study, we have used indole derivatives to modulate the splicing event that generates the cancer-associated ΔRon variant [176]. Binding of SRSF1 to an ESE sequence within exon 12 leads to skipping of exon 11 and to the production of the constitutively active ΔRon isoform [64]. Interestingly, three indole derivatives can reverse aberrant ΔRon splicing. Among these, only IDC92 is able to revert the invasive phenotype of cancer cells without affecting the splicing profile of other SRSF1 targets, suggesting that this small molecule is suitable for further in vivo studies [176].

Because of their lack of specificity in modulating pre-mRNA splicing, these compounds are expected to cause deleterious undesired events in normal cells as well. Surprisingly, however, most of them have been found to possess selective tumor cytotoxicity. One hypothesis is that tumor cells respond differently from normal cells to changes in mRNA splicing. Alternatively, transformed cells may differ from normal counterparts for the expression of modified version of tumor suppressors originated by aberrant splicing and drug treatment may reverse this defect [168]. However, molecular mechanisms underlying this specificity toward cancerous cells remain elusive and additional studies are necessary to characterize the effects of these drugs in both tumor and normal cells.

Several works have recently demonstrated that also inhibitors of oncogenic pathway components can indirectly target splicing reactions. For example, treatment of melanoma cells, harbouring B-Raf (V600E) mutation with B-RAF inhibitors, determines over-expression of SRSF6 that in turn regulates alternative splicing of the Bim gene, a member of the Bcl-2 family, promoting the production of the proapoptotic short isoform BimS [177, 178].

4.3. Oligonucleotides-Mediated Therapies

Antisense oligonucleotides (ASOs) are short oligonucleotides, usually 15–25 bases in length, that are designed to anneal to a specific target region on a pre-mRNA molecule, thus interfering with the splicing reaction (Figure 1(c)). ASO targeting an exon-intron junction may sterically block the access to the splicing machinery, redirecting splicing reaction to an adjacent splicing site. Alternatively, ASO can bind to splicing enhancer or silencer elements, masking the sequence to trans-acting regulatory factors and determining inclusion or skipping of specific exons.

The latest generations of ASOs contain chemical modifications and appear more stable compared to conventional oligonucleotides. All ASOs share the following characteristics: (i) they bind tightly to RNA through Watson-Crick base-pairs; (ii) they are specific for RNA molecule, and (iii) they do not alter the genomic sequence. In addition, other features make them appreciable therapeutic tools. Indeed, the delivery technology, usually nanoparticle, is noninvasive, nontoxic, efficient, and very stable.

Clinical trials have been already started that exploit ASOs for treatments of human genetic disorders [179]. Even though the use of these molecules in anti-cancer therapy is still at early stages [180], several recent works report therapeutically relevant and encouraging results. Below, we describe several studies, some of them performed on xenograft models of human tumors, while the more recent preliminary results on cancer cell lines are listed in Table 2.


SRA1, Steroid Receptor RNA Activator geneRetention of intron 1 alters the reading frame and occurs in breast tumors with high progesterone receptor contents[144]
Mcl-1, myeloid cell leukemia-1Antiapoptotic protein of the Bcl-2 family overexpressed in many tumors[145]
erbB-2, Her-2 receptorSkipping of exon 19 produces a dominant-negative protein isoform[146]
IG20, death-domain adaptor protein
Insulinoma-Glucagonoma 20
Antiapoptotic alternative splicing isoform expressed in gliomas[147]
CASP9, caspase9Two isoforms generated by alternative splicing: a proapoptotic and a prosurvival variant[148]
PKM, pyruvate kinase MThe PKM2 isoform is crucial for aerobic glycolysis (the Warburg effect) and tumor growth[149, 150]
hTERT, telomeraseAlternative splicing generates many nonfunctional products. ASOs treatment increases nonfunctional telomerase products in cancer cells[151]

The first demonstration of in vivo anti-tumor efficacy of ASOs was reported by Bauman and colleagues [181]. The authors challenged a modified ASO, targeting the downstream 5′ alternative splice site of exon 2 in Bcl-X pre-mRNA (Bcl-X ASO), in a mouse model of metastatic melanoma, an aggressive malignancy that shows poor prognosis when associated with increased expression Bcl-XL splice variant [182]. The oligo efficiently redirected splicing machinery to the upstream 5′ splice site, decreasing the anti-apoptotic Bcl-XL isoform, while increasing the pro-apoptotic Bcl-XS variant [181]. Importantly, the administration of the oligo coupled to nanoparticles produced a significant reduction of tumor burden in rapidly growing and highly tumorigenic lung metastases [181].

Another example is the exploitation of ASOs to efficiently modify splicing of STAT3, another gene involved in apoptosis. The usage of an alternative acceptor site within exon 23 of STAT3 pre-mRNA leads to the production of the truncated STAT3β isoform that promotes apoptosis and cell-cycle arrest [183]. Interestingly, by using a modified ASO, targeting a splicing enhancer element that regulates alternative splicing of exon 23, it was possible to promote a shift from STAT3α to STAT3β leading to tumor regression in a xenograft model of cancer [184].

Recently Cartegni’s group showed that the antagonism/association between intronic polyadenylation and pre-mRNA splicing can produce truncated soluble receptor tyrosine kinases (RTKs). These isoforms can act as dominant-negative regulators since they are deficient of the anchoring transmembrane and the intracellular kinase domains [185]. Notably, these secreted “decoy receptors” are able to inactivate the associated tumorigenic signaling pathways as a consequence of their ability to titrating the ligand or by blocking the wild-type receptors in non-functional heterodimers [185]. Interestingly, in the case of the Vascular Endothelial Growth Factor Receptor 2 (VEGFR2/KDR), the key molecule involved in the control of the VEGF signaling, morpholino antisense oligonucleotides (ASOs extremely stable within biological systems because they are resistant to a wide range of nucleases) were used to induce the expression of dominant-negative secreted VEGFR2/KDR and more importantly to inhibit the angiogenesis process [185].

A new generation of ASOs called TOES (Targeted Oligonucleotide Enhancers of Splicing) have been developed to induce the inclusion of otherwise skipped exons. TOES are complex modified antisense RNA oligonucleotides formed by two functionally distinct regions: the 5′ half of the oligo is complementary to a sequence within an exon of interest and is followed by a non-complementary RNA tail, designed to mimic an ESE sequence (Figure 1(c)). In this manner the oligo recruits specific trans-acting regulatory factors (such as SR proteins) and provides a sort of enhancer in trans that promotes exon inclusion [180, 186]. TOES have been first tested for their ability to induce the inclusion of SMN2 exon 7 in spinal muscular atrophy (SMA) patient fibroblasts [187]. The TOES technology has been so far applied only once to correct splicing in cancer cells [176]. As described before, SRSF1 over-expression produces skipping of Ron exon 11 and the production of the oncogenic ΔRon isoform [176]. In order to correct pathological ΔRon splicing, we have designed a TOES complementary to the first region of exon 11 and containing a tail of GGA repeats, known to function as a strong enhancer. This treatment was able to revert ΔRon splicing and to increase exon 11 inclusion [176], suggesting the exciting possibility to consider splicing of exon 11 as a possible target of new anti-metastatic therapeutic approaches.

Another well-established method to down-regulate a specific splicing isoform is through RNA interference (RNAi). Small interfering RNAs (siRNA) are a class of double-stranded RNA molecules interfering with the expression of specific genes with complementary nucleotide sequence through endonucleases-mediated degradation mechanism [188]. Among the most recent studies on siRNA technology performed in xenograft tumor models, it is worth mentioning the article of Sangodkar and collaborators [130]. KLF6-SV1, an oncogenic splice variant of the tumor suppressor KLF6 gene, is significantly up-regulated in several human cancers [81, 189] and its over-expression is associated with decreased survival in prostate and lung cancers [79, 190]. Sangodkar and colleagues demonstrated that knock-down of this variant via RNAi restored chemotherapy sensitivity and induction of apoptosis in lung cancer cells both in vitro and in vivo [130]. Conversely, over-expression of KLF6-SV1 resulted in a marked reduction in chemotherapy sensitivity in a tumor xenograft model.

Another target for siRNA-mediated anticancer therapy is hnRNP L. Like to SRSF1 [191], hnRNP L binds to a splicing regulatory element and regulates the splicing profile of caspase-9 gene [129], which is altered in a large percentage of human lung cancer [192]. Recently, it has been reported that RNAi-mediated down-regulation of hnRNP L is sufficient to increase the caspase-9a/9b ratio and, more importantly, to cause a complete loss of tumorigenic capacity in xenograft model [192].

