|Home | About | Journals | Submit | Contact Us | Français|
Users may view, print, copy, download and text and data- mine the content in such documents, for the purposes of academic research, subject always to the full Conditions of use: http://www.nature.com/authors/editorial_policies/license.html#terms
Variable drug responses among malignant cells within individual tumors may represent a barrier to their eradication using chemotherapy. Carcinoma cells expressing mesenchymal markers resist conventional and epidermal growth factor receptor (EGFR)-targeted chemotherapy. Here we evaluated whether mesenchymal-like subpopulations within human squamous cell carcinomas (SCCs) with predominantly epithelial features contribute to overall therapy resistance. We identified a mesenchymal-like subset expressing low E-cadherin (Ecad-lo) and high vimentin (Vim-hi) within upper aerodigestive tract SCCs. This subset was both isolated from cell lines and identified in xenografts and primary clinical specimens. The Ecad-lo subset contained more low-turnover cells, correlating with resistance to the conventional chemotherapeutic paclitaxel in vitro. Epidermal growth factor (EGF) induced less stimulation of the MAP kinase and PI3-kinase pathways in Ecad-lo cells, which was likely due to lower EGFR expression in this subset and correlated with in vivo resistance to the EGFR-targeted antibody cetuximab. The Ecad-lo and high E-cadherin (Ecad-hi) subsets were dynamic in phenotype, showing the capacity to repopulate each other from single cell clones. Taken together, these results provide evidence for a low-turnover, mesenchymal-like subpopulation in SCCs with diminished EGFR pathway function and intrinsic resistance to conventional and EGFR-targeted chemotherapies.
The inability to eradicate SCCs of the upper aerodigestive tract, including those of the head and neck (HNSCC) and esophagus (ESCC), with chemotherapy alone is a feature shared with most other malignancies. Drug therapy for advanced stage HNSCC has benefited from two recent advances: inclusion of paclitaxel in conventional chemotherapy regimens (Posner et al., 2007; Vermorken et al., 2007) and introduction of the EGFR-targeted antibody cetuximab into clinical use (Bonner et al., 2006; Herbst et al., 2005). Although these agents can produce dramatic responses, cancer recurrence is inevitable without addition of other therapeutic modalities, and treatment failures are common even with use of combined modalities. Thus, identifying and targeting minority SCC subpopulations with intrinsic resistance to these two agents is an appealing strategy for tumor eradication.
Epithelial to mesenchymal transition (EMT) generates phenotypic heterogeneity within SCCs and is one potential basis for defining subpopulations with intrinsic drug resistance. The hallmark of EMT is loss of cell surface E-cadherin, which accompanies disassembly of adherens junctions, acquired motility, and expression of mesenchymal markers including vimentin, N-cadherin, and fibronectin (Christiansen and Rajasekaran, 2006; Hugo et al., 2007). The EMT program is coordinated by multiple transcription factors, including the Twist, Snail, and Zeb families (Ansieau et al., 2008; Cano et al., 2000; Peinado et al., 2007). Originally characterized as an embryologic process that drives cell migration and diversifies phenotype, EMT concepts remain controversial in application to cancer biology. While recognizable in carcinoma lines, the dramatic phenotypic shifts of EMT are generally not observed to similar extent in vivo (Tarin et al., 2005), and it is doubtful whether carcinomas ever fully acquire mesenchymal features to parallel events during development. However, a range of mesenchymal traits do exist across SCCs, and we therefore favor the label “mesenchymal-like” to designate phenotypes arising from EMT in malignancy.
