- Open Access
The cilia-regulated proteasome and its role in the development of ciliopathies and cancer
Ciliavolume 5, Article number: 14 (2016)
The primary cilium is an essential structure for the mediation of numerous signaling pathways involved in the coordination and regulation of cellular processes essential for the development and maintenance of health. Consequently, ciliary dysfunction results in severe human diseases called ciliopathies. Since many of the cilia-mediated signaling pathways are oncogenic pathways, cilia are linked to cancer. Recent studies demonstrate the existence of a cilia-regulated proteasome and that this proteasome is involved in cancer development via the progression of oncogenic, cilia-mediated signaling. This review article investigates the association between primary cilia and cancer with particular emphasis on the role of the cilia-regulated proteasome.
The precise coordination and regulation of cellular processes is the basis for the development and the homeostasis of a multi-cellular organism. To ensure this high precision, the cell makes use of a special structure that is observed as a 1–10-μm-long cellular evagination—the primary cilium. Simplified, the structure of the cilium consists of three different compartments—the basal body (BB), the axoneme, and the transition zone (TZ). The BB is a remodeled mother centriole from which the ciliary scaffold (axoneme) consisting of circularly arranged nine doublet microtubules arises. The intermediate region from the BB to the axoneme is a short area of 0.5 μm called TZ. The primary cilium plays a decisive role in the initiation of the molecular mechanisms underlying cellular processes like proliferation, apoptosis, migration, differentiation, transcription, and the determination of cell polarity [1, 2]. Consequently, ciliary dysfunction results in severe diseases collectively summarized as ciliopathies. Well-known ciliopathies are: Joubert syndrome (JBTS), Leber’s congenital amaurosis (LCA), Senior–Løken syndrome (SLS), nephronophthisis (NPHP), Meckel–Gruber syndrome (MKS), Bardet–Biedl syndrome (BBS), orofaciodigital syndrome type 1 (OFD1), Alström syndrome (ALS), Jeune asphyxiating thoracic dystrophy (JATD), Ellis–van Creveld syndrome (EVC), and sensenbrenner syndrome (cranioectodermal dysplasia [CED]) . Additionally, cilia are linked to cancer. The current, general view is that, on the one hand, primary cilia mediate oncogenic signaling and, on the other hand, cilia are lost in some types of cancer. In this review article, the role of cilia in cancer development will be discussed with particular regard to the cilia-controlled proteasome. The focus is on the question: What is the significance of the cilia-regulated proteasome in terms of cancerogenesis?
Primary cilia, intercellular signaling, and cancer
Primary cilia mediate intercellular signaling pathways which are involved in the regulation of cellular processes and the formation and maintenance of all organs and structures within the human body. Cancer is characterized by uncontrolled cell division as well as an impaired ability to undergo apoptosis  and because it develops as a result of altered intra- and intercellular signaling, disturbances of cilia-mediated signaling pathways can result in tumor formation [5–7]. While it seems as if canonical WNT signaling is restricted by cilia [8–10], various publications have shown cilia-dependent mediation of sonic hedgehog (SHH), platelet-derived growth factor receptor-α (PDGFRα), NOTCH, transforming growth factor (TGF)-β, and non-canonical WNT signaling (Fig. 1a–e) [8, 11–18].
Of all the investigated associations between primary cilia and signaling pathways, the relationship between primary cilia and SHH signaling is the best studied. In SHH signaling, the 12-pass transmembrane protein patched1 (PTCH1) is located in the ciliary membrane of vertebrates (Fig. 1a). When the SHH ligand binds to its receptor PTCH1, the SHH/PTCH1 complex leaves the cilium. As a consequence, the seven-transmembrane protein smoothened (SMO) is allowed to accumulate in the ciliary membrane and to invoke glioblastoma (GLI) transcription factors. Three GLI isoforms exist in vertebrates—GLI1, 2, and 3. The GLI proteins regulate the expression of SHH target genes and thereby cell proliferation, differentiation, survival and growth [19, 20]. While GLI1 exclusively functions as a constitutive transcriptional activator [21, 22], GLI2 and GLI3 can serve as an activator or a repressor . In the presence of SHH, full-length GLI2 (GLI2-185) and GLI3 (GLI3-190) proteins are converted into a transcriptional activator (GLI2-A and GLI3-A, respectively) most likely by modifications [24, 25]. In the absence of SHH, the full-length proteins can be proteolytically processed into transcriptional repressors (GLI2-R, also known as GLI2-78, and GLI3-R, also known as GLI3-83, respectively) . It was reported that GLI3-R is the predominant repressor of SHH target gene transcription . The ratio of activator and repressor forms regulates cellular processes dependent on SHH signaling.
Similar to SHH signaling, activated PDGF receptors control cellular processes like proliferation, anti-apoptosis, migration, differentiation, actin reorganization, and cell growth [27–29]. The receptor PDGFRα localizes to cilia and undergoes dimerization and phosphorylation after being bound by its ligand PDGF-AA  (Fig. 1b). Stimulation of PDGFRα provokes the activation of signal transduction through the MEK 1/2-ERK 1/2 and AKT/PKB pathways. In the absence of cilia, PDGFRα signaling is inhibited . Additionally, PDGFRα signaling is restricted by the mammalian target of rapamycin (mTOR) signaling pathway [30–32], which is also associated with cilia-mediated signaling. LKB1, a negative regulator of mTOR, localizes to cilia and its action leads to an accumulation of phosphorylated AMPK at the basal body . In turn, the phosphorylation of AMPK results in the inhibition of mTOR signaling via a mechanism that is only poorly understood. Interestingly, deregulation of mTOR signaling has been described in many cancer types [34–36]. Previously, it has been demonstrated that NOTCH signaling depends on primary cilia [16, 17] (Fig. 1c). NOTCH signaling starts when the extracellular domain of a NOTCH ligand, e.g., delta-like1–4 or jagged1–2, binds to the NOTCH receptor (NOTCH1–4) . A ciliary localization was shown for NOTCH1 and NOTCH3 [16, 17]. After the binding event, the NOTCH receptor undergoes a three-step cleavage and finally releases the NOTCH intracellular domain (NIC). Following this, NIC enters the nucleus and interacts with its DNA-binding cofactor RBP-J/CBF1/CSL thereby activating NOTCH target genes. NOTCH signaling controls among other proliferation and differentiation .
Moreover, TGFβ signaling relates to cilia  (Fig. 1d). Both receptors of the pathway, TGFβ-RI and TGFβ-RII, are located at the base of primary cilia. The ligand-induced formation and activation of a heterotetrameric receptor complex composed of TGFβ-RI and TGFβ-RII results in the phosphorylation and activation of the SMAD2 and SMAD3 proteins which are present at the ciliary base . The phosphorylated SMADs 2 and 3 associate with a co-SMAD called SMAD4 that is also detectable at the base of cilia. Subsequently, the complex consisting of SMAD2, 3, and 4 enters the nucleus and activates TGFβ target genes. TGFβ target genes control cellular processes like proliferation, differentiation, morphogenesis, tissue homeostasis, and regeneration .
Primary cilia are also connected to WNT signaling , which can be classified as canonical (β-catenin dependent) or non-canonical (β-catenin independent). In the inactive state of the canonical WNT pathway, a destruction complex consisting of adenomatous polyposis coli (APC) and AXIN triggers the phosphorylation of β-catenin by casein kinase 1 (CK1) and glycogen synthase kinase 3 (GSK3) (Fig. 1e). Afterwards, β-catenin gets phosphorylated, ubiquitinated, and finally degraded . The WNT/β-catenin pathway becomes initiated by binding of WNT ligands to frizzled (FZ) receptors and low density lipoprotein-related proteins 5/6 (LRP 5/6) and leads to the activation of the cytoplasmatic phosphoprotein disheveled (DSH). Subsequently, DSH recruits the destruction complex to the plasma membrane, thereby inhibiting phosphorylation of β-catenin. This operation of DSH enables β-catenin to translocate into the nucleus for activating target gene transcription. Several processes are controlled by canonical WNT signaling: cell fate determination, migration, proliferation, tumor suppression, and self-renewal of stem and progenitor cells [42, 43].
