Pancreatic cancer is often detected late, when curative therapies are no longer possible. Here, we present non-invasive detection of pancreatic ductal adenocarcinoma (PDAC) by 5-hydroxymethylcytosine (5hmC) changes in circulating cell free DNA from a PDAC cohort (n = 64) in comparison with a non-cancer cohort (n = 243). Differential hydroxymethylation is found in thousands of genes, most significantly in genes related to pancreas development or function (GATA4, GATA6, PROX1, ONECUT1, MEIS2), and cancer pathogenesis (YAP1, TEAD1, PROX1, IGF1). cfDNA hydroxymethylome in PDAC cohort is differentially enriched for genes that are commonly de-regulated in PDAC tumors upon activation of KRAS and inactivation of TP53. Regularized regression models built using 5hmC densities in genes perform with AUC of 0.92 (discovery dataset, n = 79) and 0.92–0.94 (two independent test sets, n = 228). Furthermore, tissue-derived 5hmC features can be used to classify PDAC cfDNA (AUC = 0.88). These findings suggest that 5hmC changes enable classification of PDAC even during early stage disease.
Pancreatic cancer often presents late and has few symptoms, at which point only 10–20% of patients are eligible for surgical resection1. Pancreatic ductal adenocarcinoma (PDAC) constitute more than 90% of all pancreatic cancer cases2 with the next most common sub-type being neuroendocrine tumors1. Tobacco smoking confers a two- to three-fold higher risk of pancreatic cancer, while contributing to approximately 15–30% of cases1, with smokers diagnosed 8 to 15 years younger than non-smokers3,4. Family history is contributory in ~10% of cases, and germline mutations in genes such as BRCA2, BRCA1, CDKN2A, ATM, STK11, PRSS1, MLH1 and PALB2 are associated with pancreatic cancer with variable penetrance1. Translational research using genomic and proteomic technologies has provided molecular insights into the pathogenesis and biology of pancreatic cancer but has yet to yield robust diagnostic biomarkers to impact early diagnosis of disease, as reflected by a low overall 5-year survival rate of 10%1,2.
The management of PDAC presents physicians with challenges along the entire clinical spectrum, including early detection in high risk individuals, early diagnosis of patients with symptoms or imaging findings, prognostication of outcomes and prediction of therapeutic responsiveness. Collectively, these factors have engendered intensive efforts in translational research to identify and validate biomarkers with sufficient clinical performance metrics to improve decision algorithms and resultant clinical outcomes. Current guidelines in PDAC management are limited to two biomarker recommendations for detecting disease presence assayed in an invasive fashion from cystic fluid. First, carbohydrate antigen 19-9 (CA 19-9) guides surgery decisions, use of adjuvant therapy, or the detection of post-operative tumor recurrence, however, its utility is limited because 10% of patients do not secrete the antigen5. Second, carcinoembryonic antigen (CEA) concentration determination from cyst fluid is used to distinguish higher risk mucinous from non-mucinous cysts6,7. CA19-9 levels can also be measured by a blood test, however blood levels of CA19-9 were not found to be sensitive or specific enough for reliable detection of pancreatic cancer8.
Among the inherited risk factors for pancreatic cancer are genomic mutations such as BRCA2, which confers a 3.5-fold higher risk in carriers, with the probability of a germline mutation between 6 and 12% in PDAC patients with a first-degree relative diagnosed with PDAC9. Molecular analyses of pancreatic cancer genomes have further revealed activating mutations in KRAS and inactivation of CDKN2A, TP53 and SMAD4, either through point mutation or copy number changes at >50% population frequency10,11,12. However, mutational heterogeneity, coupled with lack of disease specificity due to pleiotropy render this subset of genes incomplete for the diagnosis of patients. Molecular subtyping of pancreatic tumors using mutational-based data11 or gene expression signatures13,14,15 have not yet seen clinical applicability. Other forms of molecular profiling have focused on epigenetics, namely chromatin-based post-translational modifications and the methylation status of cytosine bases in DNA.
Control of DNA state and chromatin regulation have been observed to underpin the onset and progression of oncologic disease16,17. DNA methylation status of cytosine bases has been shown to associate with transcriptional regulation of gene expression. DNA methylation in promoters is associated with gene silencing whereas demethylation is associated with gene activation18. Gene body methylation, on the other hand, is correlated with increased expression19. More recently, detailed understanding of demethylation has been enabled with precision around intermediate states during active demethylation20,21. Specifically, discovery of TET enzyme-mediated methyl-cytosine oxidation to 5-hydroxymethyl cytosine (5hmC) has yielded signatures that enable definition of cellular states22, as well as identification of cancer in cell free DNA23,24,25.