Finally, some of ASOs prevent ribosomal assembly and hence mRNA translation and seem to be well tolerated in patients [193]. An example of this approach is provided by survivin, an inhibitor of apoptotic proteins [194]. Survivin is expressed in several human cancers and its over-expression is associated with a poor prognosis [195]. These features make survivin an attractive target for anti-cancer therapy and several efforts, so far unsuccessful, have been made along this line. Recently, down-regulation of survivin has been achieved by using LY2181308, an ASO targeting the translation initiation codon of survivin mRNA and inducing its RNase H-mediated degradation [196]. LY2181308 treatment in multiple cancer cell lines caused apoptosis through activation of caspase-3. Most importantly, in a xenograft tumor model, LY2181308 produced significant anti-tumor activity and sensitized tumor cells to chemotherapeutic-induced apoptosis. All these findings led LY2181308 to be evaluated for clinical trial (Phase II) in combination with docetaxel for the treatment of prostate cancer, acute myeloid leukemia, and non-small cell lung cancer [196, 197].

5. Conclusions

The most important concept opened by the results reviewed here is that the RNA-binding proteins are at the centre of the oncogenic alternative splicing switch that controls all the major aspects of cancer cell biology (Figure 1). Understanding the molecular basis and the effects of the splicing regulation on the transcriptome of cancer cells promises to identify key circuits that have a fundamental role in cell proliferation, apoptosis, and other aspects of tumor progression. Moreover, despite the progress, significant challenges remain towards the rational design of more specific and selective approaches able to modulate alternative splicing events in order to control cancer growth.

In the era of the personalized medicine, each therapy would have to fit the combination of markers specific for each patient. Powerful and cost-effective methods are required to evaluate cancer markers, including those generated by alternative splicing, not only to provide a diagnosis and a prognosis but also to suggest the right personalized therapy.


Serena Bonomi and Stefania Gallo should be considered first authors.


This work was supported by grants from the Associazione Italiana per la Ricerca sul Cancro (AIRC), the Association for International Cancer Research (AICR, UK), to Claudia Ghigna and grants from the Associazione Italiana per la Ricerca sul Cancro (AIRC) and Progetto d’Interesse Invecchiamento (CNR/MIUR) to Giuseppe Biamonti.


