Abstract
Localized, nonindolent prostate cancer (PCa) is characterized by large-scale genomic rearrangements, aneuploidy, chromothripsis, and other forms of chromosomal instability (CIN), yet how this occurs remains unclear. A well-established mechanism of CIN is the overproduction of centrosomes, which promotes tumorigenesis in various mouse models. Therefore, we developed a single-cell assay for quantifying centrosomes in human prostate tissue. Surprisingly, centrosome loss—which has not been described in human cancer—was associated with PCa progression. By chemically or genetically inducing centrosome loss in nontumorigenic prostate epithelial cells, mitotic errors ensued, producing aneuploid, and multinucleated cells. Strikingly, transient or chronic centrosome loss transformed prostate epithelial cells, which produced highly proliferative and poorly differentiated malignant tumors in mice. Our findings suggest that centrosome loss could create a cellular crisis with oncogenic potential in prostate epithelial cells.
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Introduction
Tumorigenic driver mutations, common in other cancers, have not been detected in primary prostate tumors [1,2,3]. Indeed, localized PCa contains an overall low burden of single nucleotide variants, while metastatic PCa has multiple specific recurrently altered genes and pathways [3,4,5,6,7]. Instead, primary PCa displays nuclei with defects in size and DNA content, and enriched with large-scale genomic rearrangements, copy number variations (CNV), changes in DNA methylation patterns, chromothripsis, gene fusions, and other forms of genomic instability [8,9,10]. By analyzing the clonal status of genomic lesions within prostate tumors, a model has been proposed whereby oncogenic genomic alterations occur in a few successive bursts [1]. Mutations accumulate slowly at first, and a subset of driver mutations occurs late in PCa development [1, 11]. Thus, oncogenic events for localized PCa might include an unidentified mechanism, independent of specific driver mutations, to generate an early genomic crisis.
A genomic crisis could arise due to a change to centrosome numbers. Centrosomes are the major microtubule-organizing center in cells, giving rise to a variety of protein machines, including mitotic spindles [12]. At the centrosome core lies a centriole pair that serve as the duplicating elements of the organelle and recruit an organized shell of pericentriolar material possessing microtubule-nucleating activity [13, 14]. Cells exert tight control over centrosome copy number because centrosome overduplication (known as ‘amplification’) or centrosome loss produce cellular dysfunction and disease [15, 16].
Centrosome amplification is recognized as a general feature of tumors, seen in several solid tumors and blood cancers, and correlates with advanced tumor grade, recurrence, and poor survival [17]. Excess centrosomes lead to assembly of transient multipolar spindles with incorrect chromosome attachments [18, 19]. Consequently, anaphase lagging chromatids are produced, forming micronuclei susceptible to chromothripsis [20]. Induction of centrosome amplification in mice promotes tissue hyperplasia, and formation of solid tumors with focal CNV and whole chromosome aneuploidy [21,22,23,24].
In the opposite condition, vertebrate cells lacking centrosomes use an acentrosomal microtubule assembly pathway [25], and their proliferation is dependent on p53 status [26,27,28]. Acentrosomal spindles cause prolonged mitosis as well as mitotic errors including anaphase lagging chromatids, micronuclei, aneuploidy, and polyploidy [27,28,29,30]. Although centrosome amplification and loss have remarkably similar effects in promoting chromosomal instability (CIN), centrosome loss has not been reported in cancer.
Here, we show that human prostate tumors display significant centrosome loss. Moreover, centrosome loss in nontumorigenic prostate epithelial cells results in genomic alterations and malignant mouse xenograft tumors. Our results suggest that centrosome loss is a cellular crisis in prostate cancer (PCa), potentially explaining the presence of large-scale genomic defects without specific recurrent mutations.
Results
Localized prostate tumors display significant centrosome loss with increasing grade
Localized PCa was analyzed for centrosome detection and quantitation using an in situ immunofluorescence microscopy assay developed by us [31]. Since a pair of centrioles form the centrosome core, antibodies were used against centriole protein CEP135 and the PCM protein γ-Tubulin; colocalization of CEP135 and γ-Tubulin foci confirmed our ability to detect bona fide centrosomes (Fig. S1). E-Cadherin staining demarcated epithelial cell borders. Localized PCa shows elevated E-cadherin expression and, although no significant differences in E-Cadherin expression associate with higher Gleason scores [32], we used α6 integrin as an additional membrane marker.
Tissues were imaged in multiple z-sections, and although centrosomes are small, our approach reliably identified cell boundaries and maximized our ability to image entire cell volumes, allowing us to measure centrosomes within individual cells. Normal human prostate glands possess basal and luminal cell layers (Fig. 1a). CEP135 localizes to the proximal end of each centriole within the pair and, as expected, appeared as two distinct spots in the majority of basal and luminal cells (Fig. 1a, f). Each cell contained two CEP135 foci that could be positioned in different z-section planes or within the same focal section (Fig. 1a). Approximately 20% of cells in normal prostate glands contained no centrosomes (Fig. 1f), likely due to the known loss of cell content during tissue sectioning. Surprisingly, Gleason grade 3 PCa exhibited a significant increase in cells lacking centrosomes compared with cells of normal tissue. The proportion of cells devoid of centrosomes increased significantly with each increase of tumor grade: 52% for Gleason grade 4 and 73% for Gleason grade 5. This pattern held true when centrosome numbers are counted using CEP135 or γ-Tubulin foci (Fig. 1b, c, and f). Importantly, centrosomes were readily observed in surrounding normal stromal cells, distinguished as cells lacking E-Cadherin and serving as an internal control (Fig. 1c, yellow arrowheads). Detection of centrosomes in stromal cells demonstrated that our assay can identify centrosomes in cells with small volumes within the same section.
