Functional Evidence that the Self-Renewal Gene NANOG Regulates Human Tumor Development


  • Collene R. Jeter,

    1. Department of Carcinogenesis, University of Texas M.D. Anderson Cancer Center, Science Park-Research Division, Smithville, Texas, USA
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  • Mark Badeaux,

    1. Department of Carcinogenesis, University of Texas M.D. Anderson Cancer Center, Science Park-Research Division, Smithville, Texas, USA
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  • Grace Choy,

    1. Department of Carcinogenesis, University of Texas M.D. Anderson Cancer Center, Science Park-Research Division, Smithville, Texas, USA
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  • Dhyan Chandra,

    1. Department of Carcinogenesis, University of Texas M.D. Anderson Cancer Center, Science Park-Research Division, Smithville, Texas, USA
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  • Lubna Patrawala,

    1. Department of Carcinogenesis, University of Texas M.D. Anderson Cancer Center, Science Park-Research Division, Smithville, Texas, USA
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  • Can Liu,

    1. Department of Carcinogenesis, University of Texas M.D. Anderson Cancer Center, Science Park-Research Division, Smithville, Texas, USA
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  • Tammy Calhoun-Davis,

    1. Department of Carcinogenesis, University of Texas M.D. Anderson Cancer Center, Science Park-Research Division, Smithville, Texas, USA
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  • Holm Zaehres,

    1. Department of Biological Chemistry and Molecular Pharmacology, Harvard Stem Cell Institute and Harvard Medical School, Division of Hematology/Oncology Children's Hospital, Boston, Massachusetts, USA
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  • George Q. Daley,

    1. Department of Biological Chemistry and Molecular Pharmacology, Harvard Stem Cell Institute and Harvard Medical School, Division of Hematology/Oncology Children's Hospital, Boston, Massachusetts, USA
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  • Dean G. Tang

    Corresponding author
    1. Department of Carcinogenesis, University of Texas M.D. Anderson Cancer Center, Science Park-Research Division, Smithville, Texas, USA
    • Department of Carcinogenesis, University of Texas, M.D. Anderson Cancer Center, Science Park-Research Division, Smithville, TX 78957, USA
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    • Telephone: +512-237-9575; Fax: 512-237-2475

  • Author contributions: C.J.: conception and design, collection and assembly of data, data analysis and interpretation, manuscript writing; M.B., G.C., D.C., L.P., C.L., T.C.: collection and assembly of data; H.Z., G.D.: provision of study material; D.T.: conception and design, data analysis and interpretation, manuscript writing, final approval of manuscript.

  • First published online in Stem CellsExpress February 5, 2009


Tumor development has long been known to resemble abnormal embryogenesis. The embryonic stem cell (ESC) self-renewal gene NANOG is purportedly expressed by some epithelial cancer cells but a causal role in tumor development has remained unclear. Here, we provide compelling evidence that cultured cancer cells, as well as xenograft- and human primary prostate cancer cells express a functional variant of NANOG. NANOG mRNA in cancer cells is derived predominantly from a retrogene locus termed NANOGP8. NANOG protein is detectable in the nucleus of cancer cells and is expressed higher in patient prostate tumors than matched benign tissues. NANOGP8 mRNA and/or NANOG protein levels are enriched in putative cancer stem/progenitor cell populations. Importantly, extensive loss-of-function analysis reveals that RNA interference-mediated NANOG knockdown inhibits tumor development, establishing a functional significance for NANOG expression in cancer cells. Nanog short hairpin RNA transduced cancer cells exhibit decreased long-term clonal and clonogenic growth, reduced proliferation and, in some cases, altered differentiation. Thus, our results demonstrate that NANOG, a cell-fate regulatory molecule known to be important for ESC self-renewal, also plays a novel role in tumor development. Stem Cells 2009;27:993–1005


Cancer cells and embryonic stem cells (ESCs) share many key biological properties. A cardinal trait possessed by both cell types is extensive proliferative potential essential for embryogenesis and tumor development. Pluripotency is also fundamental to ESCs and gives rise to the myriad of differentiated daughter cells present in the mature embryo. Similarly, multipotent cancer cells seem to exist that may recapitulate the tumor of origin upon transplantation [1]. Such tumor-initiating cells, often termed cancer stem cells (CSCs), contribute to tumor homeostasis; however, the molecular mechanisms that underlie the perpetual growth and plasticity of CSCs have scarcely been elucidated.

Self-renewal is essential to the maintenance of stem cell (SC) populations, and cancer cells have also been evidenced to renew as demonstrated by secondary (2°) growth assays, including serial tumor transplantation and sphere-formation assays. Remarkably, single-cell derived colon cancer spheres and tumors comprising a mixture of cell lineages have recently been shown to arise from a subset of cancer cells expressing CSC markers [2]. Thus, in principle, the molecular mechanisms that mediate ESC self-renewal may also operate in renewing cancer cells. Transcription factors represent critical molecular switches regulating SC fate. Three transcription factors, Sox2, Oct3/4 (Oct4), and Nanog [3, 4], form a core regulatory network that coordinately determines ESC self-renewal and differentiation [5, 6]. These ESC self-renewal molecules may conceptually also contribute to tumorigenesis. In support, NANOG is expressed not only in germ cell tumors [7] but also reported to be expressed in other tumors including carcinomas of the breast [8, 9], cervix [10], oral cavity [11], kidney [12], and ovary [13]. Also, ectopic expression of OCT4 in transgenic mice is sufficient to induce hyperplasia and dysplasia in the epidermis and intestinal crypt [14] and NANOG overexpression promotes proliferation and transformation of NIH3T3 cells [15].

Cancer cells expressing OCT4 mRNA are frequently implied to mark putative CSCs (e.g., [13, 16]). A potential danger in making such a connection is that OCT4 has multiple copies of processed but nonfunctional pseudogenes [17], which can mimic proper mRNA and generate false-positive real-time polymerase chain reaction (RT-PCR) products [18]. In support, some “OCT4-positive” cancer cell lines were later found to lack credible expression of OCT4 mRNA and protein [19]. Genetic analysis also does not support a significant role for OCT4 in regulating normal mouse somatic SCs [20]. On the other hand, recent loss-of-function studies demonstrate that OCT4 is an important mediator of some cancer cell phenotypes including survival and invasion [21, 22].

Like OCT4, NANOG has also been reported in some nongerm cell tumors (mentioned earlier) and NANOG also possesses multiple pseudogenes (see later). However, comprehensive and systematic studies of NANOG mRNA and NANOG protein expression in human tumor cells are still lacking. More importantly, it remains unclear whether the expression of NANOG in cancer cells plays a causal role in tumor development. In this study, we set out to test the hypothesis that the ESC self-renewal molecule NANOG contributes to cancer cell clonogenic or tumorigenic growth properties. Herein, we provide convincing evidence that tumor cells in vitro and in vivo express a retrotransposed NANOG gene and that NANOG protein is functionally important in regulating human tumor development.