In contrast to canonical WNT signaling, the non-canonical WNT pathway is less well understood. Hence, it is unknown, if β-catenin-independent WNT pathways function as different distinct pathways or if these pathways form a large signaling network . Like the canonical WNT pathway, it starts with a WNT ligand binding to the FZ receptor, but does not require the presence of LRP co-receptors or β-catenin. Non-canonical WNT signals are mediated through intracellular Ca2+ levels and involvement of RHO A, ROCK, and JNK kinase. These factors play an important role in the regulation and remodeling of the cytoskeleton and are greatly involved in the control of planar cell polarity (PCP). PCP is established by intercellular communication that regulates the composition of cells polarizing structures within the plane of a tissue, i.e., stereocilia bundle orientation in the inner ear . In addition to managing cytoskeleton organization, non-canonical WNT signals regulate proliferation and migration .
The restriction of canonical WNT signals by cilia is likely, since DSH is constitutively phosphorylated in Kif3a-negative mice which are unable to assemble cilia . However, non-canonical WNT signaling seems to be mediated by primary cilia [8–10]. One core PCP gene product, van gogh-like 2 (VANGL2), was found in cilia . The ciliary presence of VANGL2  and the finding that VANGL2 is essential for the transduction of WNT5a-induced signals to establish PCP  suggest that non-canonical WNT signaling might be mediated by cilia. This hypothesis is supported by data showing that disruption of BBS protein function leads to ciliary dysfunction along with perturbation of PCP  and that ciliopathy genes interact genetically with VANGL2 [48, 50]. In summary, these data suggest that primary cilia mediate non-canonical WNT signals and limit canonical WNT signaling .
Dysregulation of any of these pathways could lead to oncogenesis. In many cases, upregulation of their target gene expressions led to an increased cell proliferation, which in turn caused tumorigenesis [52–56]. One of the best studied oncogenic signaling pathways is the SHH pathway which was already analyzed in combination with cilia in cancer cells [57, 58]. In 2009, Han et al. and Wong et al. [59, 60] described the role of primary cilia in the development of medulloblastomas and basal cell carcinomas. In regard to SHH signaling, both groups showed that the absence of cilia can protect against tumorigenesis and, in addition, that the presence of cilia can be necessary for the induction of tumors. First, they induced tumorigenesis via a cell type-specific expression of an activated SMO protein. Then, they performed the experiments in mice that were unable to form cilia in the particular cell type for the formation of either medulloblastomas or basal cell carcinomas. In both cases, ciliary deficiency protected against SMO-induced tumorigenesis [59, 60].
Second, the same groups investigated the consequences of constitutively active GLI2 on tumorigenesis [59, 60]. In case of basal cell carcinoma development, constitutively active GLI2 was sufficient to induce carcinogenesis , while, in case of medulloblastoma development, constitutively active GLI2 did not give rise to carcinogenesis . Importantly, the combination of constitutively active GLI2 and loss of cilia led to the formation of medulloblastomas  giving circumstantial evidence that the additional decreased amount of GLI3-R caused by ciliary absence might be necessary to induce oncogenesis. Accordingly, the activation of SHH target gene expression alone is not strong enough for driving the development of some cancer types, but in combination with an inhibited repression of SHH target gene expression by reducing the amount of GLI3-R, activation of SHH target gene expression is sufficient to induce oncogenesis. Possibly, the reason for these differences is that the importance of GLI3-R is different in diverse cancer types. Perhaps, it is even the case that the efficiency of GLI3 processing is different in different cancer types and the amount of GLI3-R varies. A decisive factor for the proteolytic processing of GLI3 is the proteasome.
The proteasome and cancer
The proteasome functions as the catalytic component of the ubiquitin–proteasome system and consists of 19S and 20S subunits (Fig. 1f). Proteins destined to get degraded or proteolytically processed become phosphorylated and ubiquitinated. Polyubiquitin conjugation is realized by a cooperation of an ubiquitin-activating enzyme (E1), an ubiquitin conjugation enzyme (E2), and an ubiquitin ligase (E3). In search of molecular mechanisms underlying carcinogenesis, it was reported that while E1 was never found to be associated with tumor formation, deregulation of E2 and especially E3 was detected in tumors . In some cases, E3 ligases are inactivated leading to a stabilization of oncogene products. In other cases, E3 ligases are overexpressed causing an increased degradation of tumor suppressor proteins . Finally, ubiquitinated proteins bind to the 19S regulatory complex. Hereafter, they are degraded by the multiple peptidase activities containing 20S subunit . Besides the degradation of proteins, the proteasome is able to proteolytically process proteins. A well-studied processing event is the transformation of full-length GLI3 into its shorter repressor form. This process depends on a three-part signal . The first processing signal is the zinc finger domain of the GLI3 protein, which serves as a physical barrier to the proteasome. It prevents degradation of the GLI3 protein and is an essential prerequisite for GLI3 processing. Accordingly, the proteasome is not the factor which distinguishes degradation from processing, but the protein which is degraded or processed determines its fate via its sequence. The linker sequence which expands between the zinc finger domain and the lysines of the degron sequence functions as the second processing signal. Most likely, the proteasome binds to the linker area, which is assumed to be a proteasome initiation region. The degron is the third processing signal and the starting point of proteasomal processing.
In addition to its role in SHH signaling, the proteasome is important for the proper course of several cilia-mediated signaling pathways. It was reported that PDGFRα signaling is upregulated in cancer cells due to an elevated amount of PDGFRα . In these cells, HSP90 and the co-chaperone CDC37 form a complex with PDGFRα, making it inaccessible to proteasomal degradation (Fig. 1b). Previously, it was reported that the amount of PDGFRα could also be decreased in kidney tumors, while the amount of mTOR is increased and mTOR signaling is upregulated [30, 31, 66]. Because mTOR regulates PDGFRα signaling negatively by reducing the amount of PDGFRα  and mTOR governs proteasomal activity positively , it is conceivable that mTOR controls the PDGFRα amount via regulating proteasomal activity. If this hypothesis is true, it could be possible that cancer with a high PDGFRα amount is characterized by downregulated mTOR signaling. As far as we know, the evidence for this possibility has not been found yet. The proteasome is also involved in the regulation of NOTCH signaling, because it controls the NIC amount [68, 69] (Fig. 1c). In lung adenocarcinoma cells, proteasomal degradation of NIC is impaired resulting in enhanced cell proliferation and hence tumorigenesis . Furthermore, TGFβ signaling requires the services of the proteasome. Phosphorylated SMAD2 and SMAD3, the central transducers of the pathway, are inactivated by proteasomal degradation [71, 72] (Fig. 1d). Accordingly, reduced proteasomal degradation of these SMADs gives rise to hyperproliferative diseases like cancer . As previously mentioned, canonical WNT signaling is most likely restricted by primary cilia . At the base of these cilia, the proteasome degrades β-catenin that is phosphorylated at Ser33, Ser37, and Thr41 [47, 50] (Fig. 1e). In some tumors, this kind of phosphorylation is prevented by mutations resulting in a stabilization of β-catenin which then is able to activate the transcription of many oncogenes [73, 74]. Consequently, canonical WNT signaling is not only restricted by primary cilia but also by proteasomal degradation of β-catenin. As opposed to the just described signaling pathways, an essential role of the proteasome in non-canonical WNT signaling has never been described.
In sum, a decreased proteasomal activity causes a deregulation of signaling pathways, leading to an increased cell proliferation resulting in the development of cancer. However, numerous studies show that proteasomal activity is enhanced in cancer cells [75–89] representing an obvious discrepancy. A plethora of point mutations in cancer genomes lead to a very high number of misfolded proteins . It was hypothesized that the cell faces this enormous boost of useless and even harmful proteins with enhanced proteasome-mediated degradation . Moreover, estimates suggest that 90 % of human solid tumors comprise cells with more than two copies of one or more chromosomes . For this reason, a huge surplus of proteins is produced in these cells resulting in a cellular protein imbalance [93, 94]. Consequently, many proteins are not able to form a stable conformation and get degraded by the proteasome [95, 96]. Thus, cancer cells show an increased proteasomal activity due to various reasons. This phenomenon has been designated as “proteotoxic crisis” . Based on this knowledge, proteasome inhibitors are used in anti-cancer therapies .