As a further validation for our assay, we quantified centrosomes in triple-negative breast cancer (TNBC), which is known to display centrosome amplification [33]. Compared with normal mammary glands, we confirmed that TNBC contains a significantly higher fraction of cells with >2 CEP135 foci (24%) (Fig. 1d–f). Since TNBCs contain low levels of differentiation markers and lack basal-apical polarity [34], our assay is effective regardless of cell polarity or differentiation status. Thus, unlike most epithelial cancers described to date, centrosomes are lost in localized PCa and in prostate tumors with higher Gleason scores.
PCa cell lines show both centrosome amplification and loss
We next compared centrosome numbers in primary and immortalized nontumorigenic prostate epithelial cells as well as metastatic and neuroendocrine PCa-derived cell lines. Cells were immunostained for CEP135 and CENT3 (an additional centriole marker) or γ-Tubulin, and the numbers of foci per cell were measured. Most prostate epithelial cells (80%), including PEC (primary) as well as PrEC, iPEC37, and RWPE1 (immortalized), contained a normal centrosome count (two CEP135 foci per cell), while few displayed centrosome loss (zero CEP135 foci per cell) or amplification (>2 CEP135 foci per cell) (Fig. 2a–d, j). However, metastasis-derived PCa cell lines displayed either centrosome loss or amplification and could be subclassified by their androgen receptor expression status. Androgen-responsive cell lines, LNCaP and VCaP, showed significant centrosome loss compared with RWPE1 cells (Fig. 2e, f, j). Similar loss of centrosomes in LNCaP cells was previously reported [35]. In contrast, castration-resistant DU145 and PC3 cells, and neuroendocrine H660 cells, displayed centrosome amplification (Fig. 2g–j), as previously described [35, 36]. Thus, centrosome numbers during tumor progression may be dynamic. While a majority of primary prostate PCa in situ show centrosome loss, centrosome amplification appears in more clinically-aggressive variants of hormone-resistant metastatic cancer.
Centrosome loss in prostate epithelial cells results in mitotic errors, chromosome fragmentation, and micronuclei
We next sought to determine whether the centrosome loss in localized PCa could account for the abundant genomic alterations reported [5]. To test this, we used two immortalized prostate epithelial cell lines, RWPE1 and PrEC; both have been used as stable, benign in vitro models [37,38,39,40,41] and contain normal centrosome numbers (Fig. 2j). We first induced centrosome loss chemically by treating cells with centrinone, a Polo-like kinase 4 (Plk4) inhibitor [28]. Plk4 is the master regulator of centriole duplication [42, 43], and its inhibition causes progressive centrosome depletion in proliferating cell cultures [28]. Over 90% of cells contained either one or zero centrosomes after a 10-day treatment but reassembled centrosomes within 2 days after centrinone removal (Fig. 3a). As a control for off-targeting effects, we generated a centrinone-resistant RWPE1 line, designated RWPE1-Plk4 (G95L), by substituting Leu for Gly95 (G95L) within the endogenous Plk4 gene using CRISPR/Cas9 [28]. Centrinone had no effect on centrosome number in RWPE1-Plk4 (G95L) cells after 10 days of drug treatment (Fig. 3b).
We next determined how centrosome loss affected mitosis in prostate epithelial cells using cells stably expressing histone H2B–GFP and centriole marker CETN1-tdTomato. After a 10-day mock or centrinone treatment, we identified live cells with and without centrosomes (based on the CETN1 signal) and imaged chromosomes as cells progressed through mitosis by time-lapse microscopy (Fig. 3c and Supplementary Videos 1, 2). Whereas mock and DMSO-treated cells spent ~102 min in mitosis (defined here as nuclear envelope breakdown to telophase) (Fig. 3d, Supplementary Videos 3, 4), centrinone-treated cells lacking centrosomes spent 3–4 times longer in mitosis (Fig. 3d, Fig. S2a, Supplementary Videos 5, 6). Consequently, the mitotic index of centrosome-less cells increased fivefold but remained similar to control frequencies when centrinone was applied to RWPE1-Plk4 (G95L) cells (Fig. S2b), demonstrating that the rise in mitotic index was due to Plk4 inactivation.
In centrinone-treated RWPE1 and PrEC cells, chromosomes clustered on disorganized spindles during a prolonged prometaphase (Fig. 3e, f, Supplementary Video 7), but eventually separated into two chromosome masses (Fig. 3c, Supplementary Videos 5–8). Lagging chromatids were present during anaphase (Fig. 3c, red arrowheads, Supplementary Videos 5, 6), which have been shown to form from abnormal merotelic kinetochore attachments in acentrosomal vertebrate spindles [30, 44]. Strikingly, we detected several small chromosomes surrounding the central chromosome mass(es) (Fig. 3c, e) and that were inefficiently captured by spindles (Fig. 3f, yellow arrowheads). Immunostaining for the centromere protein CENP-C revealed these errant chromosomes lacked centromeres and, thus, are chromosome fragments (Fig. 3f, Supplementary Video 7). Missegregated chromosome fragments were enveloped into micronuclei during mitotic exit, causing an increase of micronuclei frequency that was not seen in RWPE1-Plk4 (G95L) cells (Fig. 3g and Fig. S2c). Cytokinesis failure was also frequent (30%; 20 of 66 cells) in centrinone-treated cells (Fig. 3c, RWPE1), and continuous imaging revealed that 80% of these cells died soon after entering G1-phase. As an alternative to centrinone, we generated two Plk4- null clonal lines using CRISPR (Plk4KO-1 and Plk4KO-2) (Fig. S2d, e); immunostaining for CEP135 and γ-Tubulin confirmed that both clones lacked centrosomes. Both Plk4KO-1 and KO-2 clones showed a significant increase in the frequency of micronuclei (Fig. 3g). Notably, 61% of micronuclei in centrinone-treated RWPE1 cells lacked CENP-C (Fig. 3h), suggesting that most micronuclei formed from chromosome fragments.
Lastly, we examined whether centrosome loss also generates micronuclei in 3-dimensional cultured spheroids that approximate normal prostate glands [45]. Similar to 2D cultures, centrinone-treatment produced spheroids with numerous micronuclei (Fig. 3i, arrowheads). Taken together, our findings suggest that centrosome loss in cultured prostate epithelial cells induces phenotypes known to promote CIN.