Xenografts, Tumor Dissociation, Flow-Activated Cell Sorting, and Transplantation

Cells, xenografts, and basic experimental procedures for tumor dissociation, flow-activated cell sorting (FACS), in vitro characterization, and subcutaneous (s.c.) transplantation were detailed elsewhere [23–25]. Prostate cancer (PCa) samples were obtained at radical prostatectomy with patients' consent by the IRB-approved guidelines. Minced tumor tissues were subject to enzymatic digestion (type I collagenase, 50 U/ml DNase, 12 hours), followed by trypsin digestion and discontinuous Percoll gradient purification. Primary (1°) HPCa cells were recombined with rat urogenital sinus mesenchyme (rUGSM) in collagen drops and transplanted under the renal capsule as previously described [26] (see supporting information for details).

RT-PCR and Quantitative RT-PCR

Total RNA was extracted from cancer cells or human ESC (hESC; cell line WA09/H9, cultured as previously described [27]) using an RNeasy RNA-purification kit (Qiagen, Valencia, CA, PCR primers are indicated in supporting information Table S1. RT-PCR was performed using an ABI Prism 7900HT and the TaqMan system (ABI; Applied Biosystems, Foster City, CA,, and the NANOG primers and probes previously described [27] (see supporting information).

Cloning and Characterization of Cancer Cell-Derived NANOG

NANOGP8 cDNA was amplified by PCR using LDF1/LDR1 primers and cloned in pCR2.1 (Invitrogen, Carlsbad, CA, Sequencing was performed using the ABI Prism 3130xl Genetic Analyzer. The EcoR I/Sal I fragments containing the NANOG coding sequence were subcloned into pET-28b(+), and His-tagged NANOG proteins were purified from transformed bacteria per manufacturer (Qiagen). Samples were run on 12% SDS-PAGE and proteins were transferred to nitrocellulose membrane and probed as described. Tryptic digests were analyzed using a 4700 Proteomics Analyzer MALDI-TOF/TOF (Applied Biosystems).

Immunofluorescence and Immunohistochemistry Staining

Fluorescence microscopy basic procedures have been described [23–25] (see supporting information; antibodies in Table S2). Immunofluorescence (IF) detection of NANOG required permeabilization and denaturation pretreatment (0.5% TritonX100, 0.25% sodium dodecyl sulfate). For immunohistochemistry (IHC), formalin fixed, paraffin-embedded tissue sections were deparaffinized and hydrated. Endogenous peroxidase activity was blocked (3% H2O2) and antigen retrieval was performed (10 mM citrate buffer; pH 6.0). Slides were incubated with Biocare Blocking Reagent (Biocare, Concord, CA, followed by 1° antibody (1:100, 2 hours) and, either biotinylated 2° antibody and streptavidin-Alexafluor594 (Invitrogen) 3° antibody, or for IHC, horseradish peroxidase rabbit on rodent polymer (Biocare) followed by DAB development.

Lentiviral Production and Transduction

Lentiviruses containing the pLL3.7, LL-Luc, Oct4-short hair pin RNA (shRNA), and Nanog-shRNA [27] or the TRC-shRNA (TRCN000004887) or pGIPZ-Nanog-shRNA vectors (Open Biosystems, Huntsville, AL, were produced in 293FT packaging cells as previously described [27] (see supporting information).

Phenotype “Rescue” Experiments

Nondirectional cloning of NANOGP8 into pPyCAG [3] was performed by ligating the XhoI/SalI fragment of pCR2.1-HPCa5-Nanog into the XhoI site of pPyCAG. Cells were infected with lentivirus 24 hours prior to transfection, replated on coverslips, and subject to the 5-bromo-2-deoxyuridine (BrdU) proliferation assay (see supporting information).


Various Cancer Cells Express NANOGmRNA

To assess the mRNA expression of NANOG, we initially used two pairs of primers: the F1/R1 pair that spans the intron 3 of human NANOG (or NANOG1) and the LDF1/LDR1 pair that amplifies the full-length NANOG1 mRNA (Fig. 1A; supporting information Table S1 and Fig. S1). The results revealed the expected 312-bp F1/R1 NANOG band (supporting information Fig. S2A–S2C) as well as the ∼1-kb LDF1/LDR1 NANOG band (Fig. 1B, 1C; supporting information Fig. S2D) in cultured PCa (Du145, PC3, PPC-1, and LNCaP), breast cancer (MCF7 and MDA-MB435), and colon cancer (Colo320), among others. Importantly, cancer cells freshly purified from xenograft tumors (LAPC4 and LAPC9; supporting information Fig. S2A) as well as 1° human PCa (HPCa; Fig. 1C; supporting information Fig. S2C, S2D) samples also showed NANOG expression. As expected, full-length NANOG mRNA was detected in embryonal carcinoma N-tera cells (Fig. 1B). Similar to NANOG, RT-PCR for OCT4 using a pair of primers that span introns 3 and 4 detected the expected 573-bp band in all cancer cells examined (supporting information Fig. S2A–S2D). By contrast, SOX2 mRNA was detected only in a fraction of the samples, with cultured PCa cells notably lacking SOX2 mRNA (supporting information Fig. S2A–S2B).

Figure 1.

NANOG mRNA in cancer cells results from NANOGP8. (A): Schematic of human NANOG1 gene structure. PCR primers and shRNA vector target locations are indicated in blue and red, respectively. Translational start ATG and stop TGA codons are indicated. (B, C): RT-PCR using LDF1-LDR1. RNA/cDNA template was derived from cultured cancer cells (B) or primary HPCa samples (C). (D): Sequencing analysis. Shown are the nt (and predicted aa) differences between cancer cell-derived NANOG and published NANOG1 and NANOGP8 sequences. The five conserved nts consistent with expression from the NANOGP8 locus are indicated in blue. The single conserved predicted aa change is indicated in red. (E): Differential RT-PCR. F2/R2 primers are specific for NANOG1 whereas F2/R3 primers generate a 467-bp NANOG1 product and a 446-bp NANOGP8 product (arrow). The asterisks indicate two smaller amplicons. (F): NANOG1 in cancer cells is silenced. PC3 cells were treated (72 hours) with AzaC and/or TSA (500 nM each), or vehicle. RT-PCR analysis of extracted RNA (non-treated human embryonic stem cell RNA for comparison) using the F2/R2 primers (NANOG1 specific) versus F2/R3 “universal” NANOG primers. p16 INK4a (hypermethylated in PCa) amplification is used as AzaC control. (G): Cancer cell NANOGP8 cDNAs encode NANOG proteins that can be detected by an anti-NANOG1 antibody. Cancer cell NANOGP8 cDNAs cloned in pET28b(−) were either U or I with IPTG and supernatant (S) or insoluble pellet (P) was used in Western blotting using the mAb. The arrow points to the ∼42 kDa NANOG band. (H): Peptide sequences obtained by MALDI-TOF from MCF7 NANOGP8 cDNA. (I, J): Western blotting using whole cell lysate (WCLl; I) or NE (J) and eBio mAb. Abbreviations: aa, amino acid; AzaC, 5′-aza-2′-deoxycytidine control; E, exon; HPCa, human primary prostate cancer cells; I, induced; NE, nuclear extracts; No RT, no reverse transcription control; nt, nucleotide; RT-PCR, real-time polymerase chain reaction; SP, side population; TSA, trichostatin A; TSS, transcriptional start site; U, uninduced; UTR, untranslated region.