Thus far, drug resistance arising from EMT has been assessed mainly by comparing cell lines possessing or lacking prominent expression of mesenchymal markers, based on the premise that this property distinguishes two subtypes of tumors. Several studies have correlated mesenchymal-like traits with higher overall resistance to conventional cytotoxic chemotherapies (Wang et al., 2009; Yang et al., 2006) and EGFR inhibitors (Fuchs et al., 2008; Thomson et al., 2005; Yauch et al., 2005). However, carcinomas rarely fall cleanly into dichotomous epithelial or mesenchymal-like categories in vivo and instead show either predominantly epithelial features or a spectrum of mixed epithelial and mesenchymal-like differentiation (Strauss et al., 2009). It is presently unclear whether the intrinsic drug resistance in “mesenchymal” carcinoma lines is actually attributable to discrete mesenchymal-like subpopulations within them and whether comparable populations in vivo play a similar role.
Here we identify and isolate a minority mesenchymal-like subpopulation from SCCs bearing predominantly epithelial features. Distinctive growth and EGFR-signaling properties are identified in this subset and correlated with intrinsic resistance to paclitaxel and cetuximab in vitro. In addition, cetuximab resistance of these cells is evaluated in vivo using direct xenografts of human primary tumors. To clarify the developmental relationship between the epithelial and mesenchymal-like subpopulations, the phenotypic stability of each is tracked at a clonal level.
Initially, the variability in epithelial versus mesenchymal-like differentiation was defined in a panel of ten SCC cell lines, which segregated into three general patterns based on E-cadherin and vimentin staining. One end of the spectrum is represented by the SCC15, TE12, and SCC13 cell lines, which demonstrate diffuse E-cadherin expression and limited or no vimentin-staining (Figure S1A). TE1, SCC9, OCTT2, and TE9 cells represented and intermediate pattern, with distinct E-cadherin and vimentin-positive populations, and, in the case of TE9, a sizeable subset expressing both markers (Figure S1B). The other extreme is exemplified by the SCC4, TE8, and HCE4 cell lines, which show diffuse vimentin staining and minimal E-cadherin-expressing cells (Figure S1C).
To facilitate a study of mesenchymal-like subsets in tumors with predominantly epithelial features, we selected two HNSCC lines (SCC9 and OCTT2) containing minority subpopulations sizeable enough to isolate. These lines appeared heterogeneous in culture, with clustered epithelial-like cells interspersed with fusiform mesenchymal-like morphologies (Figure 1A, left panels). Both lines were comprised mostly of non-overlapping Ecad-hi/Vim-lo and Ecad-lo/Vim-hi populations (Figure 1A, right panels). The minimal overlap between these phenotypes was confirmed by segregating each line into Ecad-hi and Ecad-lo groups (Figure 1B, top) by fluorescence-activated cell sorting (FACS) and demonstrating vimentin staining reciprocal to E-cadherin expression in sorted subsets (Figure 1B, bottom). To confirm that Ecad-lo cells possess mesenchymal-like differentiation, gene expression profiles of Ecad-hi and Ecad-lo populations were compared. SCC9 and OCTT2 Ecad-lo cells up-regulated multiple genes associated with EMT (Figure 1C, left) and also down-regulated genes characteristic of epithelial phenotypes (Figure 1C, right). These findings confirmed that FACS-purification of Ecad-hi and Ecad-lo cells was a valid method of segregating the epithelial and mesenchymal-like subsets. Thus the terms “Ecad-hi” and “Ecad-lo” are subsequently used interchangeably with “epithelial” and “mesenchymal-like” in reference to SCC9 and OCTT2 cells.