Centrosome loss produces abnormal nuclear envelopes and increased multinucleate cells in PCa tissue
We next imaged chromosomes of cultured cells exiting mitosis by time-lapse microscopy. Interestingly, we observed mitotic cells that formed multinucleated daughter cells as well as abnormally-shaped, multilobed nuclei in spite of having no apparent defects in anaphase chromosome segregation or cytokinesis (Fig. 4a, Supplementary Videos 9, 10).
Since cells of early PCa contain nuclei with morphological defects [9], we analyzed whether centrosome loss results in defects in nuclear morphology by immunostaining cells for nuclear lamina proteins, Lamin A/C or Emerin. Plk4KO PrEC cells or centrinone-treated wild-type PrEC (or RWPE1) cells displayed a significant 3–9-fold increase in multinucleation frequency compared with control cells (Fig. 4b–d). Nuclear envelopes in acentrosomal cells frequently displayed invaginations (Fig. 4b, arrowheads), irregularities commonly seen in cancer cells [46].
Next, we examined whether similar nuclear defects were present in localized human PCa tissue by immunostaining for Lamin A/C or Emerin (Fig. 4e). Compared with cells from normal prostate glands, Gleason grade 3 PCa showed a higher average frequency of multinucleated cells but this was not significantly different (Fig. 4f). Gleason grade 4 PCa had an almost fourfold increase of multinucleated cells (Figs. 4e, 1 and 2, and f) and micronuclei were detected (Figs. 4e, 2′ arrowhead). Costaining for CEP135 and DNA revealed that ~70% of multinucleated cells displayed complete centrosome loss (Fig. 4g, h). Taken together, our findings suggest that centrosome loss promotes multinucleation and defects in nuclear envelope morphology in cultured cells, and these defects are also present in higher grade PCa. Although it is unclear how these defects arose, it is noteworthy that normal nuclear envelope shape and the efficiency of nuclear reformation rely on the suppression of microtubule growth near chromatin, which happens to be the primary site of microtubule assembly in mitotic cells lacking centrosomes [25, 47].
Centrosome loss results in aneuploidy and chromosomal rearrangements
Localized PCa displays numerical and structural CIN [48]. Since centrosome loss in dividing prostate epithelial cells promotes mitotic errors, we evaluated if centrosome loss could induce aneuploidy by measuring chromosome numbers from chromosome spreads of mitotic RWPE1 cells (Fig. 5a, b). Whereas mock and DMSO-treated cells had a near diploid average chromosome number (mock cells: average = 50; DMSO cells: 48) as previously reported [38], centrinone treatment induced aneuploidy, significantly increasing the average chromosome number to 69 (Fig. 5b). Chromosome fragments were also detected (Fig. 5a, arrowheads), consistent with our live-cell imaging data and the chromosome fragmentation reported in cells with micronuclei [20]. Flow cytometry confirmed that centrinone induced aneuploidy, displaying a sixfold increase in the >4N population (Fig. 5c). DNA profiles of RWPE1-Plk4 (G95L) cells (with or without centrinone) remained similar to DMSO-control cells (Fig. 5c), suggesting that changes in chromosome number were due to centrosome loss.
Using spectral karyotyping (SKY), we next examined which specific chromosomes exceeded diploidy in aneuploid, acentrosomal RWPE1 cells. Cells without centrosomes have altered chromosome copy numbers (gains and losses) compared with control cells, but primarily showed gains not specific to any particular chromosome (Fig. 5d–g). Cells that were stimulated to grow (with FBS) and centrinone-treated to deplete their centrosomes had a sharply increased chromosome number compared with FBS-mock treated cells whose karyotype was consistent with a previous report (Fig. 5e) [38]. The frequency of near tetraploid karyotypes (>80 chromosomes) also increased by 30% after centrinone treatment, suggesting that cytokinesis failure likely contributed to some karyotypes. Furthermore, both RWPE1 cells and PrEC cells showed chromosomal structural rearrangements after centrinone treatment (Fig. S3a, b). Thus, instead of specific mutations, centrosome loss appears to generate gross genomic abnormalities.
Centrosome loss can stimulate malignant xenograft tumor formation
Our findings suggest that centrosome loss is a relatively early occurrence in localized PCa, producing CIN. We next determined if centrosome depleted nontumorigenic prostate cells could generate xenograft tumors. PrEC-Plk4KO clones (clones which proliferate while chronically acentrosomal) were injected subcutaneously into male immunodeficient NSG mice and examined for tumor formation weekly for ~16 weeks. Parental PrEC cells did not form tumors (Fig. 6a), consistent with a previous study [37]. Tumors were not detected by palpation of live mice injected with the PrEC-Plk4KO-1 or two cell lines. However, after these mice were sacrificed on day 112, tumors were found at 25% of the Plk4KO injection sites (Fig. 6a). The tumors were poorly differentiated and malignant as determined by histological examination. Indeed, tumors from both clones invaded into the surrounding adipose and muscle tissue (Fig. 6b). Notably, these tumors contained mitotic figures (Fig. 6c, red arrowhead), enlarged nuclei (green arrowhead), and multinucleated cells (yellow arrowheads), suggesting that tumor cells experience CIN and had histological characteristics of aggressive cancer.