To quantify the relative mRNA expression level of NANOG in cancer cells, we performed real-time quantitative RT-PCR (qRT-PCR) analysis. NANOG mRNA in LAPC4, LAPC9, and Du145 xenograft tumor cells represented only ∼1.4%, 0.5%, and 0.45%, respectively, of the NANOG mRNA levels in undifferentiated hESCs. Primary HPCa cells freshly purified from patient tumors expressed higher relative levels of NANOG mRNA, at 4.5%, 12.1%, and 7.0% for HPCa5, HPCa6, and HPCa7, respectively.

Cancer Cell NANOG mRNA Is Derived from a Transcribed pseudogene, NANOGP8

Human NANOG1 gene (gi 13376297), the gene commonly referred to as NANOG and localized on chromosome 12, has four exons and three introns with a 915-bp open reading frame (ORF) (Fig. 1A). Alternate loci that could potentially encode NANOG mRNA variants include a tandemly duplicated gene NANOG2 (also called NANOGP1 with a 696-bp ORF; [28]) and nine retrotransposed genes, eight of which have defects (e.g., deletions, frameshifts, stop codons, etc.). Interestingly, one NANOG pseudogene (NANOGP8 or PN8 located on chromosome 15; gi 47777342) is free of structural defects and has the potential to be functionally expressed [29].

The F1/R1 primers should amplify a 312-bp NANOG1 or NANOGP8 fragment or a 255-bp NANOG2 product (supporting information Fig. S1 and Table S1). In our experiments, we only detected the 312-bp band (supporting information Fig. S2A–S2C), suggesting that NANOG2 is not expressed in cancer cells. In support, RT-PCR using primers designed to amplify full-length NANOG2 (LDF2/LDR1; supporting information Fig. S1) did not generate NANOG2-specific product in cancer cells (not shown). To distinguish whether cancer cells express NANOG1 and/or NANOGP8 mRNA, we cloned the LDF1/LDR1 PCR products from multiple cancer cells. Sequencing analyses revealed that N-tera cells expressed NANOG1 but not NANOGP8 mRNA, whereas all other cancer cells showed five of six nucleotide (nt) differences specific to NANOGP8 [29] (Fig. 1D, marked in blue). Among the five conserved nt changes in NANOGP8 (relative to NANOG1; [29]), only one (nt759) results in amino acid (aa) change (Q253H; Fig. 1D, indicated in red) although some cancer cells also showed other nonconserved nt changes that could also result in aa changes (e.g., L61P for HPCa6, Fig. 1D). The published nt sequence for NANOGP8 may contain a sequencing error (or polymorphism) at nt 47 (Fig. 1D). No stop codons or frame shifts were detected in any of the cancer cell NANOG transcripts.

To lend further support to NANOGP8 being the major NANOG transcript in cancer cells, we took advantage of a small deleted region in the 3′-untranslated region (UTR) of NANOGP8 (supporting information Fig. S1) and designed primers that can discriminate between NANOG1 and NANOGP8. As shown in Figure 1E, the same forward primer (F2) together with either a downstream “universal” NANOG reverse primer (R3) or an upstream NANOG1-specific reverse primer (R2) (supporting information Table S1 and Fig. S1) both generated a robust PCR product of the correct size in hESCs. In contrast, in cancer cell samples the F2/R2 primer pair failed to generate the 335-bp NANOG1 band (Fig. 1E, top) but the “universal” F2/R3 primer pair detected the expected 446-bp NANOGP8 in cancer cells, and the 467-bp NANOG1 in hESCs (Fig. 1E, bottom, arrow). Interestingly, smaller amplicons were also detected (Fig. 1E, bottom, asterisks), perhaps indicating splicing variations in the 3′UTR of NANOG1 and NANOGP8.

The above results suggest that cancer cells preferentially express NANOG from the NANOGP8 locus rather than NANOG1, which might be silenced in cancer cells as in differentiating ESCs [30]. Indeed, treatment of PC3 cells with the histone deacetylase inhibitor trichostatin A but not the DNA methyltransferase inhibitor 5′-aza-2′-deoxycytidine (Aza) upregulated NANOG1 mRNA (Fig. 1F). In contrast, the mRNA of cyclin-dependent kinase inhibitor p16, known to be silenced in PCa cells because of promoter hypermethylation, was upregulated by Aza treatment (Fig. 1F). Together, these results suggest that cancer cell NANOG transcript is largely derived from NANOGP8.

NANOG Protein Expression in Cancer Cells and Enrichment in CD44Hi PCa and MCF7 Side Population Cells

Human (and mouse) Nanog has 305 aa predicted to encode a ∼35 kDa protein [4]. However, NANOG proteins of 35 kDa to ∼50 kDa have been detected on Western blotting in ESCs, embryonal carcinoma, germ cell tumors, and some cancer cells [e.g.,4, 31]. NANOGP8 mRNA is essentially identical to NANOG mRNA and is thus predicted to encode a nearly identical (>99%) NANOG protein. To determine whether NANOGP8 mRNA in cancer cells could potentially encode a functional protein recognized by anti-NANOG antibodies, we cloned the LDF1/LDR1 NANOGP8 cDNAs into His-tagged bacterial expression plasmids. Western blotting showed that the recombinant proteins derived from the cancer cell NANOGP8 cDNAs were all recognized specifically by an affinity-purified monoclonal anti-Nanog antibody (i.e., eBio mAb; Table S2) as a ∼42 kDa protein (Fig. 1G). The identity of the 42 kDa protein bands was subsequently verified to be NANOG by peptide sequencing (Fig. 1H). For the sake of clarity, and because of the high degree of aa identity between the predicted polypeptides derived from the NANOG1 locus and the NANOGP8 locus, we shall simply refer to the corresponding protein in cancer cells as NANOG in most of the foregoing discussions.