However, there is a unique class of cancer cells with a decreased proteasomal activity in which the use of proteasome inhibitors would be counterproductive. Reduced proteasomal activity is a hallmark of several cancer stem cells (CSCs) [98–103]. In contrast, glioma stem-like cells (GSCs) show an increase of proteasomal activity  suggesting that proteasomal activity may vary among types of CSCs. But it is doubtful whether GSCs belong to the group of CSCs because they maintain only some properties of CSCs . CSCs (also known as cancer-initiating cells) are part of a new understanding in terms of tumorigenesis. In contrast to the “stochastic model” in which every cancer cell of a tumor is capable of repopulating the entire tumor because of its property of self-renewal, this model conveys the idea that only a small group of cancer cells (CSCs) within a tumor has the ability to repopulate the tumor and that the progeny of these cells loses this ability [106–109]. Even in the course of chemotherapy, CSCs are able to survive and initiate the re-growth of tumors [110, 111]. Thus, CSCs are the reason for the resistance of tumors to conventional anti-cancer therapies. Consequently, it is a challenging task for the current research to develop new anti-cancer therapies which target CSCs . In the development of this type of anti-cancer therapies, a broad spectrum of pharmaceutical compounds were tested. Interestingly, natural dietary compounds came into focus . Since proteasomal activity is reduced in most CSCs and since the decisive signals thought to underlie the self-renewal mechanism of the CSCs are, inter alia, SHH signaling, PDGFRα signaling, NOTCH signaling, TGFβ signaling, and WNT signaling [106, 113–119], one of these compounds is sulforaphane (SFN; 1-isothiocyanato-4(R)-methylsulfinylbutane), an ingredient of broccoli, which functions as a proteasome activator . In 2010, Li et al.  tested the effect of SFN on breast cancer cells. They came up with the conclusion that the SFN treatment downregulated canonical WNT signaling by promoting proteasomal degradation of β-catenin in CSCs. The SFN treatment eliminated breast CSCs , indicating that the decreased proteasomal activity is essential for the survival of CSCs and that SFN could be an effective drug in anti-cancer stem cell therapies.
Primary cilia and the proteasome
After reviewing the connections between primary cilia and cancer, as well as the proteasome and cancer, the relationship between primary cilia and the proteasome should be investigated in order to determine the molecular mechanisms underlying cancer development. As early as 2003, it was suggested that although proteasomes exist almost ubiquitously within the cytoplasm and the nucleus, “their function is likely to be different at different cellular locations” and that “this probably depends on post-translational modifications of proteasomal subunits and on their association and interaction with specific regulatory proteins” . In 2007, Gerdes et al.  reported that the ciliary protein BBS4 is involved in the proteasomal degradation of cytoplasmic β-catenin, the mediator of canonical WNT signaling. In the following years, interactions of a whole range of ciliary proteins with proteasomal components were identified (Table 1) indicating a possible link between cilia and the proteasome. In this context, it was shown that the ciliary proteins BBS1, BBS2, BBS4, BBS6, BBS7, BBS8, and OFD1 interact directly with different proteasomal components . The loss of BBS4, BBS7, and OFD1 leads to a reduced proteasomal activity, respectively, impairing intercellular signaling pathways [50, 122, 123]. In search of the molecular reason for the depleted proteasomal activity, Liu et al.  measured a decreased amount of different proteasomal components in the absence of BBS4 and OFD1, respectively, demonstrating that these proteins control the composition of the proteasome. Since all these proteins localize to the basal body which is equivalent to the mother centriole in ciliary absence, the authors of this study refer to the effect of these proteins on the “centrosomal proteasome” . The existence of a centrosome-associated proteasome was already shown before [124, 125]. Thus, the question arises whether the cilium is important for proteasomal function or whether it rests on the centrosome alone to regulate proteasomal activity. Three components of the 19S proteasomal subunit (PSMD2, PSMD3, and PSMD4) were detected at the BB of mouse embryonic fibroblast (MEF) cilia . However, the detection of proteasomal components at the BB is not sufficient to answer this question; it might be that the centrosomal and the putative ciliary proteasome (a proteasome that functions cilia dependent) are one and the same. Remarkably, a component of the 20S proteasomal subunit (PSMA5) was found along the whole cilium increasing the likelihood of a ciliary involvement in proteasome assembly or function . Interestingly, the ubiquitin conjugation system has been described in flagella of the single-cell green alga Chlamydomonas reinhardtii but, in contrast to the cilia of MEFs, no proteasomal components were detected in these flagella  indicating that the potential ciliary proteasome developed later in evolution and might even be vertebrate specific. Using the G-LAP-Flp purification strategy in mammalian cell lines  which ensures high-confidence proteomics, numerous interactions of the transition zone proteins INVS (also known as NPHP2), IQCB1 (also known as NPHP5), and RPGRIP1L (also known as FTM, NPHP8, or MKS5) with different components of the proteasome were detected . It was already shown that these three proteins are located at the centrosomes during mitosis [126, 129–132] enabling a putative interaction with a component of the centrosomal proteasome. In Rpgrip1l-negative MEFs and limbs of mouse embryos, a reduced proteasomal activity was quantified at the ciliary base. In contrary to the situation in the absence of BBS4 and OFD1 which was characterized by a reduced overall cellular proteasomal activity, RPGRIP1L deficiency results in a decreased proteasomal activity exclusively at the base of cilia (in ciliary absence, the proteasomal activity at centrosomes of Rpgrip1l −/− MEFs is unaltered) demonstrating the existence of a ciliary proteasome [122, 126]. This study could draw the attention from the connection between centrosome and proteasome to the link between primary cilia and proteasome. Contrary to the situation in the absence of BBS4 and OFD1 which was characterized by a depletion of proteasomal components, RPGRIP1L deficiency results in an accumulation of proteasomal 19S and 20S subunit components at the ciliary base [122, 126]. Another difference between these ciliary proteins is the choice of their proteasomal interaction partners. While RPGRIP1L and OFD1 have been shown to interact with components of the 19S proteasomal subunit, BBS4 interacts with components of the 19S as well as 20S proteasomal subunits (Table 1). All these findings indicate that ciliary proteins use different mechanisms with which they regulate proteasomal activity.
Mutations in RPGRIP1L, BBS4, and OFD1 give rise to very severe ciliopathies which often lead to death in men and mice [133–143]. These ciliary proteins regulate proteasomal activity [50, 122, 126] and the proteasome is involved in the development and function of numerous organs and structures of the human body [144–146]. Therefore, reduced activity of the cilia-regulated proteasome is a potential cause of ciliopathies. Appropriately, in silico studies using a systematic network-based approach to work out the “cilia/centrosome complex interactome (CCCI)” revealed that the greatest community of the CCCI is composed of proteasomal components . Thus, it is likely that the relationship between ciliary proteins and the proteasome is of great importance. Further evidence for this importance is given by rescue experiments in vivo. The injection of proteasomal component mRNA or SFN treatment restored defective convergent extension and somatic definition in zebrafish embryos treated with bbs4 or ofd1 morpholinos . Additionally, it could be shown that the introduction of a constitutively active Gli3-R protein (Gli3Δ699) rescues telencephalic patterning, olfactory bulb morphogenesis, and the agenesis of the corpus callosum in Rpgrip1l-negative mouse embryos [148, 149]. Together, these data demonstrate that a decreased activity of the cilia-regulated proteasome is responsible for the development of ciliopathies in these model organisms. Future studies should address if this is also true for human ciliopathies.
Does the cilia-regulated proteasome play a role in the development of cancer?