Although centrosome depletion was sufficient to generate tumors, Plk4KO cells likely experience a continuous, high rate of CIN due to their acentrosomal state, which may explain the slow growth and hence small size of these tumors. To test this, we used an alternative to chronic centrosome absence by transiently depleting centrosomes with centrinone for several days, thereby potentially inducing a burst of CIN in the parental PrEC line. After removal of the drug, centrosomes reappeared within the cell population, with the expectation that the potentially altered genomes would then be relatively stably maintained and passed to progeny cells (outlined in Fig. 6d). Accordingly, PrEC cells were treated with centrinone for 15 days (>90% of cells contained one or zero centrioles by day 10; Fig. 3a), followed by monoclonal expansion in normal culture media without centrinone. Using this approach, three of the ten generated clones (CTN-1, 6, and 9) displayed elevated MYC and ERG levels compared with the original PrEC cells (Fig. S4a, b). We selected these three lines for xenograft testing because elevated levels of MYC and ERG correlate with PCa progression [49, 50]. CTN clones were genomically verified to be derived from PrEC using a STR profile. All CTN clones reestablished normal centrosome numbers after removal of the drug, similar to parental PrEC cells (Fig. S4c). Importantly, although the three CTN clones had normal centrosome numbers, they continued to display hallmarks of CIN and showed a significant, elevated frequency of micronuclei (Fig. S4d). All three strains inherited CIN from centrinone treatment, displaying dramatic deviations in chromosome number compared to the parental line; CTN-1 and CTN-6 showed chromosome loss, while CTN-9 had chromosome gain (Fig. S4e). Chromosomal rearrangements were also observed in CTN-9 by SKY analysis (Fig. S3b and S5a, b).
Next, the CTN clones were subcutaneously injected into male immunodeficient NSG mice to evaluate their tumorigenicity. As observed with the parental line, mice injected with CTN-1 did not form tumors (0 of 12) (Fig. 6e, f). Strikingly however, two CTN clones (CTN-6, 3 of 12; CTN-9, 9 of 12) formed large, visible tumors at the injection sites; the CTN-9 tumors developed much sooner than CTN-6 (80 days vs. ~100 days, respectively) (Fig. 6e, f). Histological examination of all tumors revealed that they were similar regardless of the specific injected clone, forming highly proliferative malignant tumors with poorly differentiated epithelial glands (Fig. 6g). Similar to PrEC-Plk4KO clones, both CTN clones formed tumors that invaded the surrounding smooth muscle and adipose tissue (Fig. 6h, arrowheads). Thus, transient centrosome elimination can transform cells, enabling them to form malignant tumors.
We further characterized the CTN tumors by immunostaining tissue sections with a panel of epithelial, mesenchymal, and secretory markers (Fig. S5c, d). CTN tumors maintained epithelial proteins including CD49f and CD44 but were negative for E-cadherin, CK5/14, CK8/18, CK14-16, 19, as well as luminal (FOXA1), neuroendocrine (synaptophysin), and mesenchymal (vimentin, desmin) markers (Fig. S5c, d). Tumors were highly secretory and stained positive for mucin and hyaluronic acid (HA) (Fig. S5c, d), a feature of poorly differentiated malignant PCa [51].
Lastly, we measured centrosome numbers within all 12 tumors using our in situ centrosome-counting assay. As in PCa tissue, we identified individual cells that clearly contained CEP135-labeled centrosomes (Fig. 6i). Dividing cells were also observed and formed mitotic spindles regardless of their centrosome status (Fig. 6j). Surprisingly, many tumor cells displayed centrosome loss, in some CTN-9 tumors, the percentage of cells with zero centrosomes exceeded 70% (Fig. 6k). Thus, transient removal of centrosomes was sufficient to induce tumor formation in a subset of immortalized prostate epithelial PrEC cells. During tumorigenesis, centrosomes were lost in a large population of cells resident at the initial injection site, resembling the phenomenon we observed in primary prostate carcinoma.
Discussion
In lieu of signature driver mutations that distinguish many cancers, genomic instability itself may provide the primary oncogenic force behind prostate tumorigenesis. Localized PCa show widespread genomic rearrangements, including chromothripsis (20% of tumors) [5]. Moreover, genomic alterations occur in a few successive bursts, likely initiated by a genomic crisis, leading to a proposed punctuated-progression model of prostate tumor evolution [1, 11]. Extensive studies have been performed to understand the complexity of genomic instability in prostate tumors and our findings point to centrosome loss as a potential origin of genomic crisis.
Centrosome loss is prevalent in localized primary prostate carcinoma, becoming more pronounced in higher Gleason grade tumors. Centrosome loss also promotes aneuploidy, chromosome fragmentation, micronuclei, and other forms of CIN. Thus, centrosome loss, in principle, may account for the wide range of genomic hallmarks assigned to localized PCa. Transient centrosome loss produced much larger solid tumors, suggesting that bursts of genomic crisis may be more suitable for sustained proliferation. Centrosome amplification has been recognized by many as a cancer hallmark with the capacity to promote oncogenesis [15]. It is surprising that the opposite situation, the absence of centrosomes in proliferating tumor cells, has not been described before in human cancer. Similar to multicentrosomal/multipolar spindles, acentrosomal spindles display errors in positioning chromosomes and high rates of CIN [30]. We observed that centrosome depletion in human epithelial prostate cells is transformative, enabling the previously nontumorigenic cells to form malignant tumors in mice. Future studies should determine whether centrosome loss is a phenomenon restricted to PCa.
If centrosome loss is a driver of genomic instability in early prostate tumors, what then causes this organelle to disappear? In general, little is known about the mechanisms of centrosome elimination. However, centrosomes are normally inactivated or lost during specific developmental stages in different animals [52]. For example, in the Drosophila female germline, centrioles disassemble when PCM is downregulated; this mechanism contributes to centriole elimination in the oocyte [53]. In contrast, pericentrin, a PCM component, accumulates in prostate carcinoma [54], suggesting that changes in PCM levels may not be a mechanism underlying centrosome disappearance in primary prostate tumors. Centrosome loss may be due to other factors such as age, inflammation, hypoxia, other environmental influences, or a combination of events. Determining the root cause of centrosome disappearance will be an important line of investigation. Indeed, an unidentified environmental factor(s) might be responsible for the loss of centrosomes from the xenograft tumors that arose from injections of cells that had been transiently centrosome depleted but contained a normal centrosome number at the time of injection.