  1. P. Early, J. Rogers, and M. Davis, “Two mRNAs can be produced from a single immunoglobulin μ gene by alternative RNA processing pathways,” Cell, vol. 20, no. 2, pp. 313–319, 1980. View at: Google Scholar
  2. F. W. Alt, A. L. M. Bothwell, and M. Knapp, “Synthesis of secreted and membrane-bound immunoglobulin Mu heavy chains is directed by mRNAs that differ at their 3' ends,” Cell, vol. 20, no. 2, pp. 293–301, 1980. View at: Google Scholar
  3. E. T. Wang, R. Sandberg, S. Luo et al., “Alternative isoform regulation in human tissue transcriptomes,” Nature, vol. 456, no. 7221, pp. 470–476, 2008. View at: Publisher Site | Google Scholar
  4. Q. Pan, O. Shai, L. J. Lee, B. J. Frey, and B. J. Blencowe, “Deep surveying of alternative splicing complexity in the human transcriptome by high-throughput sequencing,” Nature Genetics, vol. 40, no. 12, pp. 1413–1415, 2008. View at: Publisher Site | Google Scholar
  5. C. Ghigna, C. Valacca, and G. Biamonti, “Alternative splicing and tumor progression,” Current Genomics, vol. 9, no. 8, pp. 556–570, 2008. View at: Publisher Site | Google Scholar
  6. T. W. Nilsen and B. R. Graveley, “Expansion of the eukaryotic proteome by alternative splicing,” Nature, vol. 463, no. 7280, pp. 457–463, 2010. View at: Publisher Site | Google Scholar
  7. D. D. Licatalosi and R. B. Darnell, “RNA processing and its regulation: global insights into biological networks,” Nature Reviews Genetics, vol. 11, no. 1, pp. 75–87, 2010. View at: Publisher Site | Google Scholar
  8. U. Braunschweig, S. Gueroussov, A. M. Plocik, B. R. Graveley, and B. J. Blencowe, “Dynamic integration of splicing within gene regulatory pathways,” Cell, vol. 152, no. 6, pp. 1252–1269, 2013. View at: Google Scholar
  9. C. J. David and J. L. Manley, “Alternative pre-mRNA splicing regulation in cancer: pathways and programs unhinged,” Genes and Development, vol. 24, no. 21, pp. 2343–2364, 2010. View at: Publisher Site | Google Scholar
  10. G. Biamonti, S. Bonomi, S. Gallo, and C. Ghigna, “Making alternative splicing decisions during epithelial-to-mesenchymal transition (EMT),” Cellular and Molecular Life Sciences, vol. 69, no. 15, pp. 2515–2526, 2012. View at: Publisher Site | Google Scholar
  11. C. He, F. Zhou, Z. Zuo, H. Cheng, and R. Zhou, “A global view of cancer-specific transcript variants by subtractive transcriptome-wide analysis,” PLoS ONE, vol. 4, no. 3, Article ID e4732, 2009. View at: Publisher Site | Google Scholar
  12. M. Jewer, S. D. Findlay, and L. Postovit, “Post-transcriptional regulation in cancer progression: microenvironmental control of alternative splicing and translation,” Journal of Cell Communication and Signaling, vol. 6, no. 4, pp. 233–248, 2012. View at: Google Scholar
  13. D. Hanahan and R. A. Weinberg, “Hallmarks of cancer: the next generation,” Cell, vol. 144, no. 5, pp. 646–674, 2011. View at: Publisher Site | Google Scholar
  14. D. Hanahan and R. A. Weinberg, “The hallmarks of cancer,” Cell, vol. 100, no. 1, pp. 57–70, 2000. View at: Publisher Site | Google Scholar
  15. P. Vaupel, “The role of hypoxia-induced factors in tumor progression,” Oncologist, vol. 9, no. 5, pp. 10–17, 2004. View at: Google Scholar
  16. G. Lorusso and C. Rüegg, “The tumor microenvironment and its contribution to tumor evolution toward metastasis,” Histochemistry and Cell Biology, vol. 130, no. 6, pp. 1091–1103, 2008. View at: Publisher Site | Google Scholar
  17. R. A. Gatenby, E. T. Gawlinski, A. F. Gmitro, B. Kaylor, and R. J. Gillies, “Acid-mediated tumor invasion: a multidisciplinary study,” Cancer Research, vol. 66, no. 10, pp. 5216–5223, 2006. View at: Publisher Site | Google Scholar
  18. R. Cairns, I. Papandreou, and N. Denko, “Overcoming physiologic barriers to cancer treatment by molecularly targeting the tumor microenvironment,” Molecular Cancer Research, vol. 4, no. 2, pp. 61–70, 2006. View at: Publisher Site | Google Scholar
  19. G. L. Semenza, “Targeting HIF-1 for cancer therapy,” Nature Reviews Cancer, vol. 3, no. 10, pp. 721–732, 2003. View at: Google Scholar
  20. C. E. Forristal, K. L. Wright, N. A. Hanley, R. O. C. Oreffo, and F. D. Houghton, “Hypoxia inducible factors regulate pluripotency and proliferation in human embryonic stem cells cultured at reduced oxygen tensions,” Reproduction, vol. 139, no. 1, pp. 85–97, 2010. View at: Publisher Site | Google Scholar
  21. J. T. Erler, K. L. Bennewith, M. Nicolau et al., “Lysyl oxidase is essential for hypoxia-induced metastasis,” Nature, vol. 440, no. 7088, pp. 1222–1226, 2006. View at: Publisher Site | Google Scholar
  22. H. Gerhardt, “VEGF and endothelial guidance in angiogenic sprouting,” Organogenesis, vol. 4, no. 4, pp. 241–246, 2008. View at: Google Scholar
  23. M. Potente, H. Gerhardt, and P. Carmeliet, “Basic and therapeutic aspects of angiogenesis,” Cell, vol. 146, no. 6, pp. 873–887, 2011. View at: Publisher Site | Google Scholar
  24. S. D. Finley and A. S. Popel, “Predicting the effects of anti-angiogenic agents targeting specific VEGF isoforms,” BMC Biology, vol. 14, no. 3, pp. 500–509, 2012. View at: Publisher Site | Google Scholar
  25. Y. Qiu, C. Hoareau-Aveilla, S. Oltean, S. J. Harper, and D. O. Bates, “The anti-angiogenic isoforms of VEGF in health and disease,” Biochemical Society Transactions, vol. 37, no. 6, pp. 1207–1213, 2009. View at: Publisher Site | Google Scholar
  26. C. Hilmi, M. Guyot, and G. Pagès, “VEGF spliced variants: possible role of anti-angiogenesis therapy,” Journal of Nucleic Acids, vol. 2012, Article ID 162692, 7 pages, 2012. View at: Publisher Site | Google Scholar
  27. D. G. Nowak, J. Woolard, E. M. Amin et al., “Expression of pro- and anti-angiogenic isoforms of VEGF is differentially regulated by splicing and growth factors,” Journal of Cell Science, vol. 121, no. 20, pp. 3487–3495, 2008. View at: Publisher Site | Google Scholar
  28. R. Karni, E. De Stanchina, S. W. Lowe, R. Sinha, D. Mu, and A. R. Krainer, “The gene encoding the splicing factor SF2/ASF is a proto-oncogene,” Nature Structural and Molecular Biology, vol. 14, no. 3, pp. 185–193, 2007. View at: Publisher Site | Google Scholar
  29. M. Cohen-Eliav, R. Golan-Gerstl, Z. Siegfried et al., “The splicing factor SRSF6 is amplified and is an oncoprotein in lung and colon cancers,” The Journal of Pathology, vol. 229, no. 4, pp. 630–639, 2013. View at: Google Scholar
  30. D. G. Nowak, E. M. Amin, E. S. Rennel et al., “Regulation of Vascular Endothelial Growth Factor (VEGF) splicing from pro-angiogenic to anti-angiogenic isoforms: a novel therapeutic strategy for angiogenesis,” Journal of Biological Chemistry, vol. 285, no. 8, pp. 5532–5540, 2010. View at: Publisher Site | Google Scholar
  31. G. M. Hayes, P. E. Carrigan, and L. J. Miller, “Serine-arginine protein kinase 1 overexpression is associated with tumorigenic imbalance in mitogen-activated protein kinase pathways in breast, colonic, and pancreatic carcinomas,” Cancer Research, vol. 67, no. 5, pp. 2072–2080, 2007. View at: Publisher Site | Google Scholar
  32. J. E. Weigand, J. Boeckel, P. Gellert, and S. Dimmeler, “Hypoxia-induced alternative splicing in endothelial cells,” PLoS ONE, vol. 7, no. 8, Article ID e42697, 2012. View at: Google Scholar
  33. C. S. Moller-Levet, G. N. J. Betts, A. L. Harris, J. J. Homer, C. M. L. West, and C. J. Miller, “Exon array analysis of head and neck cancers identifies a hypoxia related splice variant of LAMA3 associated with a poor prognosis,” PLoS Computational Biology, vol. 5, no. 11, Article ID e1000571, 2009. View at: Publisher Site | Google Scholar
  34. M. P. Marinkovich, “Tumour microenvironment: laminin 332 in squamous-cell carcinoma,” Nature Reviews Cancer, vol. 7, no. 5, pp. 370–380, 2007. View at: Publisher Site | Google Scholar
  35. M. A. Maynard, H. Qi, J. Chung et al., “Multiple splice variants of the human HIF-3α locus are targets of the von Hippel-Lindau E3 ubiquitin ligase complex,” Journal of Biological Chemistry, vol. 278, no. 13, pp. 11032–11040, 2003. View at: Publisher Site | Google Scholar
  36. H. Ando, A. Natsume, K. Iwami et al. et al., “A hypoxia-inducible factor (HIF)-3α splicing variant, HIF-3α4 impairs angiogenesis in hypervascular malignant meningiomas with epigenetically silenced HIF-3α4,” Biochemical and Biophysical Research Communications, vol. 433, no. 1, pp. 139–144, 2013. View at: Google Scholar