Molecular signatures in circulating cell free DNA (cfDNA) based on cytosine 5-hydroxymethylation have been shown previously to potentially define the tissue of tumor origin in a variety of disease types23. Therefore, we embarked on a case–control study aimed at investigating whether DNA 5hmC signatures were present in the blood of PDAC patients compared to a cohort of non-cancer individuals. We also investigated whether these signatures enable discrimination between cancer and non-cancer patients.
We find that in our study population, PDAC patients possess thousands of genes with an altered hydroxymethyl profile compared to non-cancer individuals. Furthermore, filtering to those genes with the most differentially hydroxymethylated states reveals genes that have been previously implicated in pancreas development or pancreatic cancer. This biologically significant gene set performs well in the construction of predictive models to discriminate PDAC from non-disease, suggesting that the measurement of 5hmC in cfDNA merits further investigation for the detection and classification of PDAC.
Clinical cohort and study design
Plasma specimens from 307 subjects with or without a diagnosis of PDAC were collected at multiple institutions in different geographic regions of the United States. These PDAC (n = 64) and non-cancer (n = 243) patient samples satisfied the study inclusion criteria, which included male and female subject age of minimum 40 years old with a tolerance of 5% of patients younger than 40 years old, as well as confirmed pathologic diagnosis of adenocarcinoma of any subtype at the time of biopsy or surgical resection for subjects in the cancer cohort. The non-cancer cohort was identified as satisfying the study inclusion criteria and patients were specifically negative for any form of cancer. Neither cohort were being treated with medication for disease at the time of blood collection, which was prior to any biopsy or surgical resection in the cancer cohort. Discovery dataset consisted of 41 PDAC and 38 non-cancer samples from and the remaining samples were used for validation. There were no statistically significant differences in subject age, gender or tobacco exposure between the two cohorts used for discovery (Table 1). Early stage PDAC patients (Stages I & II) made up 56% of the PDAC cohort.
Genomic distributions of 5hmC in PDAC and non-cancer cohort
To gain an understanding of the genomic regions associated with hydroxymethylation in cfDNA, we first determined 5hmC enriched loci, as measured by increased read density and subsequent detection as peaks by MACS226. The vast majority of 5hmC loci occur in non-coding regions of the genome, over introns and intergenic loci some of which overlap with SINE repetitive elements, with no preferential distribution in the PDAC or non-cancer cohort (Supplementary Fig. 1A). However, 5hmC are not particularly enriched over these regions relative to the genome background (Fig. 1a). Instead, 5hmC enrichment is observed over genic features, most significantly in promoters, 5′UTRs, 3′UTRs, exons, transcription termination sites (TTS) and SINE repetitive elements that are located in gene-rich regions, as measured by increased relative fold change compared to the genome background (Fig. 1a). These results indicate that 5hmC in cfDNA is preferentially enriched in genic regions, consistent with previously published reports27.
Comparison of 5hmC peaks in PDAC to the non-cancer cohort revealed significant differences. First, peaks detected per million reads in PDAC cfDNA cohort was significantly less than in non-cancer cohort (Fig. 1b). Decreased number of peaks suggests global decrease in 5hmC in PDAC, consistent with previous reports investigating tissue samples. Second, 5hmC peak enrichment was increased in PDAC over 3’UTR, TTS and intron regions whereas it was decreased over promoters (Fig. 1c). These global changes, observed in a statistically significant manner in each cohort, were also detected in various cancer stages, including early stage cancers (Supplementary Fig. 1B).
Next, we investigated 5hmC occupancy, and its associated changes in PDAC, with respect to chromatin state. For this purpose, we first generated histone maps of primary tumor tissues obtained from two different PDAC patients with chromatin immunoprecipitation followed by sequencing. Targeting post-translational modifications such as methylation and acetylation on histone H3 that define various functional regions, we segmented the chromatin into 15 chromatin states, that identify actively transcribed and silent regions, as well as regulatory regions, using chromHMM28 (Fig. 2a). In parallel, we profiled the 5-hydroxymethylome of primary PDAC tumor tissues from 17 PDAC patients and found that they overlapped most with the active TSS as well as active enhancer regions (Supplementary Fig. 2A), indicating that 5hmC marks regulatory regions with active transcription. Comparison of 5hmC occupancy in PDAC cfDNA and non-cancer cfDNA cohorts revealed statistically significant differences in these chromatin regions, with decreased 5-hydroxymethylation in PDAC cohort over active TSS and flanking TSS regions, while increased 5-hydroxymethylation was observed over weakly transcribed regions (Fig. 2b). 5hmC decrease over H3K4me3-marked active TSS sites was observed across all cancer stages (Fig. 1c and Supplementary Fig. 2B and C). These results suggest that differential 5hmC enrichment observed over promoters (Supplementary Fig. 1B) are driven by transcriptional activation. Overall, differential cfDNA hydroxymethylation over different chromatin contexts identified in tumor tissue, suggests that elements of epigenetic dysregulation in cancer cells can be picked up in the cfDNA 5hmC signal.