Although centrosome loss occurs in primary prostate tumors, TNBC displays centrosome amplification [34], as do metastatic-derived androgen unresponsive PCa cell lines and neuroendocrine H660 PCa cells. Possibly, centrosome numbers fluctuate during prostate tumor evolution. Indeed, centrosome loss may be an early ‘driver’ event and, through further genomic instability, gives rise to cells with genotypes that trigger centrosome amplification, paving the way to malignancy. Notably, centrosome amplification promotes an invasive cellular behavior [55, 56]. Additional studies will be needed to determine when centrosome loss occurs in PCa. Moreover, we found a possible relationship between centrosome duplication and hormone receptor status. Specifically, clinically-aggressive variants of hormone-resistant metastatic cancer show centrosome amplification, raising the possibility that androgen receptor signaling might regulate centrosome duplication, which should be explored. For PCa, this is significant because loss of androgen signaling and gain of neuorendrocine features are indicative of increased lethality. In addition, changes in centrosome number could be used as a predictive biomarker for aggressive (high risk) disease and patient survival if it were established that centrosome numbers vary in tumors of different malignancies, particular those that are metastatic and recurrent.
Materials and methods
Cell culture
RWPE1 (ATCC #CRL- 11609TM), PEC, and iPEC37 (C. Miranti, University of Arizona) cells were grown in Keratinocyte Serum Free Medium (K-SFM; ThermoFisher) with 0.05 mg/ml BPE, 5 ng/ml EGF, and penicillin/streptomycin/amphotericin (5% CO2 at 37 °C). PEC was derived from prostatectomy specimens and verified to be free of stromal contamination [57, 58]. Immortalized human PrEC cells (W. Hahn, MIT) [37] were cultured in Iscove’s Modified Dulbecco’s Medium (IMDM; ThermoFisher) with 10% FBS. iPEC37 are PEC cells immortalized with HPV E6/E7 and hTERT [37]. LNCaP (ATCC C#RL-1740), VCaP (ATCC #CRL-2876), and PC3 (ATCC #CRL-1435) were cultured in RPMI 1640 (ThermoFisher) with 10% FBS, DU145 (ATCC #HTB-81) in IMDM, and NCI-H660 (ATCC #CRL-5813) in RPMI-1640 media (supplemented with 0.005 mg/ml insulin, 0.01 mg/ml transferrin, 30 nM sodium selenite, 10 nM hydrocortisone, 10 nM beta-estradiol, 2 mM L-glutamine, and 5% FBS. Cell identities were verified using genomic probes [59]. For RWPE1 cultured in KSFM, centrinone was used at 100 nM, but 300 nM for all cells cultured in FBS. Cells were serum starved for 48 h before addition of 100 nM DHT.
Stable lines and CRISPR/Cas9
Lentiviral plasmid (pLenti6) and packaging vectors (pMD2.G/psPAX2; Addgene #12259 and 12260) were used to generate H2B-GFP stable expressing cells. Virus was harvested from HEK-293 cells at 24–48 h post transfection, filtered, and added to media with 8 μg/ml polybrene. Stable lines were selected with 500 ng/ml puromycin after 2 weeks. RWPE1 lines were then transduced with centrin1/CETN1)-tdTomato lentivirus (pLentiLox CMV; V. Bautch, University of North Carolina). The Alt-R CRISPR/Cas9 system (IDT) with Plk4 gRNA (GGAAGCTGAGTGTTAAGTTC) was used to generate Plk4(G95L) [57]. The RNP complex of Plk4-crRNA, CRISPR-Cas9 tracrRNA (IDT #1072532), and Cas9 were transfected into cells using a Nucleofector 2b (Amaxa). Repair template plasmid (pY181) (K. Oegema, University of California San Diego) and packaging plasmids (pHelper/pAAV-RC) were transfected into HEK293T cells using Lipofectamine300. Virus was harvested 48 h post transfection, filtered, and added to media for 16 h. Cells were selected in 96-well plates for 2 weeks in 0.5 mg/ml G418, and homozygous G95L knockin clones were identified by PCR and sequencing of genomic DNA. UACC Genome Editing Facility generated Plk4 homozygous knockout PrEC cells. Double-strand break sites flanking the Plk4 transcriptional unit (4:127,879,990 and 4:127,909,266) were targeted with guide sequences 5-AACTACGGAATAAGCGGTAG-3 and 3-TCTCGCCAACTTAATTAAGG-5. Cells were transfected with Cas9, crRNAs, and tracrRNA using Lipofectamine. Two days post transfection, cutting efficiency was estimated using a T7 endonuclease assay employing PCR primers flanking the predicted ligation-junction product. Single cells were deposited in 96-well plates using the UACC Flow Cytometry Shared Resource and colonies were screened by PCR. Clones that were negative for two fragments internal to the targeted deletion but positive for ligation-junction fragment were potentially homozygous for the deletion. Absence of Plk4 RNA was confirmed by rt-PCR.
Microscopy
For IF, cells were cultured on coverslips, washed in PBS, and fixed in ice-cold methanol for 10 mins. After a 5 min rehydration in PBS, cells were washed in Buffer-A (PBS, 0.5% Triton X-100) for 5 min, blocking Buffer-B (PBS, 5% NGS, 0.1% Triton X-100) for 30 min, and incubated with primary antibodies in Buffer-B for 1 h at room temperature. Next, cells were washed 3 times in Buffer-A, incubated with secondary antibodies and Hoechst33342 for 1 h at room temperature, washed 3 times in Buffer-A (5 min), and mounted in 0.1 M n-propyl gallate, PBS, 90% (by volume) glycerol. For centromere immunostaining, cells were rinsed in PHEM (60 mM PIPES, 25 mM HEPES, 10 mM EGTA, 4 mM MgSO4·7H20), permeabilized with 0.5% Triton X-100 in PHEM for 4 min, and fixed with 4% paraformaldehyde in PHEM for 20 min at room temperature.