  37. J. A. Menéndez, I. Mehmi, D. W. Griggs, and R. Lupu, “The angiogenic factor CYR61 in breast cancer: molecular pathology and therapeutic perspectives,” Endocrine-Related Cancer, vol. 10, no. 2, pp. 141–152, 2003. View at: Publisher Site | Google Scholar
  38. D. Xie, D. Yin, H.-J. Wang et al., “Levels of expression of CYR61 and CTGF are prognostic for tumor progression and survival of individuals with gliomas,” Clinical Cancer Research, vol. 10, no. 6, pp. 2072–2081, 2004. View at: Publisher Site | Google Scholar
  39. A.-M. Bleau, N. Planque, and B. Perbal, “CCN proteins and cancer: two to tango,” Frontiers in Bioscience, vol. 10, pp. 998–1009, 2005. View at: Google Scholar
  40. M. Hirschfeld, A. Z. Hausen, H. Bettendorf, M. Jäger, and E. Stickeier, “Alternative splicing of Cyr61 Is regulated by hypoxia and significantly changed in breast cancer,” Cancer Research, vol. 69, no. 5, pp. 2082–2090, 2009. View at: Publisher Site | Google Scholar
  41. D. Naor, S. Nedvetzki, I. Golan, L. Melnik, and Y. Faitelson, “CD44 in cancer,” Critical Reviews in Clinical Laboratory Sciences, vol. 39, no. 6, pp. 527–579, 2002. View at: Publisher Site | Google Scholar
  42. H. Ponta, L. Sherman, and P. A. Herrlich, “CD44: from adhesion molecules to signalling regulators,” Nature Reviews Molecular Cell Biology, vol. 4, no. 1, pp. 33–45, 2003. View at: Publisher Site | Google Scholar
  43. V. Orian-Rousseau, “CD44, a therapeutic target for metastasising tumours,” European Journal of Cancer, vol. 46, no. 7, pp. 1271–1277, 2010. View at: Publisher Site | Google Scholar
  44. P. Klingbeil, R. Natrajan, G. Everitt et al., “CD44 is overexpressed in basal-like breast cancers but is not a driver of 11p13 amplification,” Breast Cancer Research and Treatment, vol. 120, no. 1, pp. 95–109, 2010. View at: Publisher Site | Google Scholar
  45. P. Auvinen, R. Tammi, M. Tammi, R. Johansson, and V.-M. Kosma, “Expression of CD44s, CD44v3 and CD44v6 in benign and malignant breast lesions: correlation and colocalization with hyaluronan,” Histopathology, vol. 47, no. 4, pp. 420–428, 2005. View at: Publisher Site | Google Scholar
  46. S. Saito, H. Okabe, M. Watanabe et al. et al., “CD44v6 expression is related to mesenchymal phenotype and poor prognosis in patients with colorectal cancer,” Oncology Reports, vol. 29, no. 4, pp. 1570–1578, 2013. View at: Google Scholar
  47. R. Kopp, M. Fichter, G. Schalhorn, J. Danescu, and S. Classen, “Frequent expression of the high molecular, 673-bp CD44v3,v8-10 variant in colorectal adenomas and carcinomas,” International Journal of Molecular Medicine, vol. 24, no. 5, pp. 677–683, 2009. View at: Publisher Site | Google Scholar
  48. B. Krishnamachary, M. Penet, S. Nimmagadda et al., “Hypoxia regulates CD44 and its variant isoforms through HIF-1α in triple negative breast cancer,” PLoS ONE, vol. 7, no. 8, Article ID e44078, 2012. View at: Google Scholar
  49. M. Hirschfeld, B. Zhang, M. Jaeger et al., “Hypoxia-dependent mRNA expression pattern of splicing factor YT521 and its impact on oncological important target gene expression,” Molecular Carcinogenesis, 2013. View at: Publisher Site | Google Scholar
  50. B. Zhang, A. Z. Hausen, M. Orlowska-Volk et al., “Alternative splicing-related factor YT521: an independent prognostic factor in endometrial cancer,” International Journal of Gynecological Cancer, vol. 20, no. 4, pp. 492–499, 2010. View at: Publisher Site | Google Scholar
  51. S. C. Jeyaraj, D. M. O'Brien, and D. S. Chandler, “MDM2 and MDM4 splicing: an integral part of the cancer spliceome,” Frontiers in Bioscience, vol. 14, no. 7, pp. 2647–2656, 2009. View at: Publisher Site | Google Scholar
  52. J. M. García Pedrero, P. Zuazua, C. Martínez-Campa, P. S. Lazo, and S. Ramos, “The naturally occurring variant of estrogen receptor (ER) ERΔE7 suppresses estrogen-dependent transcriptional activation by both wild-type ERα and ERβ,” Endocrinology, vol. 144, no. 7, pp. 2967–2976, 2003. View at: Publisher Site | Google Scholar
  53. D. J. Farrugia, M. K. Agarwal, V. S. Pankratz et al., “Functional assays for classification of BRCA2 variants of uncertain significance,” Cancer Research, vol. 68, no. 9, pp. 3523–3531, 2008. View at: Publisher Site | Google Scholar
  54. M. Matsuyama, T. Chijiwa, Y. Inoue et al., “Alternative splicing variant of vascular endothelial growth factor-A is a critical prognostic factor in non-small cell lung cancer,” Oncology Reports, vol. 22, no. 6, pp. 1407–1413, 2009. View at: Publisher Site | Google Scholar
  55. D. M. W. Cork, T. W. J. Lennard, and A. J. Tyson-Capper, “Alternative splicing and the progesterone receptor in breast cancer,” Breast Cancer Research, vol. 10, no. 3, article 207, 2008. View at: Publisher Site | Google Scholar
  56. S. Valastyan and R. A. Weinberg, “Tumor metastasis: molecular insights and evolving paradigms,” Cell, vol. 147, no. 2, pp. 275–292, 2011. View at: Publisher Site | Google Scholar
  57. B. De Craene and G. Berx, “Regulatory networks defining EMT during cancer initiation and progression,” Nature Reviews, vol. 13, no. 2, pp. 97–110, 2013. View at: Google Scholar
  58. J. Lim and J. P. Thiery, “Epithelial-mesenchymal transitions: insights from development,” Development, vol. 139, no. 19, pp. 3471–3486, 2012. View at: Google Scholar
  59. K. Polyak and R. A. Weinberg, “Transitions between epithelial and mesenchymal states: acquisition of malignant and stem cell traits,” Nature Reviews Cancer, vol. 9, no. 4, pp. 265–273, 2009. View at: Publisher Site | Google Scholar
  60. J. P. Thiery, H. Acloque, R. Y. J. Huang, and M. A. Nieto, “Epithelial-mesenchymal transitions in development and disease,” Cell, vol. 139, no. 5, pp. 871–890, 2009. View at: Publisher Site | Google Scholar
  61. M. D. Bullock, A. E. Sayan, G. K. Packham, and A. H. Mirnezami, “MicroRNAs: critical regulators of epithelial to mesenchymal (EMT) and mesenchymal to epithelial transition (MET) in cancer progression,” Biology of the Cell/Under the Auspices of the European Cell Biology Organization, vol. 104, no. 1, pp. 3–12, 2012. View at: Google Scholar
  62. C. Wu, Y. Tsai, M. Wu, S. Teng, and K. Wu, “Epigenetic reprogramming and post-transcriptional regulation during the epithelial-mesenchymal transition,” Trends in Genetics, vol. 28, no. 9, pp. 454–463, 2012. View at: Google Scholar
  63. Y.-Q. Zhou, C. He, Y.-Q. Chen, D. Wang, and M.-H. Wang, “Altered expression of the RON receptor tyrosine kinase in primary human colorectal adenocarcinomas: generation of different splicing RON variants and their oncogenic potential,” Oncogene, vol. 22, no. 2, pp. 186–197, 2003. View at: Publisher Site | Google Scholar
  64. C. Ghigna, S. Giordano, H. Shen et al., “Cell motility is controlled by SF2/ASF through alternative splicing of the Ron protooncogene,” Molecular Cell, vol. 20, no. 6, pp. 881–890, 2005. View at: Publisher Site | Google Scholar
  65. C. Valacca, S. Bonomi, E. Buratti et al., “Sam68 regulates EMT through alternative splicing-activated nonsense-mediated mRNA decay of the SF2/ASF proto-oncogene,” Journal of Cell Biology, vol. 191, no. 1, pp. 87–99, 2010. View at: Publisher Site | Google Scholar
  66. P. Bielli, R. Busà, M. P. Paronetto, and C. Sette, “The RNA-binding protein Sam68 is a multifunctional player in human cancer,” Endocrine-Related Cancer, vol. 18, no. 4, pp. R91–R102, 2011. View at: Publisher Site | Google Scholar
  67. K. E. Lukong and S. Richard, “Sam68, the KH domain-containing superSTAR,” Biochimica et Biophysica Acta, vol. 1653, no. 2, pp. 73–86, 2003. View at: Publisher Site | Google Scholar
  68. C. Brignatz, M. P. Paronetto, S. Opi et al., “Alternative splicing modulates autoinhibition and SH3 accessibility in the Src kinase Fyn,” Molecular and Cellular Biology, vol. 29, no. 24, pp. 6438–6448, 2009. View at: Publisher Site | Google Scholar
  69. K. E. Lukong, D. Larocque, A. L. Tyner, and S. Richard, “Tyrosine phosphorylation of Sam68 by breast tumor kinase regulates intranuclear localization and cell cycle progression,” Journal of Biological Chemistry, vol. 280, no. 46, pp. 38639–38647, 2005. View at: Publisher Site | Google Scholar