Mesenchymal-like subpopulations were identified in vivo using dual immunohistochemistry (IHC) staining for E-cadherin and vimentin. Mouse xenografts of the SCC9 line contained a small vimentin positive subset with fusiform morphology, distinct from the E-cadherin-positive majority (Figure 1D, top left). To enhance the visual contrast between vimentin and E-cadherin staining, chromogens were digitally converted to red and green pseudo-colors, respectively (Figure 1D, bottom left). A vimentin-expressing subpopulation was also observed in the original human primary tumor from which the OCTT2 line was derived (Figure 1D, middle), although detection of nonmalignant stromal cells by the human-specific vimentin antibody could not be excluded here. For this reason, a similar vimentin-positive subset was sought and identified in a direct xenograft of this primary tumor (Figure 1D, right). Here mouse passage is expected to deplete all nonmalignant human cells, and use of human-specific antibody prevented labeling of mouse-derived stromal cells within xenografts. The malignant potential of the mesenchymal-like subset was demonstrated by comparing in vivo growth of sorted Ecad-hi versus Ecad-lo cells from the OCTT2 cell line (Figure S2). As xenografts, these purified subsets showed no major differences in latency, growth, histology, or distribution of mesenchymal-like cells in mature tumors. The broad in vivo relevance of the vimentin-positive subpopulation is underscored by SCC9 and OCTT2 tumors representing opposites in the spectrum of HNSCC grades, from well-differentiated to poorly differentiated (Figure S3).
To determine whether the mesenchymal-like subpopulation had altered growth features, proliferation of Ecad-hi and Ecad-lo SCC9 cells was compared by MTT assay, which demonstrated slower growth in the Ecad-lo compartment (Figure 2A). Reduced growth of Ecad-lo cells coincided with a higher proportion in G0/G1 phase by cell cycle analysis (Figure 2B) and double the percentage in resting G0 phase, as defined by absence of Ki-67 expression (Figure 2C). The turnover characteristics of Ecad-hi and Ecad-lo subpopulations were compared over an extended period, based on dilution of the fluorescent membrane label PKH-67 with ongoing cell division. After uniform PKH-67 labeling, SCC9 cells were grown in culture for 9 days to create a broad distribution of PKH-67 intensity (Figure 2D). Low and high turnover subsets were defined as populations with the 10% highest and 10% lowest PKH-67 label, respectively. Low turnover (high label-retaining) SCC9 cells contained over 5-fold more Ecad-lo cells relative to high turnover (low label-retaining) cells. Taken together, these results indicated that the mesenchymal-like subpopulation contains a larger proportion of low turnover cells and is less proliferative overall.
To assess whether diminished growth of the mesenchymal-like subset correlates with paclitaxel resistance, FACS segregated Ecad-hi and Ecad-lo cells were compared for drug-induced growth inhibition (Figure 3A). The half-maximal growth inhibitory concentration (IC50) for Ecad-lo cells was 2-log higher in SCC9 and 1.5-log higher in OCTT2, relative to Ecad-hi cells, using a 4 hour drug exposure. Prolonging the drug exposure time to 48 hours minimally impacted this difference in IC50 for OCTT2 and diminished it to a still-significant 0.75 log for SCC9 (Figure S4). Unsorted SCC9 cells also showed evidence of paclitaxel resistance in the Ecad-lo subset, which became enriched from 18% to 50% in cultures after brief drug exposure (Figure 3B, left and second panel). To exclude that paclitaxel down-regulated E-cadherin without truly enlarging the mesenchymal-like subpopulation, Ecad-lo and Ecad-hi cells surviving treatment were demonstrated to retain Vim-hi and Vim-lo phenotypes, respectively. (Figure 3B, third panel). Despite a decrease in IC50 for SCC9 Ecad-lo cells with prolonged drug exposure, 48 hours of treatment did not reduce the enrichment of Ecad-lo cells (Figure 3B, right panel). Growth potential of Ecad-hi and Ecad-lo cells surviving paclitaxel was defined by comparing their clonogenicity (Figure 3C, left) and proliferation (right). While treating Ecad-hi cells reduced their clonogenicity and overall growth, paclitaxel minimally impacted these properties in surviving Ecad-lo cells. These results demonstrated that the Ecad-lo subset not only possessed elevated intrinsic resistance to killing by paclitaxel but also maintained growth potential post-therapy.