For metaphase spreads, cells were treated with 0.06 μg/ml colcemid overnight, trypsinized, resuspended in Buffer-M (40 mM KCl, 20 mM HEPES, 0.5 mM EGTA, and 9 mM NaOH), and incubated for 50 min at 37 °C. Next, cells were fixed in methanol:acetic acid (3:1), pelleted, and washed in fixative before dropped onto a precleaned coverglass. Cells were dried on slides for 3 days and stained with Hoechst33342. SKY analysis was performed by the Roswell Park Cancer Institute Cytogenetics SKY Core Laboratory. Formalin-fixed deidentified human cancer tissues were processed for detection of centrosomes using our published procedure [31]. Specimens were imaged using a DeltaVision Core equipped with an Olympus IX71 microscope, ×60 objective (1.42NA), and a cooled charge-coupled CoolSNAP-HQ2 camera. For time-lapse microscopy, cells were grown in 8-well Lab-Tek chambered coverglass coated with anti-β1 integrin/AIIB2 antibody to inhibit cell migration; images were acquired every 5 min with 4 μm z-section thickness for 24 h. Images acquired with SoftWoRx v1.2.
Antibodies/stains used include: anti-CEP135 (cells-1:500; tissue-1:100; Abcam ab75005), anti-γ-tubulin (cells-1:500; tissue-1:100; Sigma Aldrich GTU-88), anti-E-Cadherin/M168 (1:100; Abcam ab76055), anti-Centrin-3/3E6 (1:500; Abnova H00001070-M01), anti-phospho-Histone H3 (1:1000; Cell Signaling Technology #9706 S), 7-AAD Staining Solution (1:50; BioLegend #420404), Alexa Fluor™ 647 Phalloidin (1:40; ThermoFisher A22287), anti-α-tubulin (1:1500; Sigma Aldrich DM1A), anti-CENP-C (1:1000; MBL International PD030), anti-LaminA/C (1:100; Santa Cruz Biotechnology sc-6215), anti-Emerin (1:100; Sigma-Aldrich HPA000609), anti-β1 integrin (1:1000, DSHB AIIB2), anti-α6 integrin/CD49f (1:100; produced in our lab), anti-CD44 (1:100; ThermoFisher #156-3C11), anti-N-Cadherin (1:100; Santa Cruz Biotechnology sc-8424), anti-CK5/14 (1:100; produced in our lab), anti-CK18 (1:100; Abcam EPR1626), anti-Vimentin (1:100; Cell Signaling Technology D21H3), anti-Desmin (1:100; Atlas Antibodies HPA018803), Hyaluronic Acid-Binding Protein (1:100; Sigma-Aldrich #385911), anti-cMyc (1:50-100; Cell Signaling Technology D3N8F), anti-FOXA1(1:100; Abcam EPR10881), anti-Synaptophysin (1:100; Sigma-Aldrich MRQ-40), anti-laminin-332 (1:200; Abcam ab14509), anti-ITGB4 (1:100; Abcam ab110167), and anti-p63 (1:100; biobyt orb214808). Secondary antibodies (Jackson Immunoresearch) were used at 1:1500.
Animal studies
Mouse experiments were conducted with animal care and committee approval using the Experimental Mouse Shared Service. A total of 10 × 106 prostate epithelial cells were mixed with an equal number of nontumorigenic fibroblasts (WPMY-1) in 0.1 ml growth factor reduced matrigel and injected subcutaneously into male NOD/SCID/IL2Rγnull (NSG) mice (Jackson Laboratories); three mice per treatment group. Tumor growth was measured 2 times/week and tumor volume estimated according to the formula: [(width)2 × length]/2. Animals were terminated by CO2 when total tumor reached 2000 mm3.
Statistical analysis
The statistical significance of differences in average measurements was evaluated using unpaired t-tests (GraphPad Prism 6.0). Means are significantly different if P < 0.05. In figures, “*” indicates 0.05 > P ≥ 0.01; **0.01 > P ≥ 0.001; ***0.001 > P ≥ 0.0001; ****0.0001 > P, and not significant “ns” indicates P ≥ 0.05 for indicated pairwise comparisons. Error bars in all figures indicate standard deviation (SD).
References
Baca SC, Prandi D, Lawrence MS, Mosquera JM, Romanel A, Drier Y, et al. Punctuated evolution of prostate cancer genomes. Cell. 2013;153:666–77.
Boutros PC, Fraser M, Harding NJ, de Borja R, Trudel D, Lalonde E, et al. Spatial genomic heterogeneity within localized, multifocal prostate cancer. Nat Genet. 2015;47:736–45.
Armenia J, Wankowicz SAM, Liu D, Gao J, Kundra R, Reznik E, et al. The long tail of oncogenic drivers in prostate cancer. Nat Genet. 2008;50:645–51.
Barbieri CE, Baca SC, Lawrence MS, Demichelis F, Blattner M, Theurillat JP, et al. Exome sequencing identifies recurrent SPOP, FOXA1 and MED12 mutations in prostate cancer. Nat Genet. 2012;44:685–9.
Fraser M, Sabelnykova VY, Yamaguchi TN, Heisler LE, Livingstone J, Huang V, et al. Genomic hallmarks of localized, non-indolent prostate cancer. Nature. 2017;541:359–64.
Robinson DR, Wu YM, Lonigro RJ, Vats P, Cobain E, Everett J, et al. Integrative clinical genomics of metastatic cancer. Nature. 2017;548:297–330.
Wu YM, Cieslik M, Lonigro RJ, Vats P, Reimers MA, Cao X. et al. Inactivation of CDK12 delineates a distinct immunogenic class of advanced prostate cancer. Cell. 2018;173:1770–82.
Cancer Genome Atlas Research Network. The molecular taxonomy of primary prostate cancer. Cell. 2015;163:1011–25.
Petein M, Michel P, van Velthoven R, Pasteels JL, Brawer MK, Davis JR, et al. Morphonuclear relationship between prostatic intraepithelial neoplasia and cancers as assessed by digital cell image analysis. Am J Clin Pathol. 1991;96:628–34.