The eBio mAb to NANOG also detected a ∼42 kDa band in PC3, LNCaP, MCF7, Colo320, and WM562 cells using either whole cell lysate (Fig. 1I) or nuclear extracts (Fig. 1J); similar results were obtained using another affinity-purified polyclonal antibody (Kamiya pAb; Table S2; data not shown). The eBio mAb also detected a prominent upper band migrating at ∼47 kDa (Fig. 1I–1J). Both of the bands detected by the eBio anti-NANOG antibody appear specific, because Nanog-shRNA knocked down both bands in LAPC4 xenograft cells (not shown) and completely eliminated the two bands in LNCaP cells (see Fig. 4D, later).

Indirect IF staining using either Ab with Triton permeabilization and biotin amplification (see Methods) readily detected NANOG in undifferentiated “islands” of N-tera cells (supporting information Fig. S3A). Using identical staining protocol, we only detected nuclear NANOG in a small percentage (<1%) of cultured MCF7, LNCaP, and PC3 cells (supporting information Fig. S3A) as well as PCa cells freshly purified from patient tumors (supporting information Fig. S3B). In some cells perinuclear (e.g., in MCF7) or cytoplasmic (e.g., in LNCaP and HPCa11) staining was also observed (supporting information Fig. S3).

Reports of NANOG functioning in higher order protein–protein complexes [6, 32] prompted us to develop a novel IF protocol that incorporated a denaturation step (see Methods). Using this modified protocol, we found that the Kamiya pAb stained NANOG in the nucleus and perinuclear region of Du145 cells (supporting information Fig. S4). The staining was abrogated by preincubating the Ab with recombinant NANOGP8 (supporting information Fig. S4J–S4L) and was largely absent in Du145 cells infected with Nanog-shRNA (supporting information Fig. S4P–S4R). Comparing the two staining protocols in N-tera and LNCaP cells with yet another, newly available anti-NANOG antibody (i.e., the Santa Cruz [SC] pAb; supporting information Table S2) similarly revealed that, although NANOG protein was readily detected in N-tera cells without denaturation, specific nuclear NANOG staining in LNCaP cells was observed only after denaturation (supporting information Fig. S5A). Importantly, the SC pAb, detected predominantly nuclear NANOG in other cancer cells including Du145 and PC3 (Fig. 2A; supporting information Fig. S5B) and the results were confirmed by confocal microscopy (Fig. 2B). A gradient of NANOG staining was apparent with some cells largely negative (Fig. 2Af, circled). Interestingly, we consistently observed higher levels of NANOG in dividing cancer cells (Fig. 2Af and 2Ai; supporting information Figs. S4J–S4I, S5G–S5I, S5M–S5O, S5P–S5R; arrows).

Figure 2.

NANOG protein expression and enrichment in CD44hi PCa cells. ((A): Immunofluorescence (IF) staining of Du145 cells using rabbit (Rb) IgG (control; a-c) or the SC pAb to NANOG (d-i; arrows indicate dividing cells; circle demarcates non-expressors). Note that a dividing cell showed negative staining with Rb IgG (c, arrow). (B): IF staining of cancer cells as in A and images analyzed under a confocal microscope. Shown are clusters of positive cells in N-tera, Du145, and PC3 cultures stained by the SC pAb. (C): Immunohistochemistry (IHC) staining of NANOG in Du145 and MCF7 tumor sections. Shown are a cluster of NANOG-positive cells in Du145 and a single-positive cell in MCF7 (arrow) tumor sections. (D): IHC staining of NANOG in human PCa (HPCa) sections using the Kamiya pAb. Staining with Rb IgG is shown as control. Arrows (b) point to scattered NANOG-positive cells. (E): Coordinate expression of NANOG and CD44 in Du145 cells. Shown are representative confocal images. (F-G): Real-time quantitative real-time polymerase chain reaction analysis of NANOGP8 mRNA expression in (F) CD133+ (+ve)/CD133 (−ve) HPCa39 or CD44+CD133+ (+/+)/CD44-CD133- (−/−) HPCa38 cells and (G) in MCF7 SP and non-SP cells. Abbreviations: Bn, benign; DAPI, 4′,6-diamidino-2-phenylindole; N, NANOG; PCa, Prostate cancer; Rb, rabbit; SC, stem cells; SP, side population; T, tumor.

Using a sensitive polymer-based IHC system (see Methods), we detected nuclear NANOG protein in scattered or clustered tumor cells in MCF7, Du145, and LAPC4 xenografts (Fig. 2C; data not shown). Using the Kamiya Ab, we analyzed NANOG expression in situ in 24 1° HPCa samples and, in 14 cases, compared its expression with the corresponding benign prostate tissues. This small-scale IHC study (Fig. 2D; supporting information Fig. S6 and Table S3) revealed several important points. First, NANOG-positive cells were detected in all HPCa samples but, like the histopathology of HPCa, NANOG expression was heterogeneous at both inter- and intratumoral levels. Second, in Gleason 6 and 7 tumor glands, NANOG-expressing cells were observed in both luminal and basal (like) cells. Third, in the majority of cases, NANOG was distinctly nuclear; however, cytoplasmic staining was observed in a few cases. Fourth, significantly, comparison of NANOG expression in tumors (T) and matched benign (Bn) tissues revealed more NANOG-positive cells in the tumors (Fig. 2Dd–2Df; supporting information Table S3 and Fig. S6). IHC staining using the SC pAb demonstrated similar staining patterns (supporting information Fig. S7) with some dysplastic, undifferentiated tumor areas showing large numbers of nuclear NANOG-positive cells (supporting information Fig. S7A, S7D).

To test the possibility that NANOG-expressing cells might be enriched in potential cancer stem/progenitor cell populations, we carried out double IF staining for NANOG and CD44, which marks PCa stem/progenitor cells [24, 25, 33]. The results revealed that the CD44hi Du145 (Fig. 2E) and PC3 (supporting information Fig. S8) cells appeared to express higher levels of NANOG. CD44 showed typical plasma membrane and cytoplasmic staining, whereas NANOG showed mainly nuclear/perinuclear with some cytoplasmic localization (Fig. 2E; supporting information Fig. S8). qRT-PCR analysis of purified Du145 xenograft cells revealed a 10-fold enrichment of NANOGP8 mRNA in the CD44hi compared with bulk cells (not shown). We further purified, from HPCa38 and HPCa39 tumors, respectively, the CD44+CD133+ and CD133+ cells, previously reported to mark 1° prostate CSCs [34], and qRT-PCR revealed approximately fivefold higher NANOGP8 mRNAs in both populations than their corresponding negative cell populations (Fig. 2F). Moreover, we frequently observed an inverse relationship between NANOG and the prostate differentiation marker AR (e.g., supporting information Fig. S8Bc–S8Bd, S8Cb–S8Cc). Finally, we also observed approximately fourfold higher NANOGP8 mRNA levels in the MCF7 side population cells (Fig. 2G), which we previously had shown to express higher levels of β-CATENIN and NOTCH-1 mRNAs, and be enriched in stem-like tumor-initiating cells [23].