SCC9 cultures were tracked by video to distinguish whether paclitaxel enriched the Ecad-lo subset by selectively depleting Ecad-hi cells or by causing differentiation toward the mesenchymal-like phenotype. Videos of untreated cells contrast rapidly dividing cells of epithelial morphology against slowly proliferative but more migratory cells of mesenchymal appearance (Video 1). In treated cells, cell death localized to areas with epithelial morphology, sparing regions with mesenchymal-like differentiation (Video 2 and Figure 3D). This finding demonstrated that the Ecad-hi subset was selectively killed by paclitaxel and suggested its depletion as the major mechanism behind relative expansion of the Ecad-lo subpopulation.
The EGFR-targeted antibody cetuximab is another key agent in clinical use against SCCs. To assess potential responsiveness of the mesenchymal-like subpopulation to EGFR targeting, we compared the integrity of EGFR signaling pathways between the Ecad-lo and Ecad-hi subsets. Flow cytometry (FC) of SCC9 and OCTT2 lines identified decreased surface EGFR expression in the Ecad-lo versus Ecad-hi subsets (Figure 4A, left/middle). Reduced surface EGFR expression in the Ecad-lo subset was also demonstrated in vivo by analyzing disaggregated xenografts of the tumor from which the OCTT2 line was derived (Figure 4A, right). This reduction in surface EGFR corresponded with diminished total EGFR levels in the mesenchymal like subset, as shown by immunofluorescence (IF) staining (Figure S5A), FC of permeabilized cells (Figure S5B), and western blot (Figure S5C).
We assessed whether EGFR down-regulation in Ecad-lo cells corresponded with diminished capacity of the receptor to regulate the downstream phosphatidylinositol-3-kinase (PI3K) and mitogen-activated protein kinase (MAPK) pathways. Minimal activation of both ERK (Figure 4B) and AKT (Figure 4C) was seen in serum-starved vimentin-positive SCC9 cells upon addition of EGF, in contrast to prominent activation of both molecules by ligand in vimentin-negative cells. Costaining for E-cadherin in place of vimentin confirmed a pattern of selective ERK/AKT activation in the Ecad-hi subset by EGFR ligand (Figure S6). Taken together, these results provide evidence that the MAPK and PI3K pathways are uncoupled from regulation by EGFR-specific ligands in Ecad-lo cells, most likely as a consequence of decreased EGFR expression in this subset.
Reduced signaling through EGFR in the Ecad-lo subset predicted diminished responsiveness to cetuximab. Accordingly, cetuximab showed greater activity against Ecad-hi cells in both SCC9 and OCTT2 (Figure 5A). To assess whether the mesenchymal-like subset was cetuximab-resistant in vivo, mice xenografted with the tumor of origin for the OCTT2 cell line were treated with cetuximab. Partial regression of established tumors was observed over 12 days, during which time saline-treated controls grew rapidly (Figure 5B). Dual label IHC staining of treated tumors showed a marked increase in vimentin-expressing areas relative to controls (Figure 5C, first row), and visual contrast between the dual subpopulations was enhanced by pseudo-coloring the chromogens (second row). Dual IHC-stained tumors were analyzed to quantify the increase in vimentin staining area by comparing wide fields of treated and untreated tumors (third row). Calculating relative sizes of vim-hi versus vim-lo areas (mapped in red and green, fourth row) revealed a greater than 2-fold increase in vim-hi regions with cetuximab treatment (Figure 5D). These results strongly suggest that selective targeting of the Ecad-hi subpopulation via cetuximab enriched the mesenchymal-like subset, either through depletion of epithelial cells and/or increasing their differentiation toward a mesenchymal-like phenotype.
The observed therapy resistance of the Ecad-lo cells warranted investigation of their capacity to repopulate Ecad-hi components of tumors. To clarify developmental relationships between these two subpopulations, the phenotypic stability of each was tracked using clones of single SCC9 cells. Morphologically homogeneous colonies arising from single Ecad-hi or Ecad-lo cells were confirmed for purity based on exclusive E-cadherin or vimentin staining, and similar colonies were expanded and tracked for development of heterogeneity. Epithelial colonies arising from Ecad-hi cells rapidly reconstituted a mesenchymal-like subset, detectable within two weeks of plating at clonal density (Figure 6A). Mesenchymal-like colonies from Ecad-lo cells showed phenotypic stability upon initial expansion. However, these colonies reconstituted the epithelial subset on further growth, with early evidence of a small Ecad-hi subpopulation appearing at 4 weeks and expansion of this subset noted by 8 weeks (Figure 6B). These results indicated that the mesenchymal-like subpopulation is not terminally differentiated and suggested that it retains the plasticity to reconstitute other malignant subsets post-therapy.