Several studies have focused on the association between cancer and ciliary presence [150–160]. Since a reduced number of cilia was detected in different cancer types [57–60, 150–156, 158, 159, 161], it was reported that tumorigenesis results in a reduced cilia frequency in some cancer types. Until now, it is unknown why some cancer cell types possess cilia and others not (Table 2). Although the absence of cilia is able to correct effects of an oncogenic initiating event that lies upstream of ciliary action [59, 60], the loss of cilia is not the only solution to treat cancerogenesis. If the oncogenic initiating event lies downstream of ciliary action, therapeutic targeting of cilia would not help in the development of cancer therapies. Accordingly, genetic screening for the oncogenic initiator might be the most important point to design effective anti-cancer therapies. In this context, it would be an interesting question for future investigations whether ciliary genes are mutated in patients suffering from cancer. It was previously reported that the ciliary gene RPGRIP1L might serve as a tumor suppressor gene because RPGRIP1L was downregulated in human hepatocellular carcinoma . Mechanistically, RPGRIP1L is thought to suppress tumor cell transformation in part by regulating MAD2, a mitotic checkpoint protein whose inactivation is realized by the proteasome [162, 163]. Since knockdown of RPGRIP1L led to an increased amount of MAD2, the function of RPGRIP1L as a controller of ciliary proteasome activity could be of great importance in the prevention of human hepatocellular carcinoma formation. Proteasomal activity seems to be an important factor in cancerogenesis, since proteasomal activity is altered in many cancer types (Table 3) and the use of proteasome activators and inhibitors as anti-cancer therapeutics showed promising results [100, 164, 165]. In most cancer types, proteasomal activity is elevated [75–89]. Until now, the reason for this increase is unknown. Since mutations of genes encoding ciliary proteins led to a reduced proteasomal activity in ciliopathies of mice and zebrafishes [122, 126], it might seem as if mutations in these genes could only play a role in cancer types with reduced proteasomal activity. However, it was reported that RPGRIP1L controls the ciliary proteasome in MDCK cells negatively opposing the findings in MEFs and embryonic mouse limbs [126, 166]. These findings as well as studies on cilia length argue for a cell type-specific function of RPGRIP1L allowing that mutations in RPGRIP1L cause an increase of ciliary proteasome activity in some organs and a concomitant reduction of this activity in other organs . Theoretically, it is conceivable that an increased amount of ciliary proteins leads to enhanced proteasomal activity. In this regard, a recent study demonstrated that the overexpression of the RPGRIP1L domain, which interacts with the proteasomal component PSMD2, gives rise to an elevated activity of the ciliary proteasome . What remains to be determined is if the increased proteasomal activity found in most cancer types could be due to impaired regulation of proteasomal activity by ciliary proteins.
Another cancer cell type in which the cilia-regulated proteasome might play a leading role is the CSC. Since the loss of ciliary proteins BBS4, BBS7, OFD1, and RPGRIP1L resulted in a reduced proteasomal activity [50, 122, 123, 126] and CSCs lack cilia in addition to a decreased proteasomal activity [98–103, 150], it is quite possible that a reduction of cilia-regulated proteasomal activity causes the development and/or ensures the survival of most CSCs. However, this is more of a meta-analysis. The only kind of CSC reported to lack cilia was a medulloblastoma CSC . Until now, data about the existence of cilia on other CSCs are missing. Consequently, the presence of cilia in CSCs of other cancer types needs to be investigated. To gain insight into the potential relationship between the cilia-regulated proteasome and cancerogenesis, it is necessary to perform comparative investigations focusing on the activity of the ciliary proteasome and the presence of cilia in cancer cells.
Oncogenic signaling pathways are mediated by primary cilia. Consequently, an association between primary cilia and cancer is very likely. Altered proteasomal activity is an often observed feature in cancer cells [75–89, 98–103] and it was demonstrated that ciliary proteins control proteasomal activity [50, 122, 123, 126]. Previously, it was suggested that the dysfunction of the cilia-controlled proteasome is only one contributory factor of the ciliopathic pathology . Thus, an important purpose of future studies will be to reveal the impact of the cilia-regulated proteasome in human ciliopathies. This aim is closely related to the analysis of the cilia-regulated proteasomal activity in cancer. Consequently, cancer therapies could be advanced by targeting cilia. In the context of proteasomal activity, SFN is a promising therapeutic agent for ciliopathies and any form of cancer in which proteasomal activity is reduced. It remains an open question whether the reduced activity in these cancer types corresponds to the cilia-controlled proteasomal activity. The answer to this question could extend the knowledge about oncogenic factors in a significant direction. Interestingly, a characteristic of most CSCs is a decreased proteasomal activity [98–103] making it possible that new insights into the field of cilia and in particular, the cilia-regulated proteasome, help to understand the biology of tumor formation and reformation as well as the therapeutic possibilities to treat various types of cancer. However, even if nearly all CSCs display a reduced proteasomal activity, most cancer types exhibit the exact opposite—an elevated proteasomal activity. There is scant evidence of ciliary dysfunction resulting in an increase of proteasomal activity, but it does not seem to be impossible due to cell type-specific functions of ciliary proteins [126, 166]. In this regard, it would be helpful to know whether the higher proteasomal activity in cancer cells depends on “proteotoxic crisis” or not .
Based on the novelty of the relationship between the primary cilium and the proteasome, it is difficult to make a clear statement to the role of the cilia-regulated proteasome in cancerogenesis. However, this research topic is very promising and the relationship between the cilia-controlled proteasome and cancer holds enormous potential for the development of new anti-cancer therapies.
protein kinase B
adenomatous polyposis coli
cilia/centrosome complex interactome
cell division cycle control protein 37
sensenbrenner syndrome (cranioectodermal dysplasia)
casein kinase 1
cancer stem cell
extracellular signal-regulated kinases
Ellis–van Creveld syndrome
fibroblast growth factor
glioblastoma 2/3 activator
glioblastoma 2/3 repressor
localization and affinity purification
glioma stem-like cell
glycogen synthase kinase 3
heat shock protein 90
IQ motif containing B1
Jeune asphyxiating thoracic dystrophy
C-Jun N-terminal kinases
Leber’s congenital amaurosis
- LRP 5/6:
low density lipoprotein-related proteins 5/6
mitotic arrest deficient 2
Madin-Darby canine kidney cell line
mouse embryonic fibroblasts
mitogen-activated protein kinase
messenger ribonucleic acid
NOTCH intracellular domain
orofaciodigital syndrome type 1
planar cell polarity
platelet-derived growth factor
platelet-derived growth factor receptor-α
proteasome subunit alpha type-5
proteasome 26S subunit, non-ATPase, 2
proteasome 26S subunit, non-ATPase, 3
proteasome 26S subunit, non-ATPase, 4
recombining binding protein suppressor of hairless
- RHO A:
ras homolog gene family, member A
rho-associated protein kinase
retinitis pigmentosa GTPase regulator-interacting protein-1 like
SMA- and MAD-related proteins
transforming growth factor-β
transforming growth factor β receptor I/II
van gogh-like 2
Basten S, Giles R. Functional aspects of primary cilia in signaling, cell cycle and tumorigenesis. Cilia. 2013;2(1):6.
Bisgrove B, Yost H. The roles of cilia in developmental disorders and disease. Development. 2006;133(21):4131–43.
Waters A, Beales P. Ciliopathies: an expanding disease spectrum. Pediatr Nephrol. 2011;26(7):1039–56.
Hanahan D, Weinberg R. Hallmarks of cancer: the next generation. Cell. 2011;144(5):646–74.
Fry A, Leaper M, Bayliss R. The primary cilium: guardian of organ development and homeostasis. Organogenesis. 2014;10(1):62–8.
Oh E, Katsanis N. Context-dependent regulation of Wnt signaling through the primary cilium. J Am Soc Nephrol. 2013;24(1):10–8.
Goetz S, Anderson K. The primary cilium: a signalling centre during vertebrate development. Nat Rev Genet. 2010;11(5):331–44.
Berbari N, O’Connor A, Haycraft C, Yoder B. The primary cilium as a complex signaling center. Curr Biol. 2009;19(13):R526–35.
Lancaster M, Gleeson J. Cystic kidney disease: the role of Wnt signaling. Trends Mol Med. 2010;16(8):349–60.
Wallingford J, Mitchell B. Strange as it may seem: the many links between Wnt signaling, planar cell polarity, and cilia. Genes Dev. 2011;25(3):201–13.
Eggenschwiler J, Anderson K. Cilia and developmental signaling. Annu Rev Cell Dev Biol. 2007;23:345–73.
Corbit K, Aanstad P, Singla V, Norman A, Stainier D, Reiter J. Vertebrate smoothened functions at the primary cilium. Nature. 2005;437(7061):1018–21.
Haycraft C, Banizs B, Aydin-Son Y, Zhang Q, Michaud E, Yoder B. Gli2 and Gli3 localize to cilia and require the intraflagellar transport protein polaris for processing and function. PLoS Genet. 2005;1(4):e53.