RNA Interference-Mediated Nanog Knockdown Inhibits Tumor Development

The preceding experiments provide convincing evidence for NANOG expression in cancer cells in vitro and in vivo. To determine its potential biological functions in cancer cells, we carried out pilot loss-of-function experiments using small interfering RNA (siRNA) pools. Nanog-siRNA inhibited the clonogenic growth of both LNCaP and MCF7 cells relative to control and Sox2-siRNA (supporting information Fig. S2E–S2H), despite SOX2 expression at the protein level in MCF7 cells (supporting information Fig. S9). To more fully investigate the functions of NANOG in tumor development, we made extensive use of lentiviral vectors encoding specific shRNAs. To ensure the specificity of NANOG knockdown, we utilized three different vectors targeting different regions of NANOG1/NANOGP8 (Fig. 1A; Table 1), including the pLL3.7-based lentiviral vector targeting the 3′-UTR and previously used to knockdown NANOG1 in ESCs (Nanog-shRNA; [27]); an untagged Nanog-shRNA vector obtained from The RNAi Consortium (TRC-shRNA) targeting the coding region of NANOG; and pGIPZ-NANOG (Open Biosystems), targeting the 3′-UTR. Several control vectors included empty vector pLL3.7, a control vector targeting luciferase (LL-LUC), and an shRNA expressing/non-silencing control pGIPZ vector (pGIPZ-control).

Table 1. NANOG knockdown inhibits tumor development
inline image

PCa (Du145, LAPC4, LAPC9, and HPCa18), breast cancer (MCF7), and colon cancer (Colo320) cells were infected with various lentiviral vectors at an multiplicity of infection of 10-20 and then used in tumor experiments. Infected cells (exhibiting decreased NANOG mRNA levels; supporting information Fig. S10) were either injected s.c. in Matrigel into NOD/SCID mice or transplanted in collagen drops under the renal capsule (for HPCa cells). As summarized in Table 1 and Figure 3, the three Nanog-shRNA constructs consistently inhibited tumor development of prostate, breast, and colon cancer cells with smaller and/or fewer tumors. For example, in Du145 PCa cells, two different Nanog-shRNA constructs exhibited similar tumor-inhibitory effects, even relative to the shRNA expressing, nontargeting control (pGIPZ-control; Table 1; Fig. 3Aa). Nanog-shRNA tumors that did arise exhibited reduced green fluorescent protein (GFP; Fig. 3Bb) and so we utilized FACS to sort out the GFPbright Du145 cells from their respective first-generation tumors and carried out 2° transplantation experiments. The 2° GFPbright Nanog-shRNA Du145 cells generated significantly smaller tumors compared with GFPbright LL3.7 cells (Fig. 3Ab). Similar tumor inhibitory effects were obtained in LAPC9 and LAPC4 PCa xenograft tumor models (Fig. 3Ba and Table 1).

Figure 3.

Downregulation of NANOG inhibits tumor development. (A): Nanog-shRNA inhibits Du145 tumor development and serial transplantation. (a) Sphere-derived Du145 cells transduced with the indicated pGIPZ vectors at multiplicity of infection of 10 were sorted 72 hours later, and 25,000 cells injected subcutaneously (s.c.) in Matrigel into NOD/SCID mice. Tumors were harvested 63 days after injection (a) and tumor weights are indicated in Table 1. (b) A total of 10,000 sorted GFP+ tumor cells purified from 1° tumors (Table 1) were used in 2° transplantation. (B): Nanog-shRNA inhibits LAPC9 tumor development. (a) LAPC9 cells infected with the indicated vectors were sorted 72 hours later and 1,000 GFP+ tumor cells of each type were injected s.c. in Matrigel into the male NOD/SCID mice supplemented with testosterone. Tumors were harvested 61 days later. NANOG-sh 1 and 2 were two separate infections. Tumor weights are indicated in Table 1. (b) GFP images. (C, D): Nanog-shRNA inhibits human primary prostate cancer cells tumor development. (C) Representative images of outgrowths (arrows; top) and corresponding histology (×100; bottom). (D) Enlarged images of outgrowth in LL3.7 recombinants (a and b; ×400) and immunohistochemistry staining for human mitochondria (c). Note blue color indicates implantation site. (E): NANOG knockdown inhibits MCF7 tumor development. MCF7 cells (100,000) were transduced with the lentiviral constructs (MOI 20) and injected s.c. in Matrigel into female NOD/SCID mice supplemented with estrogen pellets. (a) Tumor growth curve (see supporting information). (b) Tumor images. (F): Nanog-shRNA inhibits Colo320 tumor development. Colo320 cells (250,000) infected with the indicated lentiviruses (MOI 20) were injected in Matrigel s.c into the NOD/SCID mice. (a, b) Tumor images. Tumor weights are indicated in Table 1. (c) GFP images. Abbreviations: GFP, green fluorescent protein; K, mouse kidney; N, normal glands; PIN, prostate intraepithelial neoplasia; S, stroma; T, tumor.

To determine whether NANOG is also potentially involved in 1° HPCa tumorigenicity, freshly purified HPCa18 cells were transduced and recombined 10,000 cells each with an equal number of rUGSM cells and transplanted under the renal capsule of male NOD/SCID mice. This pilot experiment showed that LL3.7-infected HPCa18 cells formed the largest outgrowths (2/2), whereas the Oct4-shRNA infected cells generated smaller outgrowths (2/2) and the Nanog-shRNA-infected cells did not regenerate any outgrowth (0/2) (Fig. 3C–3D and Table 1). Histologically, the LL3.7-infected HPCa18 cells reconstituted the full spectrum of pathological lesions present in the patient tumor, consisting of benign glands and prostate intraepithelial neoplasia-like lesions (Fig. 3Da), and undifferentiated tumor cells with highly pleiomorphic nuclei (Fig. 3Db). The outgrowth was derived from human cells as evidenced by staining for human-specific mitochondria (Fig. 3Dc).