  70. N. Matter, P. Herrlich, and H. König, “Signal-dependent regulation of splicing via phosphorylation of Sam68,” Nature, vol. 420, no. 6916, pp. 691–695, 2002. View at: Publisher Site | Google Scholar
  71. M. Egeblad and Z. Werb, “New functions for the matrix metalloproteinases in cancer progression,” Nature Reviews Cancer, vol. 2, no. 3, pp. 161–174, 2002. View at: Google Scholar
  72. M. L. Stallings-Mann, J. Waldmann, Y. Zhang et al. et al., “Matrix metalloproteinase induction of Rac1b, a key effector of lung cancer progression,” Science Translational Medicine, vol. 4, no. 142, Article ID 142ra95, 2012. View at: Google Scholar
  73. D. C. Radisky, D. D. Levy, L. E. Littlepage et al., “Rac1b and reactive oxygen species mediate MMP-3-induced EMT and genomic instability,” Nature, vol. 436, no. 7047, pp. 123–127, 2005. View at: Publisher Site | Google Scholar
  74. E. E. Bosco, J. C. Mulloy, and Y. Zheng, “Rac1 GTPase: a “Rac” of all trades,” Cellular and Molecular Life Sciences, vol. 66, no. 3, pp. 370–374, 2009. View at: Publisher Site | Google Scholar
  75. P. Jordan, R. Brazão, M. G. Boavida, C. Gespach, and E. Chastre, “Cloning of a novel human Rac1b splice variant with increased expression in colorectal tumors,” Oncogene, vol. 18, no. 48, pp. 6835–6839, 1999. View at: Google Scholar
  76. A. Schnelzer, D. Prechtel, U. Knaus et al., “Rac1 in human breast cancer: overexpression, mutation analysis, and characterization of a new isoform, Rac1b,” Oncogene, vol. 19, no. 26, pp. 3013–3020, 2000. View at: Google Scholar
  77. B. B. McConnell and V. W. Yang, “Mammalian Krüppel-Like factors in health and diseases,” Physiological Reviews, vol. 90, no. 4, pp. 1337–1381, 2010. View at: Publisher Site | Google Scholar
  78. R. Hatami, A. M. Sieuwerts, S. Izadmehr et al. et al., “KLF6-SV1 drives breast cancer metastasis and is associated with poor survival,” Science Translational Medicine, vol. 5, no. 169, Article ID 169ra12, 2013. View at: Google Scholar
  79. G. Narla, A. DiFeo, Y. Fernandez et al., “KLF6-SV1 overexpression accelerates human and mouse prostate cancer progression and metastasis,” Journal of Clinical Investigation, vol. 118, no. 8, pp. 2711–2721, 2008. View at: Publisher Site | Google Scholar
  80. G. Narla, A. Difeo, S. Yao et al., “Targeted inhibition of the KLF6 splice variant, KLF6 SV1, suppresses prostate cancer cell growth and spread,” Cancer Research, vol. 65, no. 13, pp. 5761–5768, 2005. View at: Publisher Site | Google Scholar
  81. A. DiFeo, G. Narla, J. Hirshfeld et al., “Roles of KLF6 and KLF6-SV1 in ovarian cancer progression and intraperitoneal dissemination,” Clinical Cancer Research, vol. 12, no. 12, pp. 3730–3739, 2006. View at: Publisher Site | Google Scholar
  82. A. DiFeo, J. A. Martignetti, and G. Narla, “The role of KLF6 and its splice variants in cancer therapy,” Drug Resistance Updates, vol. 12, no. 1-2, pp. 1–7, 2009. View at: Publisher Site | Google Scholar
  83. Y. Zhu, G. Xu, A. Patel et al., “Cloning, expression, and initial characterization of a novel cytokine-like gene family,” Genomics, vol. 80, no. 2, pp. 144–150, 2002. View at: Publisher Site | Google Scholar
  84. Z. Li, H. Mou, T. Wang et al. et al., “A non-secretory form of FAM3B promotes invasion and metastasis of human colon cancer cells by upregulating Slug expression,” Cancer Letters, vol. 328, no. 2, pp. 278–284, 2013. View at: Google Scholar
  85. C. E. Robert-Cooperman, J. R. Carnegie, C. G. Wilson et al., “Targeted disruption of pancreatic-derived factor (PANDER, FAM3B) impairs pancreatic β-cell function,” Diabetes, vol. 59, no. 9, pp. 2209–2218, 2010. View at: Publisher Site | Google Scholar
  86. J. R. Carnegie, C. E. Robert-Cooperman, J. Wu, R. A. Young, B. A. Wolf, and B. R. Burkhardt, “Characterization of the expression, localization, and secretion of PANDER in α-cells,” Molecular and Cellular Endocrinology, vol. 325, no. 1-2, pp. 36–45, 2010. View at: Publisher Site | Google Scholar
  87. H.-L. Huang, B.-Y. Wu, S.-B. Yang et al., “Down-regulation of PANDER mRNA in gastric cancer,” World Chinese Journal of Digestology, vol. 16, no. 14, pp. 1513–1518, 2008. View at: Google Scholar
  88. A. J. Ridley, “Life at the leading edge,” Cell, vol. 145, no. 7, pp. 1012–1022, 2011. View at: Publisher Site | Google Scholar
  89. M. Yilmaz and G. Christofori, “EMT, the cytoskeleton, and cancer cell invasion,” Cancer and Metastasis Reviews, vol. 28, no. 1-2, pp. 15–33, 2009. View at: Publisher Site | Google Scholar
  90. B. Gligorijevic, J. Wyckoff, H. Yamaguchi, Y. Wang, E. T. Roussos, and J. Condeelis, “N-WASP-mediated invadopodium formation is involved in intravasation and lung metastasis of mammary tumors,” Journal of Cell Science, vol. 125, no. 3, pp. 724–734, 2012. View at: Publisher Site | Google Scholar
  91. M. A. Eckert, T. M. Lwin, A. T. Chang et al., “Twist1-induced invadopodia formation promotes tumor metastasis,” Cancer Cell, vol. 19, no. 3, pp. 372–386, 2011. View at: Publisher Site | Google Scholar
  92. M. Oser, H. Yamaguchi, C. C. Mader et al., “Cortactin regulates cofilin and N-WASp activities to control the stages of invadopodium assembly and maturation,” Journal of Cell Biology, vol. 186, no. 4, pp. 571–587, 2009. View at: Publisher Site | Google Scholar
  93. R. Buccione, G. Caldieri, and I. Ayala, “Invadopodia: specialized tumor cell structures for the focal degradation of the extracellular matrix,” Cancer and Metastasis Reviews, vol. 28, no. 1-2, pp. 137–149, 2009. View at: Publisher Site | Google Scholar
  94. C. C. Mader, M. Oser, M. A. O. Magalhaes et al., “An EGFR-Src-Arg-cortactin pathway mediates functional maturation of invadopodia and breast cancer cell invasion,” Cancer Research, vol. 71, no. 5, pp. 1730–1741, 2011. View at: Publisher Site | Google Scholar
  95. A. G. S. H. Van Rossum, J. H. De Graaf, E. Schuuring-Scholtes et al., “Alternative splicing of the actin binding domain of human cortactin affects cell migration,” Journal of Biological Chemistry, vol. 278, no. 46, pp. 45672–45679, 2003. View at: Publisher Site | Google Scholar
  96. Y. Liu, L. Conaway, J. Rutherford Bethard et al., “Phosphorylation of the alternative mRNA splicing factor 45 (SPF45) by Clk1 regulates its splice site utilization, cell migration and invasion,” Nucleic Acids Research, vol. 41, no. 9, pp. 4949–4962, 2013. View at: Publisher Site | Google Scholar
  97. A. M. Al-Ayoubi, H. Zheng, Y. Liu, T. Bai, and S. T. Eblen, “Mitogen-activated protein kinase phosphorylation of splicing factor 45 (SPF45) regulates SPF45 alternative splicing site utilization, proliferation, and cell adhesion,” Molecular and Cellular Biology, vol. 32, no. 14, pp. 2880–2893, 2012. View at: Google Scholar
  98. L. Corsini, S. Bonna, J. Basquin et al., “U2AF-homology motif interactions are required for alternative splicing regulation by SPF45,” Nature Structural & Molecular Biology, vol. 14, no. 7, pp. 620–629, 2007. View at: Publisher Site | Google Scholar
  99. N. Martinez-Quiles, H.-Y. H. Ho, M. W. Kirschner, N. Ramesh, and R. S. Geha, “Erk/Src phosphorylation of cortactin acts as a switch on-switch off mechanism that controls its ability to activate N-WASP,” Molecular and Cellular Biology, vol. 24, no. 12, pp. 5269–5280, 2004. View at: Publisher Site | Google Scholar
  100. F. Di Modugno, M. Mottolese, A. Di Benedetto et al., “The cytoskeleton regulatory protein hMena (ENAH) is overexpressed in human benign breast lesions with high risk of transformation and human epidermal growth factor receptor-2-positive/hormonal receptor-negative tumors,” Clinical Cancer Research, vol. 12, no. 5, pp. 1470–1478, 2006. View at: Publisher Site | Google Scholar
  101. F. Di Modugno, G. Bronzi, M. J. Scanlan et al., “Human Mena protein, a serex-defined antigen overexpressed in breast cancer eliciting both humoral and CD8+ T-cell immune response,” International Journal of Cancer, vol. 109, no. 6, pp. 909–918, 2004. View at: Publisher Site | Google Scholar
  102. F. Di Modugno, L. DeMonte, M. Balsamo et al., “Molecular cloning of hMena (ENAH) and its splice variant hMena +11a: epidermal growth factor increases their expression and stimulates hMena+11a phosphorylation in breast cancer cell lines,” Cancer Research, vol. 67, no. 6, pp. 2657–2665, 2007. View at: Publisher Site | Google Scholar