Identification of disease specific genes from plasma samples
Differential analysis of 5hmC densities in genes using an adjusted p-value (Benjamini–Hochberg method) threshold of 0.05, revealed 5700 hyper- and 6155 hypo-hydroxymethylated genes in PDAC compared to non-cancer samples (Fig. 3a). Further filtering of this gene set using a more stringent criteria (absolute fold change ≥1.5 and average log2 CPM ≥3.5) resulted in 577 upregulated and 217 downregulated genes. Among the genes with increased 5hmC density in PDAC were those related to pancreas development (GATA429, GATA629, PROX130, ONECUT131, and MEIS232) and/or implicated in cancer (YAP133, TEAD133, PROX134, ONECUT2, ONECUT1, and IGF1) (Fig. 3b). Inspection of the MSigDB for cancer relevant gene sets, C6.Oncogenic signatures and C4.Cancer modules, enriched among the 577 genes with increased 5hmC densities revealed a preponderance of gene sets that are upregulated in both KRAS and TP53 mutant cancers (Fig. 3c). These genes were also enriched in targets of transcription factors known to be involved in PDAC oncogenesis or metastasis, like NFAT and FOXA (HNF3) (Table 2). In contrast, the most significantly downregulated 217 genes in PDAC cfDNA cohort was enriched for gene sets that are downregulated in KRAS mutant cells as well as immune response and whole blood genes (Fig. 3c). These results suggest that 5hmC profiling can capture PDAC tumor relevant biological signals in plasma.
Multidimensional scaling (MDS) analysis using either the 11,855 genes with high variation in 5hmC counts (Fig. 3d) or the 794 genes filtered at the extremes of 5hmC representation in PDAC (Fig. 3e), reveal partitioning of the PDAC samples from the non-cancer equally well. We then tested the partitioning of a previously published dataset23 using the differentially represented genes we identified. This dataset, despite small cohort size, had a similar cancer stage distribution as our discovery dataset (Supplementary Fig. 3B). Hierarchical clustering using these 794 genes revealed partitioning of the 5hmC data from PDAC and non-cancer cfDNA from Song et al.23 as well as the discovery cohort (Supplementary Fig. 3A, C). Consistently, PDAC samples in Song et al. could be separated from non-cancer samples using these 794 genes as shown by the MDS plot (Fig. 3f). In summary, we have been able to identify a differentially represented gene set whose biological functions are congruent with both pancreatic development and cancer. Furthermore, 5-hydroxymethylation densities of these genes alone enable the distinction of PDAC from non-cancer.
Predictive models for detection of pancreatic cancer in cfDNA
We performed regularized logistic regression analysis in order to determine whether gene-based features are present in the PDAC and non-cancer cohorts that can enable the classification of patient samples. We employed top 65% genes with the most variable 5hmC density for model selection. Elastic net35 was utilized as the regularization method. Other modeling approaches, such as random forest, support vector machines and neural networks, were explored in a preliminary analysis and were found to have inferior cross-validated performance on the training data (data not shown).
Elastic net35 regularization method requires specifying hyper-parameters that control the level of regularization used in the fit. These hyper-parameters were selected based on out-of-fold performance on 30 repetitions of 5-fold cross-validated analysis of the training data. Out-of-fold assessments are based on the samples in the left-out fold at each step of the cross-validated analysis. The training set yielded an out-of-fold performance metric, area under the ROC curve (AUC), of 0.919 (Fig. 4a). The distribution of probability scores for each sample indicated few false negatives in the PDAC cohort and false positives in non-cancer cohort, assuming a threshold cutoff of 3rd quartile of the non-cancer (Fig. 4b). Inspection of features that were selected by the predictive model revealed cancer relevant genes, such as the cancer antigen family gene BAGE536 and transcriptional co-repressor RUNX1T137. On the other hand, model features that were downregulated in PDAC cfDNA compared to non-cancer cohort were enriched for immune/blood cell relevant genes such as SLFN14 which is important for platelet formation38 and CD22 which is expressed in B cells39 (Fig. 4c).
Next, the trained model was tested on two independent validation sets of patient samples. The first validation dataset was generated by 5hmC profiling of 23 PDAC and 205 non-cancer cfDNA samples, as described in methods section. This independent validation dataset yielded a classification performance AUC of 0.921 (Fig. 4d). A second validation set included pancreatic cancer and non-cancer samples from Song et al.23 which was profiled for 5hmC using a pull down method similar to the one used in this study (pancreas subtype specified as adenocarcinoma, 7 pancreas cancer, 10 non-cancer). This validation set exhibited a performance AUC of 0.943 (Fig. 4e).