Likewise, NANOG knockdown inhibited MCF7 and Colo320 tumor development (Table 1). As shown in Figure 3E, both Nanog-shRNA and TRC-shRNA significantly inhibited MCF7 tumor development, and, although Oct4-shRNA demonstrated a modest inhibitory effect on MCF7 tumor development, the effect was not statistically significant (Fig. 3Ea, 3Eb). Similarly, knocking down NANOG consistently inhibited Colo320 tumor development, whereas Oct4-shRNA demonstrated inconsistent effects (Table 1; Fig. 3Ea, 3Eb). As observed for Du145, LAPC9, and LAPC4 cells, Nanog-shRNA transduced Colo320 tumors that did arise had mostly lost GFP (Fig. 3Fc), suggesting that these tumors likely regenerated from rare tumor cells that were uninfected or alternatively, from tumor cells that had lost shRNA (and corresponding GFP) expression.

Nanog-shRNA-Transduced Cancer Cells Exhibit Decreased Proliferation and Clonal/Clonogenic Potentials

Next, we explored the molecular mechanisms underlying the tumor-inhibitory effects of NANOG knockdown. Nanog-shRNA significantly restricted the clonal expansion of PC3 cells such that cells infected with Nanog-shRNA formed only sparse clones, whereas cells infected with LL3.7 became confluent (Fig. 4A). Oct4-shRNA showed no apparent effect (Fig. 4A; supporting information Fig. S11) although both Nanog-shRNA and Oct4-shRNA partially downregulated their respective target mRNAs in PC3 cells (supporting information Fig. S10). Upon serial passaging, Nanog-shRNA significantly inhibited the cumulative population doublings (Fig. 4Ba), and in clonal analysis, Nanog-shRNA and TRC-shRNA treated cells showed lower cloning efficiency (CE) and smaller clone sizes (Fig. 4Bb, 4Bc; supporting information Fig. S11). In 2° clonal analysis, cells initially infected with the control or Oct4-shRNA lentiviruses showed enhanced CE, whereas the Nanog-shRNA infected PC3 cells exhibited lower CE (Fig. 4Bd).

Figure 4.

NANOG downregulation restricts clonal and clonogenic growth of prostate cancer cells. (A): PC3 cells infected with the indicated lentiviral vectors (multiplicity of infection 25) were dissociated and replated, 72 hours later, at clonal density in a 6-well plate (100 cells/well). Images 12-day postplating (×200). (B): PC3 cells infected with the indicated vectors (above) were serially passaged and cumulative PDs determined (a). Arrows, p < .05. (b) 1° CE: 100 infected PC3 cells were plated per well in a 6-well plate; clones were counted 10 days or (c) 17 days after plating. (d) 2° clonal analysis: 1° clones were cloned out using a cloning ring and replated at 100 cell/well; 2° clones were counted at 10 days. For b-d, data for each condition were derived from at least six samples (mean ± S.D.). (C): Hundred infected LNCaP cells (transduced as described above) were plated for CE and clones scored at (a) 14 days or (b) 37 days postplating. (c) Giemsa staining of clones at 37 days. (d) LNCaP 2° clonogenicity: 1,000 infected LNCaP cells were plated on 1% agarose, and, 15 days later, 1° spheres were harvested, dissociated with trypsin, and replated. (D): Western blotting (60 μg wcl/lane; eBio mAb) of LNCaP cells infected with LL3.7, NANOG- or TRC-shRNAs (72-hour postinfection). Abbreviations: CE, clonal efficiency; GFP, green fluorescent protein.

Nanog-shRNA and TRC-shRNA completely abrogated NANOG protein expression (Fig. 4D), coincident with inhibited clonal expansion of LNCaP cells (Fig. 4Ca–4Cc; supporting information Fig. S12). Nanog-shRNA also inhibited the clonogenicity of LNCaP cells sufficiently to ablate the formation of 2° spheres (Fig. 4Cd). Nanog-shRNA similarly inhibited the clonal (supporting information Fig. S12A, S12B) and clonogenic (not shown) potentials of another PCa cell line, Du145. The apparent growth inhibitory effect of NANOG knockdown was not associated with increased cell death as assessed by morphology, Annexin V labeling, and nuclear 4′,6-diamidino-2-phenylindole staining (data not shown). Rather, cell proliferation was partially inhibited as assessed by BrdU incorporation assays (supporting information Fig. S12C, S12D).

To determine whether NANOG regulates in vitro growth properties of patient tumor cells, we purified HPCa22 cells from prostatectomy specimen and carried out clonal and clonogenic assays. As shown in Figure 5A and 5B and supporting information Table S4, both Nanog-shRNAs strongly inhibited the clonal growth of 1° HPCa22 cells. Oct4-shRNA marginally inhibited the clonal development of HPCa22 cells but the inhibitory effect was not statistically significant (supporting information Table S4). LL3.7-infected HPCa22 cells formed tight holoclones (large compact clones previously shown to contain self-renewing cancer cells [35]), whereas cells infected with the NANOG/TRC-shRNA generally formed small paraclones composed of scattered, large cells (Fig. 5A–5C). When the clonal cultures were passaged, LL3.7-infected cells proliferated extensively and formed a typical “cobblestone”-like epithelial sheet, whereas HPCa22 cells infected with Nanog-shRNA became large and flat, and turned senescent evidenced by positive SA-βgal staining (Fig. 5C–5D). Similar clonal experiments with HPCa25 and HPCa37 also revealed inhibitory effects of Nanog-shRNAs (supporting information Table S4).

Figure 5.

NANOG downregulation restricts clonal and clonogenic growth of primary human primary prostate cancer cells (HPCa) cells. (A-D): Nanog-shRNA inhibits clonal expansion of HPCa22 cells. Freshly purified HPCa22 cells were infected overnight with indicated lentivirus and plated (n = 3) at 10,000 cells/well on mitomycin C-treated Swiss 3T3 fibroblast feeders. (A) Representative images of clones in C (×100). (B) Holoclones were enumerated 16 days after plating; results represent the mean ± S.D. (C) 2° clonal analyses: HPCa22 1° clones were dissociated and replated on fibroblasts and (D) 3 weeks later, cells were stained for SA-βgal (×100). (E-F): Nanog-shRNA inhibits sphere formation of HPCa22 cells. (E) Transduced HPCa22 cells (above) were plated (n = 3) at 25,000 cells/well (in 6-well plate) on agarose. Spheres were enumerated 16 days after plating and the results represent the mean ± S.D. (F) Representative images (×100) of OCT-embedded spheres; HE and immunofluorescence staining for CD44 (red) and DNA (4′,6-diamidino-2-phenylindole-blue). Abbreviations: GFP, green fluorescent protein; HE, hematoxylin and eosin.