Schneider L, Clement C, Teilmann S, Pazour G, Hoffmann E, Satir P, et al. PDGFRalphaalpha signaling is regulated through the primary cilium in fibroblasts. Curr Biol. 2005;15(20):1861–6.
Rohatgi R, Milenkovic L, Scott M. Patched1 regulates hedgehog signaling at the primary cilium. Science. 2007;317(5836):372–6.
Ezratty E, Stokes N, Chai S, Shah A, Williams S, Fuchs E. A role for the primary cilium in Notch signaling and epidermal differentiation during skin development. Cell. 2011;145(7):1129–41.
Leitch C, Lodh S, Prieto-Echagüe V, Badano J, Zaghloul N. Basal body proteins regulate Notch signaling through endosomal trafficking. J Cell Sci. 2014;127(Pt 11):2407–19.
Clement C, Ajbro K, Koefoed K, Vestergaard M, Veland I, Henriques de Jesus M, et al. TGF-β signaling is associated with endocytosis at the pocket region of the primary cilium. Cell Rep. 2013;3(6):1806–14.
Satir P, Pedersen L, Christensen S. The primary cilium at a glance. J Cell Sci. 2010;123(4):499–503.
Ruiz i Altaba A, Sánchez P, Dahmane N. Gli and hedgehog in cancer: tumours, embryos and stem cells. Nat Rev Cancer. 2002;2(5):361–72.
Hynes M, Stone D, Dowd M, Pitts-Meek S, Goddard A, Gurney A, et al. Control of cell pattern in the neural tube by the zinc finger transcription factor and oncogene Gli-1. Neuron. 1997;19(1):15–26.
Ruiz i Altaba A. The works of GLI and the power of hedgehog. Nat Cell Biol. 1999;1(6):E147–8.
Sasaki H, Nishizaki Y, Hui C, Nakafuku M, Kondoh H. Regulation of Gli2 and Gli3 activities by an amino-terminal repression domain: implication of Gli2 and Gli3 as primary mediators of Shh signaling. Development. 1999;126(17):3915–24.
Chen M, Wilson C, Li Y, Law K, Lu C, Gacayan R, et al. Cilium-independent regulation of Gli protein function by Sufu in Hedgehog signaling is evolutionarily conserved. Genes Dev. 2009;23(16):1910–28.
Humke E, Dorn K, Milenkovic L, Scott M, Rohatgi R. The output of Hedgehog signaling is controlled by the dynamic association between Suppressor of Fused and the Gli proteins. Genes Dev. 2010;24(7):670–82.
Wang B, Fallon J, Beachy P. Hedgehog-regulated processing of Gli3 produces an anterior/posterior repressor gradient in the developing vertebrate limb. Cell. 2000;100(4):423–34.
Christensen S, Pedersen S, Satir P, Veland I, Schneider L. The primary cilium coordinates signaling pathways in cell cycle control and migration during development and tissue repair. Curr Top Dev Biol. 2008;85:261–301.
Yun S, Lee M, Ryu J, Song C, Han H. Role of HIF-1alpha and VEGF in human mesenchymal stem cell proliferation by 17 beta-estradiol: involvement of PKC, PI3K/Akt, and MAPKs. Am J Physiol Cell Physiol. 2009;296(2):317–26.
Schild C, Wirth M, Reichert M, Schmid R, Saur D, Schneider G. PI3K signaling maintains c-myc expression to regulate transcription of E2F1 in pancreatic cancer cells. Mol Carcinog. 2009;48(12):1149–58.
Zhang H, Bajraszewski N, Wu E, Wang H, Moseman A, Dabora S, et al. PDGFRs are critical for PI3 K/Akt activation and negatively regulated by mTOR. J Clin Invest. 2007;117(3):730–8.
Zhang H, Cicchetti G, Onda H, Koon H, Asrican K, Bajraszewski N, et al. Loss of Tsc1/Tsc2 activates mTOR and disrupts PI3K-Akt signaling through downregulation of PDGFR. J Clin Invest. 2003;112(8):1223–33.
Umberger N, Caspary T. Ciliary transport regulates PDGF-AA/αα signaling via elevated mammalian target of rapamycin signaling and diminished PP2A activity. Mol Biol Cell. 2015;26(2):350–8.
Boehlke C, Kotsis F, Patel V, Braeg S, Voelker H, Bredt S, et al. Primary cilia regulate mTORC1 activity and cell size through Lkb1. Mol Biol Cell. 2010;12(11):1115–22.
Guertin D, Sabatini D. Defining the role of mTOR in cancer. Cancer Cell. 2007;12(1):9–22.
Pópulo H, Lopes J, Soares P. The mTOR signalling pathway in human cancer. Int J Mol Sci. 2012;13(2):1886–918.
Easton J, Houghton P. mTOR and cancer therapy. Oncogene. 2006;25(48):6436–46.
Hori K, Sen A, Artavanis-Tsakonas S. Notch signaling at a glance. J Cell Sci. 2013;126(Pt 10):2135–40.
Artavanis-Tsakonas S, Rand M, Lake R. Notch signaling: cell fate control and signal integration in development. Science. 1999;284(5415):770–6.
Massagué J. TGFβ signalling in context. Nat Rev Mol Cell Biol. 2012;13(10):616–30.
Germino G. Linking cilia to Wnts. Nat Genet. 2005;37(5):455–7.
Gerdes J, Katsanis N. Ciliary function and Wnt signal modulation. Curr Top Dev Biol. 2008;85:175–95.
Angers S, Moon R. Proximal events in Wnt signal transduction. Nat Rev Mol Cell Biol. 2009;10(7):468–77.
Chien A, Conrad W, Moon R. A Wnt survival guide: from flies to human disease. J Invest Dermatol. 2009;129(7):1614–27.
Lai S, Chien A, Moon R. Wnt/Fz signaling and the cytoskeleton: potential roles in tumorigenesis. Cell Res. 2009;19(5):532–45.
Jones C, Chen P. Primary cilia in planar cell polarity regulation of the inner ear. Curr Top Dev Biol. 2008;85:197–224.
Cheng C, Yeh J, Fan T, Smith S, Charnock-Jones D. Wnt5a-mediated non-canonical Wnt signalling regulates human endothelial cell proliferation and migration. Biochem Biophys Res Commun. 2008;365(2):285–90.
Corbit K, Shyer A, Dowdle W, Gaulden J, Singla V, Chen M, et al. Kif3a constrains beta-catenin-dependent Wnt signalling through dual ciliary and non-ciliary mechanisms. Nat Cell Biol. 2008;10(1):70–6.
Ross A, May-Simera H, Eichers E, Kai M, Hill J, Jagger D, et al. Disruption of Bardet-Biedl syndrome ciliary proteins perturbs planar cell polarity in vertebrates. Nat Genet. 2005;37(10):1135–40.
Gao B, Song H, Bishop K, Elliot G, Garrett L, English M, et al. Wnt signaling gradients establish planar cell polarity by inducing Vangl2 phosphorylation through Ror2. Dev Cell. 2011;20(2):163–76.
Gerdes J, Liu Y, Zaghloul N, Leitch C, Lawson S, Kato M, et al. Disruption of the basal body compromises proteasomal function and perturbs intracellular Wnt response. Nat Genet. 2007;39(11):1350–60.
Simons M, Gloy J, Ganner A, Bullerkotte A, Bashkurov M, Krönig C, et al. Inversin, the gene product mutated in nephronophthisis type II, functions as a molecular switch between Wnt signaling pathways. Nat Genet. 2005;37(5):537–43.
George D. Platelet-derived growth factor receptors: a therapeutic target in solid tumors. Semin Oncol. 2001;28(5 Suppl 17):27–33.
Massagué J. TGFbeta in cancer. Cell. 2008;134(2):215–30.
Nazarenko I, Hede S, He X, Hedrén A, Thompson J, Lindström M, et al. PDGF and PDGF receptors in glioma. Ups J Med Sci. 2012;117(2):99–112.
Taipale J, Beachy P. The Hedgehog and Wnt signalling pathways in cancer. Nature. 2001;411(6835):349–54.
Yuan X, Wu H, Xu H, Xiong H, Chu Q, Yu S, et al. Notch signaling: an emerging therapeutic target for cancer treatment. Cancer Lett. 2015;S0304–3835(15):00565.