In this study we demonstrate that mesenchymal-like malignant subpopulations contribute to chemotherapy resistance in SCCs with predominantly epithelial differentiation. Previous studies correlated drug resistance in carcinoma lines with increased expression of mesenchymal markers (Frederick et al., 2007; Ghoul et al., 2009; Shrader et al., 2007; Thomson et al., 2005; Yang et al., 2006; Yauch et al., 2005). However, analyzing lines as total populations does not account for the possible presence of epithelial and mesenchymal-like subsets, which may make disparate contributions to overall drug resistance. We suggest that SCCs in vivo typically do not possess uniformly epithelial or mesenchymal-like phenotypes; accordingly, the heterogeneity defined here in SCC cell lines was maintained by their in vivo counterparts. Consistent with this observation, a study examining several HNSCC histologic types revealed heterogeneous vimentin staining to be typical, with only a rare subtype, the “sarcomatoid” carcinoma, expressing uniformly high levels throughout (Mandal et al., 2008). At the other end of the spectrum, cell lines with high E-cadherin expression can still contain small vimentin-expressing subsets (Figure S1), and we note the same observation in xenografts of human HNSCC specimens (unpublished data). Nevertheless, it is unlikely that the precise markers used here to define the treatment resistant subpopulation will identify subsets with similar properties across all SCCs. We speculate that more subtle phenotypic transitions sharing key molecular traits with the ones documented here may be a basis for intrinsic treatment resistance across many SCC tumors.
In this study, intrinsic paclitaxel resistance of the mesenchymal-like subpopulation seemed attributable to its slower growth. However, cytotoxic drug resistance after EMT is likely more than a direct function of growth rate and instead reflects the outcome of gene-regulatory programs with complex relationships to proliferation, differentiation, and apoptosis. For instance, a recent study showed that paclitaxel induces snail and slug, which, in addition to being transcription factor mediators of EMT, also repressed promoters of key molecules involved in p53-mediated apoptosis (Kurrey et al., 2009). Thus, at least in vitro, paclitaxel likely depletes the epithelial subset by multiple mechanisms and may also contribute to enrichment of mesenchymal-like cells by promoting EMT. Similarly, adriamycin, a cytotoxic drug of differing mechanism, also enhances EMT and creates resistance to itself and other agents as a twist1-mediated phenomenon (Li et al., 2009b).
Resistance to cetuximab in the Ecad-lo subset here likely arose from reduced EGFR expression and resulting loss of MAPK and PI3K pathway regulation by the receptor. This correlation contrasts with the lack of positive association between EGFR over-expression and clinical cetuximab sensitivity in HNSCC (Kalyankrishna and Grandis, 2006). Our findings also differ with a study of hepatocellular carcinoma cell lines, where EGFR levels appeared independent of mesenchymal marker expression (Fuchs et al., 2008). However, EGFR expression had thus far been compared against mesenchymal features using bulk lines, where overall receptor levels may not reflect those of any mesenchymal-like subsets they contain.