Nanog-shRNAs also inhibited the anchorage-independent growth of HPCa22 cells. Although LL3.7-infected HPCa22 cells formed numerous large/solid spheres, HPCa22 cells infected with either Nanog-shRNA formed fewer and smaller spheres (Fig. 5E) exhibiting a differentiated morphology with a hollow core (Fig. 5E–5F). Interestingly, CD44 appeared downregulated in Nanog-shRNA spheres (Fig. 5F). When the 1° spheres were dissociated and replated, the LL3.7, Oct4, NANOG, and TRC-shRNA infected cells showed a 2° sphere-forming capacity of 54 ± 12, 22 ± 3.8, 16 ± 3.2, and 0, respectively. Similarly, LAPC4 xenograft cells transduced with Nanog-shRNA constructs also demonstrated reduced sphere-forming potential (supporting information Fig. S13).

Nanog-shRNA also inhibited MCF7 breast cancer cell clonal expansion (Fig. 6A) clearly associated with an inhibition of proliferation (Fig. 6B, 6C). Following a 4-hour BrdU pulse, ∼49% of the LL3.7 or Oct4-shRNA transduced MCF7 cells incorporated BrdU, whereas only ∼22% of the Nanog-shRNA-infected MCF7 cells incorporated BrdU. We took advantage of this distinct phenotype and carried out a functional “rescue” experiment to confirm the specificity of the Nanog-shRNA effects. We cloned the HPCa5-NANOGP8 cDNA into the pPyCAG expression plasmid [3] which, when transfected into MCF7 cells, produced NANOGP8 protein (supporting information Fig. S14A). MCF7 cells transduced with LL3.7 or the two Nanog-shRNA vectors were subsequently (24 hours later) transfected with pPyCAG or pPyCAG-NANOGP8 and, 48 hours after transfection, cells were pulsed with BrdU. Immunostaining revealed that both Nanog-shRNAs significantly downregulated the percentages of BrdU-positive cells and NANOGP8-cDNA fully “rescued” (i.e., reversed) the Nanog-shRNA phenotype but not the TRC-shRNA effect (Fig. 6C; supporting information Fig. S14B). This was expected because Nanog-shRNA targets the 3′-UTR, whereas TRC-shRNA targets the coding region (Fig. 1A). Therefore, the NANOGP8-cDNA (encoded by pPyCAG-NANOGP8; supporting information Fig. S14B) will still be degraded by TRC-shRNA but not by Nanog-shRNA. The functional rescue experiments strongly suggest that the loss-of-function phenotypes of Nanog-shRNAs on cancer cell clonal/clonogenic growth and tumor development are direct and specific consequences of NANOG downregulation.

Figure 6.

NANOG knockdown inhibits MCF7 cell clonogenic growth, reduces proliferation and alters differentiation. (A): MCF7 clonal growth. MCF7 cells (100) infected with the indicated vectors were plated (n = 3) in 6-well plates. Twenty-one days postplating, cells were trypsinized, pooled, and counted. (B): BrdU incorporation assays. MCF7 cells infected with the indicated lentiviruses were cultured overnight on glass coverslips and pulsed with 5 μM BrdU for 4 hours. Fixed cells were processed for BrdU immunostaining (red), markedly reduced in Nanog-shRNA transduced cells. (C): Functional “rescue” experiments. MCF7 cells were infected with the indicated vectors (LL, LL3.7; N, Nanog-shRNA; TRC, TRC-shRNA; multiplicity of infection 20) and 24 hours later, transfected with either pPyCAG or pPyCAG-PN8 (i.e., NANOGP8). 48-hour later cells were pulsed with BrdU (4 hours) and processed for BrdU staining. A total of 500-1,000 cells were counted by three individuals and the bars represent the mean ± S.D. *p < .05 between the two conditions. (D): 2° MCF7 clonogenic growth. MCF7 cells (1000) were plated (n = 3) on agarose, and spheres were scored 10 days postplating. (E): 2° sphere images. One° spheres were harvested (10 days after infection) and replated. Shown are representative images one month after replating. (F): Tumors derived from Nanog-shRNA and TRC-Nanog-shRNA-infected MCF7 cells appeared more differentiated (ductal structures and increased mucin) and exhibit lower proliferation (Ki67) than the control tumors. Five-micrometer serial sections were stained for HE or the molecules indicated on the right (×200). Abbreviations: BrdU, 5-bromo-2-deoxyuridine; DAPI, 4′,6-diamidino-2-phenylindole; GFP, green fluorescent protein; HE, hematoxylin and eosin.

Nanog-shRNA transduced MCF7 cells also exhibited significantly decreased clonogenic growth (Fig. 6D–6E) consistent with NANOG siRNA-mediated inhibition of sphere formation (supporting information Fig. S2H). Upon passaging of the 1° spheres, LL3.7-infected MCF7 cells showed robust 2° sphere formation, whereas the Nanog-shRNA 1° spheres formed degenerate 2° spheres that could not be further passaged (Fig. 6E and data not shown). The striking hollow spheres formed by Nanog-shRNA transduced MCF7 cells (Fig. 6E) suggest that NANOG knockdown might be causing a differentiation phenotype. In support, the LL3.7-infected MCF7 tumors were comprised of characteristic undifferentiated, cytokeratin 18-positive carcinoma cells, many of which were proliferating as evidenced by positive Ki67 staining (Fig. 6F). In contrast, the two Nanog-shRNA infected MCF7 tumors demonstrated a more differentiated histology with numerous glandular-like structures exhibiting increased mucin production and fewer Ki67-positive cells (Fig. 6F).


In this study, we have endeavored to systematically investigate the expression, origin, and functions of NANOG in tumor cells and we have made the following significant findings. First, multiple tumor cells in vitro and in vivo express NANOGP8 mRNA as well as NANOG protein. Second, NANOG-positive cells are increased in prostate tumors compared with the benign tissues and, NANOGP8 mRNA and NANOG protein seem to be enriched in the CD44hi PCa stem/progenitor cells. Third, most importantly, downregulation of NANOG inhibits tumor development of prostate, breast, and colon cancer cells. Finally, the tumor-inhibitory effects of NANOG knockdown are associated with an inhibition of cell proliferation, clonal expansion, and clonogenic growth of tumor cells. Thus, NANOG expressed in human cancer cells is biologically functional in regulating tumor development.