  103. S. Goswami, U. Philippar, D. Sun et al., “Identification of invasion specific splice variants of the cytoskeletal protein Mena present in mammary tumor cells during invasion in vivo,” Clinical and Experimental Metastasis, vol. 26, no. 2, pp. 153–159, 2009. View at: Publisher Site | Google Scholar
  104. F. Di Modugno, P. Iapicca, A. Boudreau et al. et al., “Splicing program of human MENA produces a previously undescribed isoform associated with invasive, mesenchymal-like breast tumors,” Proceedings of the National Academy of Sciences of the United States of America, vol. 109, no. 47, pp. 19280–19285, 2012. View at: Google Scholar
  105. U. Philippar, E. T. Roussos, M. Oser et al., “A Mena invasion isoform potentiates EGF-induced carcinoma cell invasion and metastasis,” Developmental Cell, vol. 15, no. 6, pp. 813–828, 2008. View at: Publisher Site | Google Scholar
  106. E. T. Roussos, M. Balsamo, S. K. Alford et al., “Mena invasive (MenaINV) promotes multicellular streaming motility and transendothelial migration in a mouse model of breast cancer,” Journal of Cell Science, vol. 124, no. 13, pp. 2120–2131, 2011. View at: Publisher Site | Google Scholar
  107. C. C. Warzecha and R. P. Carstens, “Complex changes in alternative pre-mRNA splicing play a central role in the epithelial-to-mesenchymal transition (EMT),” Seminars in Cancer Biology, vol. 22, no. 5-6, pp. 417–427, 2012. View at: Publisher Site | Google Scholar
  108. C. C. Warzecha, P. Jiang, K. Amirikian et al., “An ESRP-regulated splicing programme is abrogated during the epithelial-mesenchymal transition,” EMBO Journal, vol. 29, no. 19, pp. 3286–3300, 2010. View at: Publisher Site | Google Scholar
  109. C. C. Warzecha, S. Shen, Y. Xing, and R. P. Carstens, “The epithelial splicing factors ESRP1 and ESRP2 positively and negatively regulate diverse types of alternative splicing events,” RNA Biology, vol. 6, no. 5, pp. 546–562, 2009. View at: Google Scholar
  110. M. Björklund and E. Koivunen, “Gelatinase-mediated migration and invasion of cancer cells,” Biochimica et Biophysica Acta, vol. 1755, no. 1, pp. 37–69, 2005. View at: Publisher Site | Google Scholar
  111. S. Hauser, L. Bickel, D. Weinspach et al., “Full-length L1CAM and not its δ2δ27 splice variant promotes metastasis through induction of gelatinase expression,” PLoS ONE, vol. 6, no. 4, Article ID e18989, 2011. View at: Publisher Site | Google Scholar
  112. J. E. Talmadge and I. J. Fidler, “AACR centennial series: the biology of cancer metastasis: historical perspective,” Cancer Research, vol. 70, no. 14, pp. 5649–5669, 2010. View at: Publisher Site | Google Scholar
  113. I. Shur, E. Zemer-Tov, R. Socher, and D. Benayahu, “SVEP1 expression is regulated in estrogen-dependent manner,” Journal of Cellular Physiology, vol. 210, no. 3, pp. 732–739, 2007. View at: Publisher Site | Google Scholar
  114. C.-W. Li, W. Xia, L. Huo et al., “Epithelial-mesenchymal transition induced by TNF-α requires NF-κB-mediated transcriptional upregulation of Twist1,” Cancer Research, vol. 72, no. 5, pp. 1290–1300, 2012. View at: Publisher Site | Google Scholar
  115. C. Glait-Santar and D. Benayahu, “Regulation of SVEP1 gene expression by 17β-estradiol and TNFα in pre-osteoblastic and mammary adenocarcinoma cells,” Journal of Steroid Biochemistry and Molecular Biology, vol. 130, no. 1-2, pp. 36–44, 2012. View at: Publisher Site | Google Scholar
  116. C. Glait-Santar, M. Pasmanik-Chor, and D. Benayahu, “Expression pattern of SVEP1 alternatively-spliced forms,” Gene, vol. 505, no. 1, pp. 137–145, 2012. View at: Google Scholar
  117. G. P. Gupta and J. Massagué, “Cancer metastasis: building a framework,” Cell, vol. 127, no. 4, pp. 679–695, 2006. View at: Publisher Site | Google Scholar
  118. D. Trachootham, J. Alexandre, and P. Huang, “Targeting cancer cells by ROS-mediated mechanisms: a radical therapeutic approach?” Nature Reviews Drug Discovery, vol. 8, no. 7, pp. 579–591, 2009. View at: Publisher Site | Google Scholar
  119. O. Nagano, S. Okazaki, and H. Saya, “Redox regulation in stem-like cancer cells by CD44 variant isoforms,” Oncogene, 2013. View at: Publisher Site | Google Scholar
  120. M. Lo, Y.-Z. Wang, and P. W. Gout, “The xc- cystine/glutamate antiporter: a potential target for therapy of cancer and other diseases,” Journal of Cellular Physiology, vol. 215, no. 3, pp. 593–602, 2008. View at: Publisher Site | Google Scholar
  121. T. Yae, K. Tsuchihashi, T. Ishimoto et al. et al., “Alternative splicing of CD44 mRNA by ESRP1 enhances lung colonization of metastatic cancer cell,” Nature Communications, vol. 3, article 883, 2012. View at: Google Scholar
  122. T. Ishimoto, O. Nagano, T. Yae et al., “CD44 variant regulates redox status in cancer cells by stabilizing the xCT subunit of system xc- and thereby promotes tumor growth,” Cancer Cell, vol. 19, no. 3, pp. 387–400, 2011. View at: Publisher Site | Google Scholar
  123. M. Yoshikawa, K. Tsuchihashi, T. Ishimoto et al. et al., “xCT inhibition depletes CD44v-expressing tumor cells that are resistant to EGFR-targeted therapy in head and neck squamous cell carcinoma,” Cancer Research, vol. 73, no. 6, pp. 1855–1866, 2013. View at: Google Scholar
  124. J. P. Venables, J. Brosseau, G. Gadea et al. et al., “RBFOX2 is an important regulator of mesenchymal tissue-specific splicing in both normal and cancer tissues,” Molecular and Cellular Biology, vol. 33, no. 2, pp. 396–405, 2013. View at: Google Scholar
  125. C. M. Misquitta-Ali, E. Cheng, D. O'Hanlon et al., “Global profiling and molecular characterization of alternative splicing events misregulated in lung cancer,” Molecular and Cellular Biology, vol. 31, no. 1, pp. 138–150, 2011. View at: Publisher Site | Google Scholar
  126. R. Menon and G. S. Omenn, “Identification of alternatively spliced transcripts using a proteomic informatics approach,” Methods in Molecular Biology, vol. 696, pp. 319–326, 2011. View at: Google Scholar
  127. R. Klinck, A. Bramard, L. Inkel et al., “Multiple alternative splicing markers for ovarian cancer,” Cancer Research, vol. 68, no. 3, pp. 657–663, 2008. View at: Publisher Site | Google Scholar
  128. A. Bemmo, C. Dias, A. A. N. R. Rose, C. Russo, P. Siegel, and J. Majewski, “Exon-Level transcriptome profiling in murine breast cancer reveals splicing changes specific to tumors with different metastatic abilities,” PLoS ONE, vol. 5, no. 8, Article ID e11981, 2010. View at: Publisher Site | Google Scholar
  129. J. C. Shultz, R. W. Goehe, D. S. Wijesinghe et al., “Alternative splicing of caspase 9 is modulated by the phosphoinositide 3-kinase/Akt pathway via phosphorylation of SRp30a,” Cancer Research, vol. 70, no. 22, pp. 9185–9196, 2010. View at: Publisher Site | Google Scholar
  130. J. Sangodkar, A. DiFeo, L. Feld et al., “Targeted reduction of KLF6-SV1 restores chemotherapy sensitivity in resistant lung adenocarcinoma,” Lung Cancer, vol. 66, no. 3, pp. 292–297, 2009. View at: Publisher Site | Google Scholar
  131. J. Wang, J. Zhang, K. Li, W. Zhao, and Q. Cui, “SpliceDisease database: linking RNA splicing and disease,” Nucleic Acids Research, vol. 40, pp. D1055–D1059, 2012. View at: Google Scholar
  132. F. Bartel, J. Schulz, A. Böhnke et al., “Significance of HDMX-S (or MDM4) mRNA splice variant overexpression and HDMX gene amplification on primary soft tissue sarcoma prognosis,” International Journal of Cancer, vol. 117, no. 3, pp. 469–475, 2005. View at: Publisher Site | Google Scholar
  133. D. A. Arvanitis, E. Lianos, N. Soulitzis, D. Delakas, and D. A. Spandidos, “Deregulation of p73 isoform equilibrium in benign prostate hyperplasia and prostate cancer,” Oncology Reports, vol. 12, no. 5, pp. 1131–1137, 2004. View at: Google Scholar
  134. J. C. Shultz, R. W. Goehe, C. S. Murudkar et al., “SRSF1 regulates the alternative splicing of caspase 9 via a novel intronic splicing enhancer affecting the chemotherapeutic sensitivity of non-small cell lung cancer cells,” Molecular Cancer Research, vol. 9, no. 7, pp. 889–900, 2011. View at: Publisher Site | Google Scholar