Known resistance mechanisms to EGFR-targeted therapies (Bianco et al., 2005; Cooper and Cohen, 2009) provide context for understanding the cetuximab insensitivity observed here. A novel mechanism for acquired cetuximab resistance is ligand-independent EGFR function through down-regulation of surface receptor and elevated nuclear, cytoplasmic, and total receptor levels (Li et al., 2009a). This mechanism may partly explain the association in HNSCCs of EGFR gene amplification and poor prognosis (Chung et al., 2006; Temam et al., 2007), but the reduced surface and total EGFR here in Ecad-lo cells argues against this explanation for their resistance. An alternative explanation is switching to other receptor tyrosine kinases to restore downstream survival and proliferation signals. For instance, EGFR and ErbB2 expression were noted to segregate to different regions within ESCCs (Kawaguchi et al., 2007) and thus might serve comparable functions in distinct subpopulations. Also, EGFR down-regulation and coordinate up-regulation of ErbB2/ErbB3 in HNSCC are described in response to the EGFR-targeted small molecule gefitinib (Erjala et al., 2006). Kinase switching to receptors outside the EGFR family is observed in mesenchymal-like cell lines of non small cell lung cancers (NSLC) (Thomson et al., 2005) and is a plausible mechanism here. Notably, the EGFR activating mutations that sensitize NSLC to gefitinib (Gazdar, 2009) are largely absent in HNSCC (Temam et al., 2007), and thus sensitivity to this inhibitor is not anticipated in the face of cetuximab resistance.
Traits of the mesenchymal-like subpopulation in SCCs have implications in the wider discussion regarding origins of phenotypic heterogeneity within solid tumors. Specifically, it remains unclear how much intra-tumor heterogeneity arises from epigenetic differences versus genetic change driven by clonal evolution (Shackleton et al., 2009). The ability of epithelial and mesenchymal-like subsets to reconstitute each other from single cell clones, as shown here, suggests that these phenotypes are distinguished primarily by epigenetic alterations and not genotypic selection. The cancer stem cell hypothesis is one framework for explaining how an epigenetically distinct subpopulation may sustain tumor growth and resist drug therapy. We have elected here not to frame the mesenchymal-like subset explicitly within controversial and evolving definitions of cancer stem cells; however, this subset appears to maintain malignant potential and does not represent a terminally differentiated phenotype. The subpopulation in SCC may have functions analogous to the CD44+/CD24− stem-like subset in breast carcinoma on the basis of sharing its mesenchymal-like gene expression profile (Mani et al., 2008). If so, the in vitro plasticity of our subpopulations argues against a rigid developmental hierarchy originating with stem cells and ending in terminal differentiation, instead favoring one where phenotypes are dynamic and sensitive to microenvironments. It is possible that the mesenchymal-like subset in SCCs retains the phenotypic plasticity to repopulate other subpopulations post therapy.
In context of our findings, promoting phenotypic reversal of Ecad-lo cells through mesenchymal to epithelial transition (MET) may be a viable strategy for chemosensitization. Here pure mesenchymal-like clones of SCC lines showed initial resistance to MET but did restore the epithelial subpopulation spontaneously after extended culture. Experimental maneuvers that both promote MET and enhance drug sensitivity include down-regulation of Notch (Wang et al., 2009), induction of Raf-kinase inhibitor protein (Wu and Bonavida, 2009), knockdown of zeb-1 (Haddad et al., 2009), and induction of miR-200 microRNA family members (Adam et al., 2009; Gregory et al., 2008; Li et al., 2009c). Future studies will seek pharmacologic strategies for both specifically targeting the mesenchymal-like subpopulation in SCCs and promoting its phenotypic reversal.
Cell lines were maintained in 1:1 Dulbecco’s modified Eagle and Ham’s F12 media, with 400ng/ml hydrocortisone and 10% fetal calf serum. Genetic purity of cell lines was confirmed with an Identify Mapping Kit (Coriell Institute, Camden, NJ, USA). SCC9, SCC4, and SCC15 cells were obtained from the ATCC (CRL-1629, 1624, 1623). TE12, SCC13, TE1, TE9, TE8, and HCE4 cell lines are previously described (Okano et al., 2000; Opitz et al., 1998). The OCTT2 cell line was derived from a surgical specimen of an oral HNSCC in compliance with University of Pennsylvania Institutional Review Board-approved protocol #417200. Tumor cells purified from xenografts of this specimen were seeded at 5000 cells/cm2 on mitomycin C-treated 3T3 fibroblasts and cultured as described (Rheinwald and Beckett, 1981).