Egeberg D, Lethan M, Manguso R, Schneider L, Awan A, Jørgensen T, et al. Primary cilia and aberrant cell signaling in epithelial ovarian cancer. Cilia. 2012;1(1):15.
Fei D, Sanchez-Mejias A, Wang Z, Flaveny C, Long J, Singh S, et al. Hedgehog signaling regulates bladder cancer growth and tumorigenicity. Cancer Res. 2012;72(17):4449–58.
Han Y, Kim H, Dlugosz A, Ellison D, Gilbertson R, Alvarez-Buylla A. Dual and opposing roles of primary cilia in medulloblastoma development. Nat Med. 2009;15(9):1062–5.
Wong S, Seol A, So P, Ermilov A, Bichakjian C, Epstein EJ, et al. Primary cilia can both mediate and suppress Hedgehog pathway-dependent tumorigenesis. Nat Med. 2009;15(9):1055–61.
Kitagawa K, Kotake Y, Kitagawa M. Ubiquitin-mediated control of oncogene and tumor suppressor gene products. Cancer Sci. 2009;100(8):1374–81.
Micel L, Tentler J, Smith P, Eckhardt G. Role of ubiquitin ligases and the proteasome in oncogenesis: novel targets for anticancer therapies. J Clin Oncol. 2013;31(9):1231–8.
Coux O, Tanaka K, Goldberg A. Structure and functions of the 20S and 26S proteasomes. Annu Rev Biochem. 1996;65:801–47.
Schrader E, Harstad K, Holmgren R, Matouschek A. A three-part signal governs differential processing of Gli1 and Gli3 proteins by the proteasome. J Biol Chem. 2011;286(45):39051–8.
Matei D, Satpathy M, Cao L, Lai Y, Nakshatri H, Donner D. The platelet-derived growth factor receptor alpha is destabilized by geldanamycins in cancer cells. J Biol Chem. 2007;282(1):445–53.
Kwiatkowski D, Zhang H, Bandura J, Heiberger K, Glogauer M, elHashemite N, et al. A mouse model of TSC1 reveals sex-dependent lethality from liver hemangiomas, and up-regulation of p70S6 kinase activity in Tsc1 null cells. Hum Mol Genet. 2002;11(5):525–34.
Zhang Y, Nicholatos J, Dreier J, Ricoult S, Widenmaier S, Hotamisligil G, et al. Coordinated regulation of protein synthesis and degradation by mTORC1. Nature. 2014;513(7518):440–3.
McGill M, McGlade C. Mammalian numb proteins promote Notch1 receptor ubiquitination and degradation of the Notch1 intracellular domain. J Biol Chem. 2003;278(25):23196–203.
Öberg C, Li J, Pauley A, Wolf E, Gurney M, Lendahl U. The Notch intracellular domain is ubiquitinated and negatively regulated by the mammalian Sel-10 homolog. J Biol Chem. 2001;276(38):35847–53.
Tang Y, Hu C, Yang H, Cao L, Li Y, Deng P, et al. Rnd3 regulates lung cancer cell proliferation through notch signaling. PLoS One. 2014;9(11):e111897.
Lo R, Massagué J. Ubiquitin-dependent degradation of TGF-beta-activated smad2. Nat Cell Biol. 1999;1(8):472–8.
Fukuchi M, Imamura T, Chiba T, Ebisawa T, Kawabata M, Tanaka K, et al. Ligand-dependent degradation of Smad3 by a ubiquitin ligase complex of ROC1 and associated proteins. Mol Biol Cell. 2001;12(5):1431–43.
Deshaies R. SCF and Cullin/Ring H2-based ubiquitin ligases. Annu Rev Cell Dev Biol. 1999;15:435–67.
Polakis P. Wnt signaling in cancer. Cold Spring Harb Perspect Biol. 2012;4(5). pii: a008052.
Kamat A, Karashima T, Davis D, Lashinger L, Bar-Eli M, Millikan R, et al. The proteasome inhibitor bortezomib synergizes with gemcitabine to block the growth of human 253JB-V bladder tumors in vivo. Mol Cancer Ther. 2004;3(3):279–90.
Papageorgiou A, Kamat A, Benedict W, Dinney C, McConkey D. Combination therapy with IFN-alpha plus bortezomib induces apoptosis and inhibits angiogenesis in human bladder cancer cells. Mol Cancer Ther. 2006;5(12):3032–41.
Konac E, Varol N, Kiliccioglu I, Bilen C. Synergistic effects of cisplatin and proteasome inhibitor bortezomib on human bladder cancer cells. Oncol Lett. 2015;10(1):560–4.
Agyin J, Santhamma B, Nair H, Roy S, Tekmal R. BU-32: a novel proteasome inhibitor for breast cancer. Breast Cancer Res Treat. 2009;11(5):R74.
Bonfili L, Cuccioloni M, Cecarini V, Mozzicafreddo M, Palermo F, Cocci P, et al. Ghrelin induces apoptosis in colon adenocarcinoma cells via proteasome inhibition and autophagy induction. Apoptosis. 2013;18(10):1188–200.
Mackay H, Hedley D, Major P, Townsley C, Mackenzie M, Vincent M, et al. A phase II trial with pharmacodynamic endpoints of the proteasome inhibitor bortezomib in patients with metastatic colorectal cancer. Clin Cancer Res. 2005;11(15):5526–33.
Ao L, Reichel D, Hu D, Jeong H, Kim K, Bae Y et al. Polymer micelle formulations of proteasome inhibitor carfilzomib for improved metabolic stability and anti-cancer efficacy in human multiple myeloma and lung cancer cell lines. J Pharmacol Exp Ther. 2015;[Epub ahead of print].
Zhu W, Liu J, Nie J, Sheng W, Cao H, Shen W, et al. MG132 enhances the radiosensitivity of lung cancer cells in vitro and in vivo. Oncol Rep. 2015;34(4):2083–9.
Bazzaro M, Lee M, Zoso A, Stirling W, Santillan A, Shih I, et al. Ubiquitin-proteasome system stress sensitizes ovarian cancer to proteasome inhibitor-induced apoptosis. Cancer Res. 2006;66(7):3754–63.
Mlynarczuk-Bialy I, Doeppner T, Golab J, Nowis D, Wilczynski G, Parobczak K, et al. Biodistribution and efficacy studies of the proteasome inhibitor BSc2118 in a mouse melanoma model. Transl Oncol. 2014;7(5):570–9.
Bold R, Virudachalam S, McConkey D. Chemosensitization of pancreatic cancer by inhibition of the 26S proteasome. J Surg Res. 2001;100(1):11–7.
Befani C, Vlachostergios P, Hatzidaki E, Patrikidou A, Bonanou S, Simos G, et al. Bortezomib represses HIF-1α protein expression and nuclear accumulation by inhibiting both PI3K/Akt/TOR and MAPK pathways in prostate cancer cells. J Mol Med (Berl). 2012;90(1):45–54.
Davis N, Taber D, Ansari R, Ryan C, George C, Vokes E, et al. Phase II trial of PS-341 in patients with renal cell cancer: a University of Chicago phase II consortium study. J Clin Oncol. 2004;22(1):115–9.
Kondagunta G, Drucker B, Schwartz L, Bacik J, Marion S, Russo P, et al. Phase II trial of bortezomib for patients with advanced renal cell carcinoma. J Clin Oncol. 2004;22(18):3720–5.
Vaziri S, Grabowski D, Hill J, Rybicki L, Burk R, Bukowski R, et al. Inhibition of proteasome activity by bortezomib in renal cancer cells is p53 dependent and VHL independent. Anticancer Res. 2009;29(8):2961–9.
Vogelstein B, Papadopoulos N, Velculescu V, Zhou S, Diaz LJ, Kinzler K. Cancer genome landscapes. Science. 2013;339(6127):1546–58.
Deshaies R. Proteotoxic crisis, the ubiquitin-proteasome system, and cancer therapy. BMC Biol. 2014;12:94.
Weaver B, Cleveland D. Does aneuploidy cause cancer? Curr Opin Cell Biol. 2006;18(6):658–67.