Correlation of prediction performance with CA19-9
We next investigated the performance of 5hmC-based prediction probabilities with relationship to plasma levels of CA19-9 (Cancer Antigen 19-9), which is a clinically relevant biomarker in pancreatic cancer. Despite being one of the most clinically utilized PDAC biomarkers, it is well established that CA19-9 levels in blood have challenges associated with specificity and sensitivity. Consistent with these previous observations, we found that CA19-9 level was abnormally high in one non-cancer sample (200 U/ml) and was within normal range for some Stage I, Stage II and even Stage III PDAC samples (Fig. 4f). Interestingly, high probability scores calculated by our predictive model allowed detection of these early stage, namely Stage I and Stage II PDAC samples, that had low CA19-9 levels (8 out of 30 samples) (Fig. 4f). On the other hand, probability scores of some PDAC samples were low despite high CA19-9 levels. Taken together, these results suggest that 5hmC signals can significantly improve detection on existing methods for both sensitivity and specificity, particularly for early stage PDAC.
Prediction performance with tissue-derived features
Next, we wanted to explore whether we can detect tumor-originated 5hmC features in cfDNA. For this purpose, we first profiled 5hmC in 17 PDAC tumor tissues. We then ranked all the genes based on FPKM values in these tissue profiles and took two gene sets; one representing the highest level of 5hmC occupancy (top 50 hyper-hydroxymethylated genes) and another set that represents the lowest levels of 5hmC occupancy (top 50 hypo-hydroxymethylated genes) in PDAC tissue (Fig. 5a). PDAC tissue-derived top 50 hyper-hydroxymethylated genes can separate non-cancer cfDNA from PDAC cfDNA samples well (Fig. 5b, top panel). In contrast, non-cancer and PDAC cfDNA samples did not cluster separately when top 50 hypo-hydroxymethylated gene set was used as features (Fig. 5b, bottom panel). Consistent with these findings, a prediction model built using hyper-hydroxymethylated gene set performed well with an AUC of 0.88 in classifying PDAC and non-cancer cfDNA samples correctly (Fig. 5c, coral line), unlike the model that used hypo-hydroxymethylated gene set as features, which had an AUC of 0.57 (Fig. 5c, dotted coral line). While the model trained with cfDNA 5hmC profiles performed best with an AUC of 0.919 (Fig. 5c, teal line), inspection of normalized 5hmC signal (RPKM) from 37 features selected in cfDNA model demonstrates that PDAC cfDNA signal is overall admixed between non-cancer cfDNA and PDAC tissue (Fig. 5d). Taken together, our results indicate that PDAC tumor tissue-derived features are useful in classification of PDAC in cfDNA, suggesting that tumor-derived epigenomic signals are retained in the cfDNA compartment.
Pancreatic cancer is the deadliest form of cancer with 10 percent five-year survival rate40. A major factor behind such abysmal survival rate is the difficulty in diagnosing patients early when tumors can be surgically removed. This study was focused on the discovery of hydroxymethylation-based biomarkers in cfDNA that may facilitate the development of molecular diagnostic tests to detect pancreatic cancer at not only late but also early stages. 5hmC-based methods were previously reported to have potential for cancer detection from plasma samples, particularly in the context of lung cancer, hepatocellular carcinoma23, colon and gastric cancer25. Furthermore, differential 5hmC profiles, albeit from limited number of pancreatic cancer patients, suggested such an approach could be possible for pancreatic cancer23. Early stage detection from plasma have proved to be difficult for approaches that depend solely on tumor originating DNA, such as mutational analysis, due to minute levels of circulating tumor DNA present at early stage disease. Methods such as DNA methylation or hydroxymethylation profiling, on the other hand, has the potential to leverage all signals in the plasma, including the ones that originate from immune cells, a major contributor of cfDNA41, which can, in turn, improve detection for early stage cancers. Indeed, DNA methylation-based methods have recently shown promise in cancer detection42,43. Our data show that pancreatic cancer detection at early stages is possible with 5hmC-based methods.
Our data highlight the ability to detect differentially hydroxymethylated genes whose underlying biology shows association with both pancreas and cancer development as well as established trends in chromatin mark maps and other functional regions of the genome. Furthermore, regularized regression was used to build a predictive model from a comprehensive gene set that is highly variable, yielding an AUC of 0.919 along with two independent external dataset validations with AUC of 0.921 and 0.943.