Non-obese diabetic/severe combined immunodeficient/interleukin-2 receptor γ-chain-deficient mice were used in all experiments. Animals were bred and utilized at the Wistar Institute animal facility under protocols approved by the institutional animal care and use committee. To generate xenografts from human SCC specimens, 1mm tumor fragments were placed in subcutaneous pockets through flank incisions in anesthetized mice. Growth Factor Reduced Matrigel (BD, Franklin Lakes, NJ, USA) was added, and incisions were closed with suture. Xenografts were utilized prior to 10 in vivo passages, and tumor volumes were measured as [length × width × thickness]. Xenografts of SCC9 cells were generated by subcutaneous injection of 2×106 cells in 100μl Matrigel. For drug treatment, 1mg cetuximab (Imclone, New York, NY, USA) or equivalent volume saline control was injected intraperitoneally every three days.
Images obtained using Nikon TE2000 and E600 microscopes were processed with ImagePro-Plusv6.2 and ACT-1 software using uniform settings within each experiment. For video microscopy, SCC9 cells cultured in 6-well plates were treated with paclitaxel or control dimethylsulfoxide (DMSO). Drug was removed after 4 hours, and medium was supplemented with 20 μg/ml propidium iodide (PI). Cell death (PI uptake) was monitored using a Nikon TE300 microscope configured with automated filter wheels and stage, and an environmental chamber. Three fields/well were captured at 10-minute intervals and sequenced into video using ImagePro-Plus.
IF staining was performed in 24-well plates or gelatin-coated glass chamber slides, as described (Smalley et al., 2005). Antibodies of the following specificities were used: Alexafluor488-E-cadherin (BD), phosphoERK1/2-Thr202/Tyr204 (pERK), phosphoAKT-Ser473 (pAKT) (Cell Signaling, Danvers, MA, USA), vimentin (AnaSpec, Fremont, CA, USA), vimentin (Dako, Carpinteria, CA). Secondary antibodies included alexafluor488-anti-rabbit IgG, alexafluor594-anti-human IgG, and alexafluor594-anti-rabbit IgG (Invitrogen, Carlsbad, CA, USA). Isotype-matched mouse and rabbit antibodies were used as controls. In signaling experiments, cells were serum-starved for 24 hours before treatment with 200ng/ml recombinant human EGF (Invitrogen) for 1 hour.
A FACSAria (BD) sorter was used for FACS. FC was performed using a FACSCalibur instrument (BD) and analyzed using WinMDIv2.9. Dead cells were removed by exclusion of either PI or 7-amino-actinomycin-D positive cells. Where required for intracellular staining, sorted cells were permeabilized with acetone, as described (Mancaniello and Carbonari, 2008). Cell cycle analysis was performed as previously described (Smalley et al., 2006). FC staining (Fang et al., 2005) was performed with the following human specific antibodies: fluorescein isothiocyanate (FITC)-Ki-67, allophycocyanin (APC)-E-cadherin (Biolegend, San Diego, CA, USA), phycoerythrin (PE)-vimentin (Abcam, Cambridge, MA, USA), FITC-EGFR (Santa Cruz Biotech., Santa Cruz, CA, USA), FITC mouse IgG1,κ control (BD), APC mouse IgG1 control, and PE mouse IgG1 control (BD). PKH-67 labeling was performed per supplier protocol (Sigma, St. Louis, MO, USA).
To FACS-purify tumor cells from xenografts, minced tumors were digested overnight at 4°C in culture medium containing 2mg/ml collagenase-I and 1mg/ml collagenase-IV. Suspensions were passed through 40μm filters and pretreated with rat anti-mouse CD16/32 (Fc-Block, BD). Mouse-derived cells were excluded by positive selection of human cells with mouse anti-human major histocompatibility class I (Abcam) and PE-anti-mouse IgG F(ab)2 secondary antibody (Sigma).