  135. A. Mohr, R. M. Zwacka, G. Jarmy et al., “Caspase-8L expression protects CD34+ hematopoietic progenitor cells and leukemic cells from CD95-mediated apoptosis,” Oncogene, vol. 24, no. 14, pp. 2421–2429, 2005. View at: Publisher Site | Google Scholar
  136. D. W. Neklason, C. H. Solomon, A. L. Dalton, S. K. Kuwada, and R. W. Burt, “Intron 4 mutation in APC gene results in splice defect and attenuated FAP phenotype,” Familial Cancer, vol. 3, no. 1, pp. 35–40, 2004. View at: Publisher Site | Google Scholar
  137. N. Okumura, H. Yoshida, Y. Kitagishi, Y. Nishimura, and S. Matsuda, “Alternative splicings on p53, BRCA1 and PTEN genes involved in breast cancer,” Biochemical and Biophysical Research Communications, vol. 413, no. 3, pp. 395–399, 2011. View at: Publisher Site | Google Scholar
  138. V. A. Barron and H. Lou, “Alternative splicing of the neurofibromatosis type I pre-mRNA,” Bioscience Reports, vol. 32, no. 2, pp. 131–138, 2012. View at: Publisher Site | Google Scholar
  139. Y. Hu, C. Fang, and Y. Xu, “The effect of isoforms of the cell polarity protein, human ASIP, on the cell cycle and Fas/FasL-mediated apoptosis in human hepatoma cells,” Cellular and Molecular Life Sciences, vol. 62, no. 17, pp. 1974–1983, 2005. View at: Publisher Site | Google Scholar
  140. T. Takehara, X. Liu, J. Fujimoto, S. L. Friedman, and H. Takahashi, “Expression and role of Bcl-xL in human hepatocellular carcinomas,” Hepatology, vol. 34, no. 1, pp. 55–61, 2001. View at: Publisher Site | Google Scholar
  141. A. Line, Z. Slucka, A. Stengrevics, G. Li, and R. C. Rees, “Altered splicing pattern of TACC1 mRNA in gastric cancer,” Cancer Genetics and Cytogenetics, vol. 139, no. 1, pp. 78–83, 2002. View at: Publisher Site | Google Scholar
  142. V. Kotoula, S. Barbanis, E. Nikolakaki, D. Koufoyannis, C. S. Papadimitriou, and G. Karkavelas, “Relative expression of human telomerase catalytic subunit (hTERT) transcripts in astrocytic gliomas,” Acta Neuropathologica, vol. 107, no. 5, pp. 443–451, 2004. View at: Publisher Site | Google Scholar
  143. X. Q. Wang, J. M. Luk, P. P. Leung, B. W. Wong, E. J. Stanbridge, and S. T. Fan, “Alternative mRNA splicing of liver intestine-cadherin in hepatocellular carcinoma,” Clinical Cancer Research, vol. 11, no. 2, pp. 483–489, 2005. View at: Google Scholar
  144. C. Cooper, J. Guo, Y. Yan et al., “Increasing the relative expression of endogenous non-coding Steroid Receptor RNA Activator (SRA) in human breast cancer cells using modified oligonucleotides,” Nucleic Acids Research, vol. 37, no. 13, pp. 4518–4531, 2009. View at: Publisher Site | Google Scholar
  145. J.-J. Shieh, K.-T. Liu, S.-W. Huang, Y.-J. Chen, and T.-Y. Hsieh, “Modification of alternative splicing of Mcl-1 pre-mRNA using antisense morpholino oligonucleotides induces apoptosis in basal cell carcinoma cells,” Journal of Investigative Dermatology, vol. 129, no. 10, pp. 2497–2506, 2009. View at: Publisher Site | Google Scholar
  146. S. Pankratova, B. N. Nielsen, T. Shiraishi, and P. E. Nielsen, “PNA-mediated modulation and redirection of Her-2 pre-mRNA splicing: specific skipping of erbB-2 exon 19 coding for the ATP catalytic domain,” International Journal of Oncology, vol. 36, no. 1, pp. 29–38, 2010. View at: Publisher Site | Google Scholar
  147. C. V. Lefave, M. Squatrito, S. Vorlova et al., “Splicing factor hnRNPH drives an oncogenic splicing switch in gliomas,” EMBO Journal, vol. 30, no. 19, pp. 4084–4097, 2011. View at: Publisher Site | Google Scholar
  148. J. C. Shultz and C. E. Chalfant, “Caspase 9b: a new target for therapy in non-small-cell lung cancer,” Expert Review of Anticancer Therapy, vol. 11, no. 4, pp. 499–502, 2011. View at: Publisher Site | Google Scholar
  149. M. S. Goldberg and P. A. Sharp, “Pyruvate kinase M2-specific siRNA induces apoptosis and tumor regression,” Journal of Experimental Medicine, vol. 209, no. 2, pp. 217–224, 2012. View at: Publisher Site | Google Scholar
  150. Z. Wang, H. Y. Jeon, F. Rigo, C. F. Bennett, and A. R. Krainer, “Manipulation of PK-M mutually exclusive alternative splicing by antisense oligonucleotides,” Open Biology, vol. 2, no. 10, p. 120133, 2012. View at: Google Scholar
  151. M. S. Wong, L. Chen, C. Foster, R. Kainthla, J. W. Shay, and W. E. Wright, “Regulation of telomerase alternative splicing: a target for chemotherapy,” Cell Reports, vol. 3, no. 4, pp. 1028–1035. View at: Publisher Site | Google Scholar
  152. U. H. Weidle, D. Maisel, S. Klostermann, E. H. Weiss, and M. Schmitt, “Differential splicing generates new transmembrane receptor and extracellular matrix-related targets for antibody-based therapy of cancer,” Cancer Genomics and Proteomics, vol. 8, no. 5, pp. 211–226, 2011. View at: Google Scholar
  153. I. Okamoto, L. C. Kenyon, D. R. Emlet et al., “Expression of constitutively activated EGFRvIII in non-small cell lung cancer,” Cancer Science, vol. 94, no. 1, pp. 50–56, 2003. View at: Publisher Site | Google Scholar
  154. C. Gridelli, P. Maione, M. L. Ferrara, and A. Rossi, “Cetuximab and other anti-epidermal growth factor receptor monoclonal antibodies in the treatment of non-small cell lung cancer,” Oncologist, vol. 14, no. 6, pp. 601–611, 2009. View at: Publisher Site | Google Scholar
  155. A. M. Scott, F.-T. Lee, N. Tebbutt et al., “A phase I clinical trial with monoclonal antibody ch806 targeting transitional state and mutant epidermal growth factor receptors,” Proceedings of the National Academy of Sciences of the United States of America, vol. 104, no. 40, pp. 4071–4076, 2007. View at: Publisher Site | Google Scholar
  156. K. Klausz, S. Berger, J. J. Lammerts van Bueren et al., “Complement-mediated tumor-specific cell lysis by antibody combinations targeting epidermal growth factor receptor (EGFR) and its variant III (EGFRvIII),” Cancer Science, vol. 102, no. 10, pp. 1761–1768, 2011. View at: Publisher Site | Google Scholar
  157. H. Wang, M. Zhou, B. Shi et al., “Identification of an exon 4-deletion variant of epidermal growth factor receptor with increased metastasis-promoting capacity,” Neoplasia, vol. 13, no. 5, pp. 461–471, 2011. View at: Publisher Site | Google Scholar
  158. H. Wang, B. Shi, Q. Zhang et al., “Growth and metastasis suppression of glioma xenografts expressing exon 4-deletion variant of epidermal growth factor receptor by monoclonal antibody CH12-mediated receptor degradation,” FASEB Journal, vol. 26, no. 1, pp. 73–80, 2012. View at: Publisher Site | Google Scholar
  159. S. Seiter, W. Tilgen, K. Herrmann et al., “Expression of CD44 splice variants in human skin and epidermal tumours,” Virchows Archiv, vol. 428, no. 3, pp. 141–149, 1996. View at: Google Scholar
  160. B. Mack and O. Gires, “CD44s and CD44v6 expression in head and neck epithelia,” PLoS ONE, vol. 3, no. 10, Article ID e3360, 2008. View at: Publisher Site | Google Scholar
  161. H. Riechelmann, A. Sauter, W. Golze et al., “Phase I trial with the CD44v6-targeting immunoconjugate bivatuzumab mertansine in head and neck squamous cell carcinoma,” Oral Oncology, vol. 44, no. 9, pp. 823–829, 2008. View at: Publisher Site | Google Scholar
  162. P. K. E. Börjesson, E. J. Postema, J. C. Roos et al., “Phase I therapy study with 186Re-labeled humanized monoclonal antibody BIWA 4 (Bivatuzumab) in patients with head and neck squamous cell carcinoma,” Clinical Cancer Research, vol. 9, no. 10, 2003. View at: Google Scholar
  163. K. Masuko, S. Okazaki, M. Satoh et al., “Anti-tumor effect against human cancer xenografts by a fully human monoclonal antibody to a variant 8-epitope of CD44R1 expressed on cancer stem cells,” PLoS ONE, vol. 7, no. 1, Article ID e29728, 2012. View at: Publisher Site | Google Scholar
  164. P. Carmeliet, “Angiogenesis in life, disease and medicine,” Nature, vol. 438, no. 7070, pp. 932–936, 2005. View at: Publisher Site | Google Scholar
  165. P. Castellani, V. G. Viale g., A. Dorcaratto et al., “The fibronectin isoform containing the ED-B oncofetal domain: a marker of angiogenesis,” International Journal of Cancer, vol. 59, no. 5, pp. 612–618, 1994. View at: Publisher Site | Google Scholar