The 5hmC signal was readily found to overlap in gene-centric functional regions (enrichment in promoter, exons, UTR and TTS), as well as transposable elements like SINEs (enriched) and LINEs (depleted) (Fig. 1a). Globally, PDAC cfDNA cohort had decreased number of peaks compared to non-cancer cfDNA cohort (Fig. 1b), consistent with previous reports of decreased 5hmC in several types of cancer, including pancreatic cancer44. Indeed, decreased 5hmC was recently linked to malignant transformation in KRAS mutant pancreatic cells upon deactivation of p53, which are commonly observed in PDAC patients45. Hydroxymethylcytosine changes in functional regions have also been reported in cfDNA from colorectal25, esophageal24,46 and lung cancer24. Consistent with these reports, we observed decreased number of peaks in PDAC cfDNA relative to non-cancer cfDNA. Furthermore, we report PDAC specific gains or losses in hydroxymethylation in functional regions in our data. PDAC specific 5hmC increase in 3’UTR, TTS and exons and 5hmC decrease in promoters detectable in cfDNA (Fig. 1c). These changes were also observed in various pancreatic cancer stages (Supplementary Fig. 1). In embryonic stem cells, 5-hydroxymethylation decreases in the promoter region have been shown to associate with elevated gene transcription27. An increase in disease relevant transcription is implicitly supported in our PDAC data by the 5hmC increase in gene-centric features mentioned earlier, as well as an apparent decrease of 5hmC in promoter regions (Fig. 1c). Taken together, disease specific remodeling of active demethylation in PDAC patients is captured via changes in 5hmC representation.
Dynamic changes in chromatin have been shown to control cell development and transition of cells with oncogenic potential47. Intersection of our 5hmC data with various chromatin states determined by ChIPseq in PDAC primary tumor tissues revealed 5hmC localization in active chromatin regions, most significantly active TSS and active enhancer regions (Fig. 2a). Consistent with 5hmC changes over promoters, 5hmC decrease in PDAC cfDNA in active TSS regions also suggests disease specific increases in gene transcription via chromatin modifications, given the permissive transcriptional state associated with H3K4me348. Furthermore, we observed 5hmC decrease in weak enhancer regions identified by H3K27ac and H3K4me1 (Fig. 2a). While 5hmC patterning around known functional elements of the genome suggests a broader interplay between hydroxymethylation and the epigenetic control of transcriptional processes, these results also indicate that 5hmC in cfDNA can potentially be utilized for non-invasive monitoring of epigenomic dysregulation in PDAC. Additional work will reveal the extent to which models predictive of PDAC can be built from a combination of gene-specific features, genomic loci with different chromatin states and transposable elements detected in cfDNA.
In this study, we employed aggregate quantification of hydroxymethylation at gene level in PDAC, and yet, were able to find genes and other functional regions with changes in 5hmC signals that highlighted pathways implicated in pancreatic cancer (Fig. 3c). The majority of PDAC cancers harbor activating mutations in KRAS (~90%) and inactivating mutations in TP53 (~70%)49. Gene set enrichment analysis for the genes with increased 5hmC representation in gene body revealed several gene sets that are upregulated when KRAS is up or when p53 is down (Fig. 3c left panel). Furthermore, among genes with increased 5hmC were targets of transcription factors NFAT and FOXA (HNF3) (Table 2), previously reported to be involved in promoting pancreatic cancer initiation50 and metastasis51, respectively, via enhancer reprogramming. Investigation of genes with decreased 5hmC in PDAC cfDNA as compared to non-cancer cfDNA indicated enrichment of genes downregulated when KRAS is up. Genes related to whole blood and immune response were enriched among the genes with decreased 5hmC in PDAC cfDNA (Fig. 3c right panels). This would be consistent with an increase in (tumor) tissue derived DNA in cfDNA in PDAC patients, diluting immune and blood cell derived DNA that make up the majority of cfDNA in non-cancer individuals41. These results, taken together, suggest that PDAC tissue derived signals can be detected in cfDNA from cancer patients using 5hmC.
Inspection of individual genes that were either significantly increased or decreased in 5hmC density revealed genes implicated in normal pancreas development, for instance the transcription factors GATA4, GATA6, PROX1, ONECUT1/2, in addition to genes whose increased expression is implicated in cancer, such as YAP1, TEAD, PROX1, ONECUT2, ONECUT1 and IGF1. The relative 5hmC increase in transcription factor genes like GATA4, GATA6, PROX1, ONECUT1/2, MEIS2, which were previously reported to be involved in early pancreatic development29,30,31, suggest a reversion to a stem-like state in PDAC samples.