Tomlins SA, Rhodes DR, Perner S, Dhanasekaran SM, Mehra R, Sun XW, et al. Recurrent fusion of TMPRSS2 and ETS transcription factor genes in prostate cancer. Science. 2005;310:644–8.
Espiritu SMG, Liu LY, Rubanova Y, Bhandari V, Holgersen EM, Szyca LM. et al. The evolutionary landscape of localized prostate cancers drives clinical aggression. Cell. 2018;173:1003–13.
Conduit PT, Wainman A, Raff JW. Centrosome function and assembly in animal cells. Nat Rev Mol Cell Biol. 2015;16:611–24.
Bettencourt-Dias M, Glover DM. Centrosome biogenesis and function: centrosomics brings new understanding. Nat Rev Mol Cell Biol. 2007;8:451–63.
Lawo S, Hasegan M, Gupta GD, Pelletier L. Subdiffraction imaging of centrosomes reveals higher-order organizational features of pericentriolar material. Nat Cell Biol. 2012;14:1148–58.
Nigg EA, Holland AJ. Once and only once: mechanisms of centriole duplication and their deregulation in disease. Nat Rev Mol Cell Biol. 2018;19:297–312.
Godinho SA, Pellman D. Causes and consequences of centrosome abnormalities in cancer. Philos Trans R Soc Lond B Biol Sci. 2014;369 pii: 20130467. https://doi.org/10.1098/rstb.2013.0467.
Chan JY. A clinical overview of centrosome amplification in human cancers. Int J Biol Sci. 2011;7:1122–44.
Ganem NJ, Godinho SA, Pellman D. A mechanism linking extra centrosomes to chromosomal instability. Nature. 2009;460:278–82.
Silkworth WT, Nardi IK, Scholl LM, Cimini D. Multipolar spindle pole coalescence is a major source of kinetochore mis-attachment and chromosome mis-segregation in cancer cells. PLoS ONE. 2009;4:e6564.
Crasta K, Ganem NJ, Dagher R, Lantermann AB, Ivanova EV, Pan Y, et al. DNA breaks and chromosome pulverization from errors in mitosis. Nature. 2012;482:53–8.
Coelho PA, Bury L, Shahbazi MN, Liakath-Ali K, Tate PH, Wormald S, et al. Over-expression of Plk4 induces centrosome amplification, loss of primary cilia and associated tissue hyperplasia in the mouse. Open Biol. 2015;5:150209.
Levine MS, Bakker B, Boeckx B, Moyett J, Lu J, Vitre B, et al. Centrosome amplification Is sufficient to promote spontaneous tumorigenesis in mammals. Dev Cell. 2017;40:313–22.
Sercin O, Larsimont JC, Karambelas AE, Marthiens V, Moers V, Boeckx B, et al. Transient PLK4 overexpression accelerates tumorigenesis in p53-deficient epidermis. Nat Cell Biol. 2016;18:100–10.
Vitre B, Holland AJ, Kulukian A, Shoshani O, Hirai M, Wang Y, et al. Chronic centrosome amplification without tumorigenesis. Proc Natl Acad Sci USA. 2015;112:E6321–30.
Meunier S, Vernos I. Acentrosomal microtubule assembly in mitosis: the where, when, and how. Trends Cell Biol. 2016;26:80–7.
Bazzi H, Anderson KV. Acentriolar mitosis activates a p53-dependent apoptosis pathway in the mouse embryo. Proc Natl Acad Sci USA. 2014;111:E1491–500.
Lambrus BG, Uetake Y, Clutario KM, Daggubati V, Snyder M, Sluder G, et al. p53 protects against genome instability following centriole duplication failure. J Cell Biol. 2015;210:63–77.
Wong YL, Anzola JV, Davis RL, Yoon M, Motamedi A, Kroll A, et al. Cell biology. Reversible centriole depletion with an inhibitor of Polo-like kinase 4. Science. 2015;348:1155–60.
Khodjakov A, Rieder CL. Centrosomes enhance the fidelity of cytokinesis in vertebrates and are required for cell cycle progression. J Cell Biol. 2001;153:237–42.
Sir JH, Putz M, Daly O, Morrison CG, Dunning M, Kilmartin JV, et al. Loss of centrioles causes chromosomal instability in vertebrate somatic cells. J Cell Biol. 2013;203:747–56.
Wang, M, Knudsen, BS, Nagle RB, Rogers GC, Cress AE. A method to quantify centrosomes at single-cell level in human normal and cancer tissue. Mol Biol Cell. 2019. https://doi.org/10.1091/mcb.E18-10-0651.
Rubin MA, Mucci NR, Figurski J, Fecko A, Pienta KJ, Day ML. E-cadherin expression in prostate cancer: a broad survey using high-density tissue microarray technology. Hum Pathol. 2001;32:690–7.
Denu RA, Zasadil LM, Kanugh C, Laffin J, Weaver BA, Burkard ME. Centrosome amplification induces high grade features and is prognostic of worse outcomes in breast cancer. BMC Cancer. 2016;16:47.
Chatterjee SJ, McCaffrey L. Emerging role of cell polarity proteins in breast cancer progression and metastasis. Breast Cancer. 2014;6:15–27.
Ouyang X, Wang X, Xu K, Jin DY, Cheung AL, Tsao SW, et al. Effect of p53 on centrosome amplification in prostate cancer cells. Biochim Biophys Acta. 2001;1541:212–20.
Cosenza MR, Cazzola A, Rossberg A, Schieber NL, Konotop G, Bausch E. et al. Asymmetric centriole numbers at spindle poles cause chromosome missegregation in cancer. Cell Rep. 2017;20:1906–20.
Berger R, Febbo PG, Majumder PK, Zhao JJ, Mukherjee S, Signoretti S, et al. Androgen-induced differentiation and tumorigenicity of human prostate epithelial cells. Cancer Res. 2004;64:8867–75.