Williams B, Prabhu V, Hunter K, Glazier C, Whittaker C, Housman D, et al. Aneuploidy affects proliferation and spontaneous immortalization in mammalian cells. Science. 2008;322(5902):703–9.
Torres E, Dephoure N, Panneerselvam A, Tucker C, Whittaker C, Gygi S, et al. Identification of aneuploidy-tolerating mutations. Cell. 2010;143(1):71–83.
Warner J, Mitra G, Schwindinger W, Studeny M, Fried H. Saccharomyces cerevisiae coordinates accumulation of yeast ribosomal proteins by modulating mRNA splicing, translational initiation, and protein turnover. Mol Cell Biol. 1985;5(6):1512–21.
Dephoure N, Hwang S, O’Sullivan C, Dodgson S, Gygi S, Amon A, et al. Quantitative proteomic analysis reveals posttranslational responses to aneuploidy in yeast. Elife. 2014;3:e03023.
Grigoreva T, Tribulovich V, Garabadzhiu A, Melino G, Barlev N. The 26S proteasome is a multifaceted target for anti-cancer therapies. Oncotarget. 2015;[Epub ahead of print].
Vlashi E, Kim K, Lagadec C, Donna L, McDonald J, Eghbali M, et al. In vivo imaging, tracking, and targeting of cancer stem cells. J Natl Cancer Inst. 2009;101(5):350–9.
Vlashi E, Lagadec C, Chan M, Frohnen P, McDonald A, Pajonk F. Targeted elimination of breast cancer cells with low proteasome activity is sufficient for tumor regression. Breast Cancer Res Treat. 2013;141(2):197–203.
Li Y, Zhang T. Targeting cancer stem cells with sulforaphane, a dietary component from broccoli and broccoli sprouts. Future Oncol. 2013;9(8):1097–103.
Li Y, Zhang T, Korkaya H, Liu S, Lee H, Newman B, et al. Sulforaphane, a dietary component of broccoli/broccoli sprouts, inhibits breast cancer stem cells. Clin Cancer Res. 2010;16(9):2580–90.
Lagadec C, Vlashi E, Bhuta S, Lai C, Mischel P, Werner M, et al. Tumor cells with low proteasome subunit expression predict overall survival in head and neck cancer patients. BMC Cancer. 2014;14:152.
Li S, Fu J, Watkins D, Srivastava R, Shankar S. Sulforaphane regulates self-renewal of pancreatic cancer stem cells through the modulation of Sonic hedgehog-GLI pathway. Mol Cell Biochem. 2013;373(1–2):217–27.
Bota D, Alexandru D, Keir S, Bigner D, Vredenburgh J, Friedman H. Proteasome inhibition with bortezomib induces cell death in GBM stem-like cells and temozolomide-resistant glioma cell lines, but stimulates GBM stem-like cells’ VEGF production and angiogenesis. J Neurosurg. 2013;119(6):1415–23.
Yamamuro S, Okamoto Y, Sano E, Ochiai Y, Ogino A, Ohta T, et al. Characterization of glioma stem-like cells from human glioblastomas. Int J Oncol. 2015;47(1):91–6.
Reya T, Morrison S, Clarke M, Weissman I. Stem cells, cancer, and cancer stem cells. Nature. 2001;414(6859):105–11.
Lagasse E. Cancer stem cells with genetic instability: the best vehicle with the best engine for cancer. Gene Ther. 2008;15(2):136–42.
Huntly B, Gilliland D. Cancer biology: summing up cancer stem cells. Nature. 2005;435(7046):1169–70.
Beck B, Blanpain C. Unravelling cancer stem cell potential. Nat Rev Cancer. 2013;13(10):727–38.
Dean M, Fojo T, Bates S. Tumour stem cells and drug resistance. Nat Rev Cancer. 2005;5(4):275–84.
Vidal S, Rodriguez-Bravo V, Galsky M, Cordon-Cardo C, Domingo-Domenech J. Targeting cancer stem cells to suppress acquired chemotherapy resistance. Oncogene. 2014;33(36):4451–63.
Li Y, Wicha M, Schwartz S, Sun D. Implications of cancer stem cell theory for cancer chemoprevention by natural dietary compounds. J Nutr Biochem. 2011;22(9):799–806.
Merchant A, Matsui W. Targeting Hedgehog–a cancer stem cell pathway. Clin Cancer Res. 2010;16(12):3130–40.
Holland J, Klaus A, Garratt A, Birchmeier W. Wnt signaling in stem and cancer stem cells. Curr Opin Cell Biol. 2013;25(2):254–64.
Takebe N, Miele L, Harris P, Jeong W, Bando H, Kahn M, et al. Targeting Notch, Hedgehog, and Wnt pathways in cancer stem cells: clinical update. Nat Rev Clin Oncol. 2015;12(8):445–64.
Ajani J, Song S, Hochster H, Steinberg I. Cancer stem cells: the promise and the potential. Semin Oncol. 2015;42(Suppl. 1):S3–17.
Cenciarelli C, Marei H, Zonfrillo M, Pierimarchi P, Paldino E, Casalbore P, et al. PDGF receptor alpha inhibition induces apoptosis in glioblastoma cancer stem cells refractory to anti-Notch and anti-EGFR treatment. Mol Cancer. 2014;13:247.
Karamboulas C, Ailles L. Developmental signaling pathways in cancer stem cells of solid tumors. Biochim Biophys Acta. 2013;1830(2):2481–95.
Chen K, Huang Y, Chen J. Understanding and targeting cancer stem cells: therapeutic implications and challenges. Acta Pharmacol Sin. 2013;34(6):732–40.
Kwak M, Cho J, Huang B, Shin S, Kensler T. Role of increased expression of the proteasome in the protective effects of sulforaphane against hydrogen peroxide-mediated cytotoxicity in murine neuroblastoma cells. Free Radic Biol Med. 2007;43(5):809–17.
Wójcik C, DeMartino G. Intracellular localization of proteasomes. Int J Biochem Cell Biol. 2003;35(5):579–89.
Liu Y, Tsai I, Morleo M, Oh E, Leitch C, Massa F, et al. Ciliopathy proteins regulate paracrine signaling by modulating proteasomal degradation of mediators. J Clin Invest. 2014;124(5):2059–70.
Gascue C, Tan P, Cardenas-Rodriguez M, Libisch G, Fernandez-Calero T, Liu YP, et al. Direct role of Bardet-Biedl syndrome proteins in transcriptional regulation. J Cell Sci. 2012;125(Pt 2):362–75.
Fabunmi R, Wigley W, Thomas P, DeMartino G. Activity and regulation of the centrosome-associated proteasome. J Biol Chem. 2000;275(1):409–13.
Wigley W, Fabunmi R, Lee M, Marino C, Muallem S, DeMartino G, et al. Dynamic association of proteasomal machinery with the centrosome. J Cell Biol. 1999;145(3):481–90.
Gerhardt C, Lier J, Burmühl S, Struchtrup A, Deutschmann K, Vetter M, et al. The transition zone protein Rpgrip1l regulates proteasomal activity at the primary cilium. J Cell Biol. 2015;210(1):115–33.
Huang K, Diener D, Rosenbaum J. The ubiquitin conjugation system is involved in the disassembly of cilia and flagella. J Cell Biol. 2009;186(4):601–13.
Torres J, Miller J, Jackson P. High-throughput generation of tagged stable cell lines for proteomic analysis. Proteomics. 2009;9(10):2888–91.
Sang L, Miller J, Corbit K, Giles R, Brauer M, Otto E, et al. Mapping the NPHP-JBTS-MKS protein network reveals ciliopathy disease genes and pathways. Cell. 2011;145(4):513–28.
Barbelanne M, Song J, Ahmadzai M, Tsang W. Pathogenic NPHP5 mutations impair protein interaction with Cep290, a prerequisite for ciliogenesis. Hum Mol Genet. 2013;22(12):2482–94.
Otto E, Hurd T, Airik R, Chaki M, Zhou W, Stoetzel C, et al. Candidate exome capture identifies mutation of SDCCAG8 as the cause of a retinal-renal ciliopathy. Nat Genet. 2010;42(10):840–50.
Morgan D, Eley L, Sayer J, Strachan T, Yates L, Craighead A, et al. Expression analyses and interaction with the anaphase promoting complex protein Apc2 suggest a role for inversin in primary cilia and involvement in the cell cycle. Hum Mol Genet. 2002;11(26):3345–50.