Genes with the most significant increase in 5hmC in PDAC cfDNA are enriched in annotated relevant biology which can be used to build regularized regression models with a high performance (training AUC of 0.919 with external dataset validation AUCs of 0.921 and 0.943). This gives us good confidence that our models are measuring underlying biological signals relevant to PDAC. One such signal is the cancer antigen BAGE that is selected among the 37 features in our model.
Despite the large number of differentially hydroxymethylated genes identified in PDAC cfDNA compared to non-cancer cfDNA, the regularized regression model with only 37 genes was sufficient to perform well for classification of cfDNA. However, 13,180 differentially hydroxymethylated genes detected in PDAC cfDNA compared to non-cancer cfDNA suggest that other biological signals may also reside in our dataset. Future work is needed to understand the impact of other biological factors on differential hydroxymethylation in PDAC cfDNA.
Smoking status is a known risk factor for PDAC up to 20 years post smoking cessation and DNA methylation changes have been associated with tobacco-based toxins52. In our prospective case–control designed study, ever smokers constituted 51.2% and 55.3% of PDAC and non-cancer cohorts respectively, indicating that ever smokers are well represented in each cohort. Consequently, we do not believe that smoking association in our PDAC cohort could account for the significantly hydroxymethylated genes found. Indeed, statistical adjustment for genes affected by smoking results in comparable performance for predictive models (data not shown). However, a more extensive future study focused on sub-partitioning PDAC and non-cancer patient into never and ever smokers with pack-year characteristics will enable us to address the impact of smoking on the hydroxymethylome in PDAC patients. Furthermore, high specificity is crucial to achieve in the clinical setting for detection of cancers with low incidence rate such as pancreatic cancer. Pancreatic cancer risk parameters combined into a clinically relevant, intent-to-test population-based study, will allow testing of our findings beyond our current case–control cohort study, which numbers less than 100 participants. Further consideration of disease-related clinical parameters will enable us to explore hydroxymethylcytosine features with the aim of yielding refined signals capable of earlier diagnosis of PDAC.
Clinical cohorts and study design
A case–control study was performed using plasma obtained from subjects without (termed non-cancer) and with pancreatic cancer. Patients were enrolled from participating sites in the United States at which informed consent was obtained and biospecimens collected as approved by the Institutional Review Boards (IRBs) responsible at each site (Sterling IRB or WIRB, Supplementary Table 1). The study protocol submission, IRB approval and specimen handling across all sites were managed by MT Group (Van Nuys, CA), who provided clinical research specimen handling services.
Plasma samples for the cancer cohort were obtained from subjects who had undergone management for pancreatic cancer in the United States, and also provided consent for use of blood specimens for archival storage and retrospective analyses.
Criteria for subject eligibility for inclusion in the analysis included male and female subject age of minimum 40 years old with a tolerance of 5% of patients younger than 40 years old, with additional requirements for the cancer cohort including: (1) no cancer treatment, e.g., surgical, chemotherapy, immunotherapy, targeted therapy, or radiation therapy, prior to study enrollment and blood specimen acquisition; and (2) a confirmed pathologic diagnosis of adenocarcinoma inclusive of all subtypes.
Subject exclusion criteria for the non-cancer cohort also included any of the following: prior cancer diagnosis within prior six months; surgery or invasive procedure requiring general anesthesia within prior month; non-cancer systemic therapy associated with molecularly targeted immune modulation; concurrent or prior pregnancy within previous 12 months; history of organ tissue transplantation; history of blood product transfusion within one month; and major trauma within six months. Clinical data required for all subjects included age, gender, smoking history, and both tissue pathology and grade, and were managed in accordance with the guidance established by the Health Insurance Portability and Accountability Act (HIPAA) of 1996 to ensure subject privacy.
Plasma was isolated from whole blood specimens obtained by routine venous phlebotomy at the time of subject enrollment. For both cancer and non-cancer control subjects, whole blood was collected in Cell-Free DNA BCT® tubes according to the manufacturer’s protocol (Streck, La Vista, NE) (https://www.streck.com/collection/cell-free-dna-bct/). Tubes were maintained at 15 °C to 25 °C with plasma separation performed within 24 h of phlebotomy by centrifugation of whole blood at 1600 x g for 10 min at RT, followed by transfer of the plasma layer to a new tube for centrifugation at 16,000 x g for 10 min. Plasma was aliquoted for subsequent cfDNA isolation or storage at −80 °C.
cfDNA was isolated using the QIAamp Circulating Nucleic Acid Kit (QIAGEN, Germantown, MD) following the manufacturer’s protocol excepting the omission of carrier RNA during cfDNA extraction. Four milliliter plasma volumes were lysed for 30 min prior to collection of nucleic acids. Eluates were collected in a volume of 60 µl buffer. All cfDNA eluates were quantified by Bioanalyzer dsDNA High Sensitivity assay (Agilent Technologies, Santa Clara, CA) and Qubit dsDNA High Sensitivity Assay (Thermo Fisher Scientific, Waltham, MA) was employed to ensure the absence of contaminating high molecular weight DNA emanating from white blood cell lysis.