Zhang et al. [31] has previously reported that several tumor cell lines express NANOGP8. We confirm and significantly extend these findings in a large panel of cancer cell lines and xenograft and 1° HPCa samples. We further provide evidence that tumor cell-derived NANOGP8 is biologically active in that its enforced expression could functionally rescue the proliferative defect caused by a 3′-UTR-targeting Nanog-shRNA. This work, to our knowledge, represents the most comprehensive study on endogenous NANOG protein expression in cancer cells. Curiously, IF staining using the standard permeabilization protocol only identifies NANOG expression in a small population of cultured cells. However, denaturation before immunolabeling reveals NANOG expression as a hierarchy or gradient. Thus, a small percentage of cultured cancer cells seem to express high levels of NANOG that can be readily detected by regular staining protocol. A similar gradient in NANOG positivity has also been observed in PCa cells in situ, a heterogeneous NANOG expression pattern that is reminiscent of its expression pattern in ESCs [36]. Since most cultured N-tera cells readily reveal NANOG without requiring denaturation, the NANOG protein in cancer cells might be biochemically distinct and/or present in unique protein complexes.

The increased nuclear NANOG expression in a fraction of tumor cells raises the possibility that these cells might represent tumor stem/progenitor cells. In support, we have found evidence that both NANOGP8 mRNA and NANOG protein are enriched in the CD44hi HPCa cell populations, which harbor colony- and tumor-initiating PCa stem/progenitor cells [24, 25, 34]. These observations are interesting in light of a recent report that suggests that cell surface CD44, upon binding to its ligand hyaluronan, may interact in the cytoplasm with NANOG in MCF7 cells to activate ABC transporter expression via a Stat3-dependent mechanism [37]. Indeed, we frequently observe a small fraction of cytoplasmically localized NANOG in cancer cells and, NANOG and CD44, although showing overall distinct subcellular localization, are sometimes observed adjacent to each other in the cytoplasm. Although normal prostate SCs are thought to localize mainly in the basal layer of the prostatic glands [38], NANOG-expressing PCa cells in tumor glands appear to localize in both basal and suprabasal layers. Preliminary observations show inverse nuclear NANOG and AR expression in a subset of PCa cells in situ (supporting information Fig. S7B, S7C), consistent with the notion that NANOG-expressing PCa cells might be less differentiated cancer stem/progenitor cells. Further studies to validate the observed correlation between NANOG expression and PCa stem/progenitor cells (e.g., CD44+/high, CD133+, AR−/low) are currently ongoing. Regardless, our data show that NANOG-expressing cells are increased in PCa compared with corresponding benign tissues. Whether the abundance of NANOG-expressing cells correlates with tumor grade, stage, and propensity to disseminate will await further studies using a larger cohort of patient samples. Notably, through an unbiased prospective proteomic analysis, Alldridge et al. [8] reported that NANOG was overexpressed in 1° breast cancers.

The most significant finding of this study is that NANOG knockdown inhibits tumor development and this inhibitory effect has been observed in three different tumor systems. Since two Nanog-shRNAs targeting the 3′-UTR and one Nanog-shRNA targeting the coding region have all demonstrated inhibitory effects, the loss-of-function phenotypes are likely related to direct NANOG inhibition rather than to some off-target effects. In support, several different types of control vectors do not display tumor-inhibitory effects. Furthermore, in contrast to the reproducible tumor-inhibitory effects of NANOG knockdown, Oct4-shRNA shows inconsistent tumor-inhibitory effects. This latter observation is intriguing in that Nanog and Oct4 cooperate to regulate several hundred target genes and self-renewal process in ESCs [5, 6].

How might NANOG regulate tumor development? We have demonstrated that downregulation of NANOG is associated with decreased cancer cell proliferation both in vitro and in vivo. Furthermore, high NANOG-expressing cells are often found to be undergoing cell division. These observations are in accord with overexpressed NANOG being able to promote NIH3T3 cell proliferation [15]. The fact that NANOG downregulation inhibits serial clonal growth, sphere development, as well as serial tumor transplantations suggests that NANOG in tumor cells might enhance self-renewal. Alternatively, NANOG decrease may drive aberrant differentiation, such as that observed in Nanog-shRNA MCF7 tumors (this study). Further experiments are required to discriminate among relative contributions of altered proliferation, self-renewal, and/or differentiation states, as well as associated perturbations in the cell cycle, in cancer cells exhibiting decreased NANOG expression.

Complementing the loss-of-function studies in tumors in this study, we have found that ectopic expression of patient tumor-derived NANOGP8 in the K14 cellular compartment in transgenic mice disrupts tissue homeostasis associated with hyperplasia, dysplasia, and abnormal differentiation (Badeaux et al., manuscript in preparation). Although we are still dissecting the detailed molecular mechanisms underlying these proliferation and differentiation defects caused by NANOG expression, the apparent dysplasia, hyperplasia, and abnormal differentiation, which are omnipresent histological traits of all benign tumors and cancers, strongly suggest that cancer cell NANOG could possess oncogenic potential.

In summary, this study presents compelling experimental evidence that a variant of the ESC self-renewal gene NANOG also functions in human tumor development. The study also raises many critical questions, foremost among which are the following: How is NANOGP8 transcriptionally activated and regulated in tumor cells? What are the NANOG-mediated signaling networks in tumor cells? Does NANOG expression promote tumor initiation and/or malignant progression? The answers to these important and interconnected questions, which we are actively pursuing, will help us better understand the functions of NANOG in regulating tumor development.


We are grateful to Dr. K. Kiguchi for confocal microscopy, K. Claypool for FACS, Dr. JJ Shen and MB Core for sequencing and qPCR, Nancy Otto and Histology Core for IHC, Drs. JJ Shen and M. Person and Proteomics Core for protein ID, S. Gaddis for sequence alignment, Animal Facility Core for tumor-related experiments, Drs. R. Fagin, S. Pickett, J. Waxman, and L. Dalton for primary HPCa samples, and other members of the Tang lab for support and helpful discussions. We also thank Dr. I. Chambers for the pPyCAG vector, and Dr. S. Orkin for critically reading the manuscript. This work was supported in part by grants from NIH (R01-AG023374, R01-ES015888, and R21-ES015893-01A1), American Cancer Society (RSG MGO-105961), Department of Defense (W81XWH-07-1-0616 and W81XWH-08-1-0472), Prostate Cancer Foundation, and Elsa Pardee Foundation (D.G.T) and by two Center Grants (CCSG-5 P30 CA166672 and ES07784). C. Jeter was supported in part by a postdoctoral fellowship from NIH and American Urological Association. G. Choy and D. Chandra were supported in part by a postdoctoral fellowship from DOD and an NIH K01 award, respectively. M. Badeaux and L. Patrawala were supported in part by predoctoral fellowships from NIEHS and DOD, respectively. We apologize to those colleagues whose work could not be cited due to stringent space limit.


The authors indicate no potential conflicts of interest.