  166. E. Ventura, F. Sassi, A. Parodi et al., “Alternative splicing of the angiogenesis associated extra-domain B of fibronectin regulates the accessibility of the B-C loop of the type III repeat 8,” PLoS ONE, vol. 5, no. 2, Article ID e9145, 2010. View at: Publisher Site | Google Scholar
  167. M. Czabanka, G. Parmaksiz, S. H. Bayerl et al., “Microvascular biodistribution of L19-SIP in angiogenesis targeting strategies,” European Journal of Cancer, vol. 47, no. 8, pp. 1276–1284, 2011. View at: Publisher Site | Google Scholar
  168. T. R. Webb, A. S. Joyner, and P. M. Potter, “The development and application of small molecule modulators of SF3b as therapeutic agents for cancer,” Drug Discovery Today, vol. 18, no. 1-2, pp. 43–49, 2013. View at: Google Scholar
  169. S. Bonnal, L. Vigevani, and J. Valcárcel, “The spliceosome as a target of novel antitumour drugs,” Nature Reviews, vol. 11, no. 11, pp. 847–859, 2012. View at: Google Scholar
  170. A. Corrionero, B. Miñana, and J. Valcárcel, “Reduced fidelity of branch point recognition and alternative splicing induced by the anti-tumor drug spliceostatin A,” Genes and Development, vol. 25, no. 5, pp. 445–459, 2011. View at: Publisher Site | Google Scholar
  171. K. O'Brien, A. J. Matlin, A. M. Lowell, and M. J. Moore, “The biflavonoid isoginkgetin is a general inhibitor of pre-mRNA splicing,” Journal of Biological Chemistry, vol. 283, no. 48, pp. 33147–33154, 2008. View at: Publisher Site | Google Scholar
  172. M. Muraki, B. Ohkawara, T. Hosoya et al., “Manipulation of alternative splicing by a newly developed inhibitor of Clks,” Journal of Biological Chemistry, vol. 279, no. 23, pp. 24246–24254, 2004. View at: Publisher Site | Google Scholar
  173. N. Allende-Vega, S. Dayal, U. Agarwala, A. Sparks, J.-C. Bourdon, and M. K. Saville, “p53 is activated in response to disruption of the pre-mRNA splicing machinery,” Oncogene, vol. 32, pp. 1–14, 2012. View at: Publisher Site | Google Scholar
  174. E. M. Amin, S. Oltean, J. Hua et al., “WT1 mutants reveal SRPK1 to be a downstream angiogenesis target by altering VEGF splicing,” Cancer Cell, vol. 20, no. 6, pp. 768–780, 2011. View at: Publisher Site | Google Scholar
  175. J. Soret, N. Bakkour, S. Maire et al., “Selective modification of alternative splicing by indole derivatives that target serine-arginine-rich protein splicing factors,” Proceedings of the National Academy of Sciences of the United States of America, vol. 102, no. 24, pp. 8764–8769, 2005. View at: Publisher Site | Google Scholar
  176. C. Ghigna, M. De Toledo, S. Bonomi et al., “Pro-metastatic splicing of Ron proto-oncogene mRNA can be reversed: therapeutic potential of bifunctional oligonucleotides and indole derivatives,” RNA Biology, vol. 7, no. 4, pp. 495–503, 2010. View at: Publisher Site | Google Scholar
  177. F. Lai, C. C. Jiang, M. L. Farrelly, X. D. Zhang, and P. Hersey, “Evidence for upregulation of Bim and the splicing factor SRp55 in melanoma cells from patients treated with selective BRAF inhibitors,” Melanoma Research, vol. 22, no. 3, pp. 244–251, 2012. View at: Publisher Site | Google Scholar
  178. C. C. Jiang, F. Lai, K. H. Tay et al., “Apoptosis of human melanoma cells induced by inhibition of B-RAFV600E involves preferential splicing of bimS,” Cell Death and Disease, vol. 1, no. 9, article e69, 2010. View at: Publisher Site | Google Scholar
  179. F. Muntoni and M. J. A. Wood, “Targeting RNA to treat neuromuscular disease,” Nature Reviews Drug Discovery, vol. 10, no. 8, pp. 621–637, 2011. View at: Publisher Site | Google Scholar
  180. M. A. Havens, D. M. Duelli, and M. L. Hastings, “Targeting RNA splicing for disease therapy,” Wiley Interdisciplinary Reviews, vol. 4, no. 3, pp. 247–266, 2013. View at: Google Scholar
  181. J. A. Bauman, S.-D. Li, A. Yang, L. Huang, and R. Kole, “Anti-tumor activity of splice-switching oligonucleotides,” Nucleic Acids Research, vol. 38, no. 22, pp. 8348–8356, 2010. View at: Publisher Site | Google Scholar
  182. R. Liu, C. Page, D. R. Beidler, M. S. Wicha, and G. Núñez, “Overexpression of Bcl-X(L) promotes chemotherapy resistance of mammary tumors in a syngeneic mouse model,” American Journal of Pathology, vol. 155, no. 6, pp. 1861–1867, 1999. View at: Google Scholar
  183. G. Xu, C. Zhang, and J. Zhang, “Dominant negative STAT3 suppresses the growth and invasion capability of human lung cancer cells,” Molecular Medicine Reports, vol. 2, no. 5, pp. 819–824, 2009. View at: Publisher Site | Google Scholar
  184. F. Zammarchi, E. De Stanchina, E. Bournazou et al., “Antitumorigenic potential of STAT3 alternative splicing modulation,” Proceedings of the National Academy of Sciences of the United States of America, vol. 108, no. 43, pp. 17779–17784, 2011. View at: Publisher Site | Google Scholar
  185. S. Vorlová, G. Rocco, C. V. LeFave et al., “Induction of antagonistic soluble decoy receptor tyrosine kinases by intronic poly A activation,” Molecular Cell, vol. 43, no. 6, pp. 927–939, 2011. View at: Publisher Site | Google Scholar
  186. J. A. Bauman and R. Kole, “Modulation of RNA splicing as a potential treatment for cancer,” Bioengineered Bugs, vol. 2, no. 3, pp. 125–128, 2011. View at: Publisher Site | Google Scholar
  187. L. A. Skordis, M. G. Dunckley, B. Yue, I. C. Eperon, and F. Muntoni, “Bifunctional antisense oligonucleotides provide a trans-acting splicing enhancer that stimulates SMN2 gene expression in patient fibroblasts,” Proceedings of the National Academy of Sciences of the United States of America, vol. 100, no. 7, pp. 4114–4119, 2003. View at: Publisher Site | Google Scholar
  188. S. M. Elbashir, J. Harborth, W. Lendeckel, A. Yalcin, K. Weber, and T. Tuschl, “Duplexes of 21-nucleotide RNAs mediate RNA interference in cultured mammalian cells,” Nature, vol. 411, no. 6836, pp. 494–498, 2001. View at: Publisher Site | Google Scholar
  189. O. Camacho-Vanegas, G. Narla, M. S. Teixeira et al., “Functional inactivation of the KLF6 tumor suppressor gene by loss of heterozygosity and increased alternative splicing in glioblastoma,” International Journal of Cancer, vol. 121, no. 6, pp. 1390–1395, 2007. View at: Publisher Site | Google Scholar
  190. A. DiFeo, L. Feld, E. Rodriguez et al., “A functional role for KLF6-SV1 in lung adenocarcinoma prognosis and chemotherapy response,” Cancer Research, vol. 68, no. 4, pp. 965–970, 2008. View at: Publisher Site | Google Scholar
  191. A. Massiello and C. E. Chalfant, “SRp30a (ASF/SF2) regulates the alternative splicing of caspase-9 pre-mRNA and is required for ceramide-responsiveness,” Journal of Lipid Research, vol. 47, no. 5, pp. 892–897, 2006. View at: Publisher Site | Google Scholar
  192. R. W. Goehe, J. C. Shultz, C. Murudkar et al., “hnRNP L regulates the tumorigenic capacity of lung cancer xenografts in mice via caspase-9 pre-mRNA processing,” Journal of Clinical Investigation, vol. 120, no. 11, pp. 3923–3939, 2010. View at: Publisher Site | Google Scholar
  193. G. R. Devi, T. M. Beer, C. L. Corless, V. Arora, D. L. Weller, and P. L. Iversen, “In vivo bioavailability and pharmacokinetics of a c-MYC antisense phosphorodiamidate morpholino oligomer, AVI-4126, in solid tumors,” Clinical Cancer Research, vol. 11, no. 10, pp. 3930–3938, 2005. View at: Publisher Site | Google Scholar
  194. D. C. Altieri, “Survivin, cancer networks and pathway-directed drug discovery,” Nature Reviews Cancer, vol. 8, no. 1, pp. 61–70, 2008. View at: Publisher Site | Google Scholar
  195. D. C. Altieri, “Validating survivin as a cancer therapeutic target,” Nature Reviews Cancer, vol. 3, no. 1, pp. 46–54, 2003. View at: Publisher Site | Google Scholar
  196. R. A. Carrasco, N. B. Stamm, E. Marcusson, G. Sandusky, P. Iversen, and B. K. R. Patel, “Antisense inhibition of survivin expression as a cancer therapeutic,” Molecular Cancer Therapeutics, vol. 10, no. 2, pp. 221–232, 2011. View at: Publisher Site | Google Scholar
  197. D. C. Talbot, M. Ranson, J. Davies et al., “Tumor survivin is downregulated by the antisense oligonucleotide LY2181308: a proof-of-concept, first-in-human dose study,” Clinical Cancer Research, vol. 16, no. 24, pp. 6150–6158, 2010. View at: Publisher Site | Google Scholar

Copyright © 2013 Serena Bonomi et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

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