Tissue and genomic DNA processing
All tissue samples were stored in H media for the interval between surgical resection and laboratory processing. Each sample was weighed and aliquoted into sections of approximately 35 mg. Each resulting subsection was briefly incubated on dry ice, then homogenized in 500 µl RLT Buffer Plus using a Tissue Lyser LT (QIAGEN Germantown, MD) at 50 Hz for two minutes. Resulting homogenates were stored at −80 C until DNA extraction. Genomic DNA was extracted using DNeasy Blood & Tissue Kit (QIAGEN Germantown, MD) according to the manufacturer instructions. Genomic DNA eluates were quantified using the Qubit dsDNA High Sensitivity assay (Thermo Fisher Scientific, Waltham, MA) and stored at −20 °C until further processing. Prior to sequencing library construction, genomic DNA was fragmented to a modal 150 base pair size using an ME220 focused ultrasonicator (Covaris, Woburn, MA), Modal fragmented DNA sizes were verified using the TapeStation 2200 dsDNA high sensitivity assay (Agilent Technologies, Santa Clara, CA) and quantified as described above prior to commencing library construction.
5-hydroxymethyl Cytosine (5hmC) enrichment assay
35cfDNA was normalized to 10 ng total input for each assay and ligated to sequencing adapters. 5hmC bases were biotinylated via a two-step chemistry and subsequently enriched by binding to Dynabeads M270 Streptavidin (Thermo Fisher Scientific, Waltham, MA). All libraries were quantified by Bioanalyzer dsDNA High Sensitivity assay (Agilent Technologies, Santa Clara, CA) and Qubit dsDNA High Sensitivity Assay (Thermo Fisher Scientific, Waltham, MA) and normalized in preparation for sequencing.
DNA sequencing and alignment
DNA sequencing was performed according to manufacturer’s recommendations with 75 base-pair, paired-end sequencing using a NextSeq550 instrument with version 2 reagent chemistry (Illumina, San Diego, CA). Data were collected using NextSeq System Suite 2.2.04. Twenty-four libraries were sequenced per flowcell. Raw data processing and demultiplexing was performed using the Illumina BaseSpace Sequence Hub to generate sample specific FASTQ output. Sequencing reads were aligned to the hg19 reference genome using BWA-MEM with default parameters53. Sequencing data quality was assessed using picard54.
BWA-MEM read alignments were employed to identify regions or peaks of dense read accumulation that mark the location of a hydroxymethylated cytosine residue. Prior to identifying peaks, BAM files containing the locations of aligned reads were filtered for poorly mapped (MAPQ < 30) and not properly paired reads using samtools and HTSlib55. 5hmC peak calling was carried out using MACS2 (https://github.com/taoliu/MACS) with a p-value cut off = 1.00e−5. Identified 5hmC peaks residing in “blacklist regions” as defined elsewhere (https://sites.google.com/site/anshulkundaje/projects/blacklists) and residing on chromosomes X, Y, and mitochondrial genome were also removed using bedtools56. Computation of genomic feature enrichment overlap 5hmC peaks were performed using HOMER software (http://homer.ucsd.edu/homer/) with default parameters.
Chromatin immunoprecipitations of H3K4me1, H3K4me3, H3K27ac, H3K36me3, H3K9me3, and H3K27me3 in primary PDAC tumor tissues were performed at Active Motif (Carlsbad, CA). Briefly, tumor tissues were homogenized, then sonicated and subjected to chromatin immunoprecipitation with antibodies specific to chromatin modifications mentioned above (anti-H3K4me1 Active Motif 39297, 4 μl per IP; anti-H3K4me3 Active Motif 39159, 3 μl per IP; anti-H3K9me3 Abcam ab8898, 5 μl per IP; anti-H3K27ac Active Motif 39133, 4 μg per IP; anti-H3K27me3 Active Motif 39155, 4 μg per IP; anti-H3K36me3 Active Motif 61101, 4 μg per IP). Immunoprecipitated DNA was isolated, then subjected to the library preparation and was subsequently sequenced. Reads were mapped using BWA-MEM, then filtered for quality reads as described above. Peaks for each histone modification was determined using MACS2 with default parameters for H3K4me1, H3K4me3, and H3K27ac; while –broad option was used for H3K9me3, H3K27me3, and H3K36me3. ChromHMM was run with all 6 histone ChIPseq mentioned above28. For comparisons between PDAC and non-cancer, two-sided Wilcoxon test was used, and for across stages comparison, two-sided Kruskal–Wallis test was employed. Genomic regions were visualized using IGV57.