Delous M, Baala L, Salomon R, Laclef C, Vierkotten J, Tory K, et al. The ciliary gene RPGRIP1L is mutated in cerebello-oculo-renal syndrome (Joubert syndrome type B) and Meckel syndrome. Nat Genet. 2007;39(7):875–81.
Arts H, Doherty D, van Beersum S, Parisi M, Letteboer S, Gorden N, et al. Mutations in the gene encoding the basal body protein RPGRIP1L, a nephrocystin-4 interactor, cause Joubert syndrome. Nat Genet. 2007;39(7):882–8.
Wolf M, Saunier S, O’Toole J, Wanner N, Groshong T, Attanasio M, et al. Mutational analysis of the RPGRIP1L gene in patients with Joubert syndrome and nephronophthisis. Kidney Int. 2007;72(12):1520–6.
Karmous-Benailly H, Martinovic J, Gubler M, Sirot Y, Clech L, Ozilou C, et al. Antenatal presentation of Bardet-Biedl syndrome may mimic Meckel syndrome. Am J Hum Genet. 2005;76(3):493–504.
Macca M, Franco B. The molecular basis of oral-facial-digital syndrome, type 1. Am J Med Genet C Semin Med Genet. 2009;151C(4):318–25.
Bisschoff I, Zeschnigk C, Horn D, Wellek B, Rieß A, Wessels M, et al. Novel mutations including deletions of the entire OFD1 gene in 30 families with type 1 orofaciodigital syndrome: a study of the extensive clinical variability. Hum Mutat. 2013;34(1):237–47.
Bimonte S, De Angelis A, Quagliata L, Giusti F, Tammaro R, Dallai R, et al. Ofd1 is required in limb bud patterning and endochondral bone development. Dev Biol. 2011;349(5):179–91.
Ferrante M, Zullo A, Barra A, Bimonte S, Messaddeq N, Studer M, et al. Oral-facial-digital type I protein is required for primary cilia formation and left-right axis specification. Nat Genet. 2006;38(1):112–7.
Vierkotten J, Dildrop R, Peters T, Wang B, Rüther U. Ftm is a novel basal body protein of cilia involved in Shh signalling. Development. 2007;134(14):2569–77.
Gerhardt C, Lier J, Kuschel S, Rüther U. The ciliary protein Ftm is required for ventricular wall and septal development. PLoS One. 2013;8(2):e57545.
Eichers E, Abd-El-Barr M, Paylor R, Lewis R, Bi W, Lin X, et al. Phenotypic characterization of Bbs4 null mice reveals age-dependent penetrance and variable expressivity. Hum Genet. 2006;120(2):211–26.
Rubinsztein D. The roles of intracellular protein-degradation pathways in neurodegeneration. Nature. 2006;443(7113):780–6.
Breusing N, Arndt J, Voss P, Bresgen N, Wiswedel I, Gardemann A, et al. Inverse correlation of protein oxidation and proteasome activity in liver and lung. Mech Ageing Dev. 2009;130(11–12):748–53.
Wang X, Robbins J. Proteasomal and lysosomal protein degradation and heart disease. J Mol Cell Cardiol. 2014;71:16–24.
Amato R, Morleo M, Giaquinto L, di Bernardo D, Franco B. A network-based approach to dissect the cilia/centrosome complex interactome. BMC Genom. 2014;15:658.
Besse L, Neti M, Anselme I, Gerhardt C, Rüther U, Laclef C, et al. Primary cilia control telencephalic patterning and morphogenesis via Gli3 proteolytic processing. Development. 2011;138(10):2079–88.
Laclef C, Anselme I, Besse L, Catala M, Palmyre A, Baas D, et al. The role of primary cilia in corpus callosum formation is mediated by production of the Gli3 repressor. Hum Mol Genet. 2015;24(17):4997–5014.
Gate D, Danielpour M, Bannykh S, Town T. Characterization of cancer stem cells and primary cilia in medulloblastoma. CNS Neurol Disord Drug Targets. 2015;14(5):600–11.
Menzl I, Lebeau L, Pandey R, Hassounah N, Li F, Nagle R, et al. Loss of primary cilia occurs early in breast cancer development. Cilia. 2014;3:7.
Nobutani K, Shimono Y, Yoshida M, Mizutani K, Minami A, Kono S, et al. Absence of primary cilia in cell cycle-arrested human breast cancer cells. Genes Cells. 2014;19(2):141–52.
Yuan K, Frolova N, Xie Y, Wang D, Cook L, Kwon Y, et al. Primary cilia are decreased in breast cancer: analysis of a collection of human breast cancer cell lines and tissues. J Histochem Cytochem. 2010;58(10):857–70.
Rocha C, Papon L, Cacheux W, Marques Sousa P, Lascano V, Tort O, et al. Tubulin glycylases are required for primary cilia, control of cell proliferation and tumor development in colon. EMBO J. 2014;33(19):2247–60.
Park W, Kim M, Shin D, Lee J, Choi K, Kim J, et al. Ciliated adenocarcinomas of the lung: a tumor of non-terminal respiratory unit origin. Mod Pathol. 2012;25(9):1265–74.
Snedecor E, Sung C, Moncayo A, Rothstein B, Mockler D, Tonnesen M, et al. Loss of primary cilia in melanoma cells is likely independent of proliferation and cell cycle progression. J Invest Dermatol. 2015;135(5):1456–8.
Emoto K, Masugi Y, Yamazaki K, Effendi K, Tsujikawa H, Tanabe M, et al. Presence of primary cilia in cancer cells correlates with prognosis of pancreatic ductal adenocarcinoma. Hum Pathol. 2014;45(4):817–25.
Hassounah N, Nagle R, Saboda K, Roe D, Dalkin B, McDermott K. Primary cilia are lost in preinvasive and invasive prostate cancer. PLoS One. 2013;8(7):e68521.
Basten S, Willekers S, Vermaat J, Slaats G, Voest E, van Diest P, et al. Reduced cilia frequencies in human renal cell carcinomas versus neighboring parenchymal tissue. Cilia. 2013;2(1):2.
Schraml P, Frew I, Thoma C, Boysen G, Struckmann K, Krek W, et al. Sporadic clear cell renal cell carcinoma but not the papillary type is characterized by severely reduced frequency of primary cilia. Mod Pathol. 2009;22(1):31–6.
Schraml P, Frew I, Thoma C, Boysen G, Struckmann K, Krek W, et al. Sporadic clear cell renal cell carcinoma but not the papillary type is characterized by severely reduced frequency of primary cilia. Mod Pathol. 2009;22(1):31–6.
Lin Y, Yan M, Shih Y, Hsieh C. The basal body gene, RPGRIP1L, is a candidate tumour suppressor gene in human hepatocellular carcinoma. Eur J Cancer. 2009;45(11):2041–9.
Ma H, Poon R. Orderly inactivation of the key checkpoint protein mitotic arrest deficient 2 (MAD2) during mitotic progression. J Biol Chem. 2011;286(15):13052–9.
Weathington N, Mallampalli R. Emerging therapies targeting the ubiquitin proteasome system in cancer. J Clin Invest. 2014;124(1):6–12.
Chen D, Dou Q. The ubiquitin-proteasome system as a prospective molecular target for cancer treatment and prevention. Curr Protein Pept Sci. 2010;11(6):459–70.
Mahuzier A, Gaudé H, Grampa V, Anselme I, Silbermann F, Leroux-Berger M, et al. Dishevelled stabilization by the ciliopathy protein Rpgrip1l is essential for planar cell polarity. J Cell Biol. 2012;198(5):927–40.
CG and UR wrote the manuscript. CG and TL compiled the tables. TL and JML designed the illustrations. All authors read and approved the final manuscript.
The authors thank Andreas Struchtrup for his help in regard to literature research and Renate Dildrop for fruitful discussion. Special thanks go to Lauren Biwer, Nen͂a Krüger, Leonie-Alexa Koch, Antonia Wiegering, and André Spychala for critical reading of the manuscript. This work was supported by the Deutsche Forschungsgemeinschaft (Sonderforschungsbereiche 590 and 612) to U. R.
The authors declare that they have no competing interests.