Formalin-fixed, paraffin-embedded specimens were cut in 5μm sections, and antigens were retrieved by boiling for 15 minutes in EDTA buffer (Lab Vision, Fremont, CA, USA). Staining was performed sequentially for E-cadherin and vimentin, using the Envision Detection Kit (Dako), followed by hematoxylin counterstain. Mouse anti-human E-cadherin (Dako) was used at 1:10 dilution and detected with 3′,3-diaminobenzidine (DAB). After re-quenching peroxidase activity, mouse anti-human vimentin (Dako) was used without dilution and detected using Vector VIP (V-VIP) chromogen (Vector, Burlingame, CA, USA). Specificity was confirmed using mouse IgG1 controls for each antibody. To generate pseudo-colored images, IHC micrographs were processed using Adobe Photoshop CS2. Color ranges corresponding to DAB and V-VIP-stained areas were separated using histogram analysis and color-replaced with green and red, respectively. Images in each experiment were batch-processed with uniform color-replacement settings using Photoshop Bridge. Image-based quantitative analysis of E-cadherin versus vimentin staining areas was performed with ImagePro-Plus, using the Count/Size tool. Two color masks were created using color cube analysis to separate labeled components based on spectral distribution. The count tool was then used to quantify relative percentages of E-cadherin versus vimentin staining areas. Masks were copied to black backgrounds to create the displayed images. Batch-processing ensured unbiased comparison of groups.
Clonogenicity was measured by seeding 6-well plates at 1,000 cells/well. After 7 days, colonies were stained with 0.5% crystal violet in 25% methanol and counted on high resolution digital images. Methylthiazonletetrazolium (MTT) assays were performed by seeding 3,000 cells/well (OCTT2) or 5,000 cells/well (SCC9) on 96-well plates, unless otherwise noted. Growth was quantified using a MTT Proliferation Kit (Invitrogen). Optical density in each well was measured at 590nm (OD-590nm), and values were normalized relative to OD-590nm for non-treated controls in drug treatment experiments.
In three independent experiments, Ecad-hi and Ecad-lo subpopulations were sorted, and RNA was extracted using an RNAeasy Kit (Qiagen, Valencia, CA, USA) to generate triplicate samples. A TotalPrep RNA Amplification Kit (Ambion, Austin, TX, USA) generated biotinylated cRNA, which was hybridized and analyzed on Illumina HumanHT-12v3 Beadchips (Illumina, San Diego, CA, USA) per manufacturer protocols. Raw data underwent variance-stabilizing transformation and quantile normalization using the Bioconductor Lumi package (Du et al., 2008). Probes below background level (detection P value <0.01) were excluded, and differential expression was identified with Bayes-adjusted variance analysis using the Bioconductor Limma package (Smyth, 2004). Gene identifications were made using false discovery rate adjusted P values of <0.05. Raw data is made available under Gene Expression Omnibus #18722.
Total cellular protein was extracted and blotted as described (Smalley et al., 2005) using antibody to human EGFR (Santa Cruz). After analysis, western blots were stripped once and reprobed for β-actin to assess even protein loading.
Data points with error bars show means ± standard error of mean (SEM) based on triplicate values. Differences are analyzed between individual data points by paired Student’s t-test and between curves by ANOVA.
Grant support: NIH/NCI P01 CA098101 (M. Herlyn, A. Rustgi, and D. Basu) and ACS IRG-78-002-30 (D. Basu).
We acknowledge Fredrick Keeny in the Wistar Institute Microscopy Core for assistance with digital image processing and Ademi Santiago-Walker, PhD for critical review of the manuscript. This work is supported by grants from the NIH (NCI P01 CA098101) and the American Cancer Society (IRG-78-002-30). Work is also supported in part with resources and use of facilities at the Philadelphia VA Medical Center.
Conflict of Interest
All authors declare no conflict of interest.