Bello D, Webber MM, Kleinman HK, Wartinger DD, Rhim JS. Androgen responsive adult human prostatic epithelial cell lines immortalized by human papillomavirus 18. Carcinogenesis. 1997;18:1215–23.
Cangemi R, Mensah A, Albertini V, Jain A, Mello-Grand M, Chiorino G, et al. Reduced expression and tumor suppressor function of the ETS transcription factor ESE-3 in prostate cancer. Oncogene. 2008;27:2877–85.
Rickman DS, Soong TD, Moss B, Mosquera JM, Dlabal J, Terry S, et al. Oncogene-mediated alterations in chromatin conformation. Proc Natl Acad Sci USA. 2012;109:9083–8.
Shi Q, King RW. Chromosome nondisjunction yields tetraploid rather than aneuploid cells in human cell lines. Nature. 2005;437:1038–42.
Bettencourt-Dias M, Rodrigues-Martins A, Carpenter L, Riparbelli M, Lehmann L, Gatt MK, et al. SAK/PLK4 is required for centriole duplication and flagella development. Curr Biol. 2005;15:2199–207.
Habedanck R, Stierhof YD, Wilkinson CJ, Nigg EA. The Polo kinase Plk4 functions in centriole duplication. Nat Cell Biol. 2005;7:1140–6.
Gregan J, Polakova S, Zhang L, Tolic-Norrelykke IM, Cimini D. Merotelic kinetochore attachment: causes and effects. Trends Cell Biol. 2011;21:374–81.
Wang M, Nagle RB, Knudsen BS, Rogers GC, Cress AE. A basal cell defect promotes budding of prostatic intraepithelial neoplasia. J Cell Sci. 2017;130:104–10.
Malhas AN, Vaux DJ. Nuclear envelope invaginations and cancer. Adv Exp Med Biol. 2014;773:523–35.
Xue JZ, Woo EM, Postow BT, Chait H, Funabiki H. Chromatin-bound Xenopus Dppa2 shapes the nucleus by locally inhibiting microtubule assembly. Dev Cell. 2013;27:47–59.
Beheshti B, Park PC, Sweet JM, Trachtenberg J, Jewett MA, Squire JA. Evidence of chromosomal instability in prostate cancer determined by spectral karyotyping (SKY) and interphase fish analysis. Neoplasia. 2001;3:62–9.
Sun C, Dobi A, Mohamed A, Li H, Thangapazham RL, Furusato B, et al. TMPRSS2-ERG fusion, a common genomic alteration in prostate cancer activates C-MYC and abrogates prostate epithelial differentiation. Oncogene. 2008;27:5348–53.
Zeng W, Sun H, Meng F, Liu Z, Xiong J, Zhou S, et al. Nuclear C-MYC expression level is associated with disease progression and potentially predictive of two year overall survival in prostate cancer. Int J Clin Exp Pathol. 2015;8:1878–88.
Lipponen P, Aaltomaa S, Tammi R, Tammi M, Agren U, Kosma VM. High stromal hyaluronan level is associated with poor differentiation and metastasis in prostate cancer. Eur J Cancer. 2001;37:849–56.
Werner S, Pimenta-Marques A, Bettencourt-Dias M. Maintaining centrosomes and cilia. J Cell Sci. 2017;130:3789–3800.
Pimenta-Marques A, Bento I, Lopes CA, Duarte P, Jana SC, Bettencourt-Dias M. A mechanism for the elimination of the female gamete centrosome in Drosophila melanogaster. Science. 2016;353:aaf4866.
Pihan GA, Purohit A, Wallace J, Malhotra R, Liotta L, Doxsey SJ. Centrosome defects can account for cellular and genetic changes that characterize prostate cancer progression. Cancer Res. 2001;61:2212–9.
Godinho SA, Picone R, Burute M, Dagher R, Su Y, Leung CT, et al. Oncogene-like induction of cellular invasion from centrosome amplification. Nature. 2014;510:167–71.
Kushner EJ, Ferro LS, Liu JY, Durrant JR, Rogers SL, Dudley AC, et al. Excess centrosomes disrupt endothelial cell migration via centrosome scattering. J Cell Biol. 2014;206:257–72.
Edick MJ, Tesfay L, Lamb LE, Knudsen BS, Miranti CK. Inhibition of integrin-mediated crosstalk with epidermal growth factor receptor/Erk or Src signaling pathways in autophagic prostate epithelial cells induces caspase-independent death. Mol Biol Cell. 2007;18:2481–90.
Gmyrek GA, Walburg M, Webb CP, Yu HM, You X, Vaughan ED, et al. Normal and malignant prostate epithelial cells differ in their response to hepatocyte growth factor/scatter factor. Am J Pathol. 2001;159:579–90.
van Bokhoven A, Varella-Garcia M, Korch C, Hessels D, Miller GJ. Widely used prostate carcinoma cell lines share common origins. Prostate. 2001;47:36–51.
Acknowledgements
We thank K. Oegema for providing centrinone and CRISPR constructs, D. Pellman for histone-H2B construct, V. Bautch for centrin1 construct, W. Hahn for PrEC cells, C. Miranti for iPEC37 cells, and N. Ellis and J. DeLuca for technical advice. Tissue samples were obtained from the PCa Biorepository Network (PCBN) (DoD PCa Research Program Award No W81XWH-14-2-0182, W81XWH-14-2-0183, W81XWH-14-2-0185, W81XWH-14-2-0186, and W81XWH-15-2-0062). This work was supported by NIH grants NCI P30 CA23074, R01GM110166, and R01GM126035 to GCR, R01CA159406 to AEC and Tim and Diane Bowden Cancer Biology Research Fellowship to MW.
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Wang, M., Nagle, R.B., Knudsen, B.S. et al. Centrosome loss results in an unstable genome and malignant prostate tumors. Oncogene 39, 399–413 (2020). https://doi.org/10.1038/s41388-019-0995-z
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DOI: https://doi.org/10.1038/s41388-019-0995-z
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