Differential representation analysis
For the purpose of reliably identifying gene bodies with differential representation between the PDAC and the non-cancer groups, we closely followed the RNA-Seq workflow outlined in Law et al.58, including much of the preliminary QC steps, using R59. In brief, the analysis includes data pre-processing by adopting the following workflow: (i) transforming the data from raw counts to log2(counts per million), (ii) removing genes that are weakly represented, (iii) normalizing the gene representation distributions, and (iv) performing unsupervised clustering of samples. To accomplish differential representation analysis, we applied the following steps: (i) creating a design matrix to contrast PDAC versus non-cancer cohorts, (ii) removing heteroscedasticity from the data, (iii) fitting regression models for the comparison of interest, PDAC vs non-cancer, (iv) examining the number of differentially represented genes. In most of these analysis steps the default settings were used when appropriate. To remove weakly represented genes, we excluded genes that did not have greater than 3 counts per million reads in at least 20 samples. This filter excludes roughly 12% of the genes. For the identification of the significantly differentially represented regions, we used the method of Benjamini and Hochberg60 to obtain p-values adjusted for multiple comparisons. In this report, we use adjusted p-value and false discovery rate (FDR) interchangeably.
For the purpose of assessing the feasibility of building classifiers that can discriminate between PDAC and non-cancer samples based on the 5hmC representation of gene bodies, we used elastic net, which is commonly used in the classification context, where the number of examples are few and the number of features are large. See Friedman et al.35 for a description of the general Elastic net procedure. Software implementation of these methods can be found at https://cran.r-project.org/web/packages/glmnet/index.html. Weakly represented genes were excluded from analysis as described in the section on “Differential representation analysis”.
All training and fitting were done on 80% of the samples selected at random in a balanced way to keep the ratio of the number of PDAC to non-cancer samples similar in both the training and testing subsets. Before any fitting, genes were filtered to include the top 65% of the most variable genes for model fitting task. The filter was designed using training samples only and was done in a way to ensure that genes of all levels of 5hmC representation were included.
Hyperparameters of the regularization model were selected based on out-of-fold performance on 30 repetitions of 5-fold cross-validated analysis of the training data. Out-of-fold assessments are based on the samples in the left-out fold at each step of the cross-validated analysis. The out-of-fold performance of the models fitted with hyperparameter values set at the optimal values might yield a slightly optimistic assessment of performance. The performance of these models applied to the test set should provide less biased estimate of performance, although generalizability to external datasets is not always guaranteed.
The hyperparameter values that lead to the best out-of-fold performance were then used to fit the final models which were fitted to the entire set of samples, including both training and testing subsets. The performance of these final models can thus only be evaluated based on their performance on external datasets. These do provide a sense of the generalizability of the performance observed in the local training and testing datasets.
To evaluate the effect of feature selection on prediction performance, we repeated the training and evaluation task based on a filtered set of genes that included genes found to be significantly differentially represented, having a 1.5-fold differential 5hmC representation, and a level of representation exceeding the median level (log2 CPM ≥ 3.5). This filter was designed based on training data statistics only.
CA 19-9 was detected from plasma by electrochemiluminescent immunoassay (Roche) at Arup Laboratories.
Further information on research design is available in the Nature Research Reporting Summary linked to this article.
Processed gene counts and BED files data from this study can be accessed from NCBI Gene Expression Omnibus under accession number GSE152137. The Fastq files can be made available upon written request for submission to the study institutional review boards at the participating sites (Sterling IRB or WIRB) for approval, please contact the corresponding author with requests. The remaining data is available in the Article, Supplementary Information.
Kleeff, J. et al. Pancreatic cancer. Nat. Rev. Dis. Primers https://doi.org/10.1038/nrdp.2016.22 (2016).
Tempero, M. A. et al. Pancreatic adenocarcinoma, Version 2.2017, NCCN Clinical Practice Guidelines in Oncology. J. Natl Compr. Cancer Netw. 15, 1028–1061 (2017).
Anderson, M. et al. Alcohol and tobacco lower the age of presentation in sporadic pancreatic cancer in a dose-dependent manner: a multicenter study. Am J Gastroenterol. 107, 1730–1739 (2012).
Maisonneuve, P. & Lowenfels, A. Epidemiology of pancreatic cancer: an update. Dig. Dis. 28, 645–656 (2010).
Swords, D., Firpo, M., Scaife, C. & Mulvihill, S. Biomarkers in pancreatic adenocarcinoma: current perspectives. Onco Targets Ther. 9, 7459–7467 (2016).
Fonseca, A., Kirkwood, K., Kim, M., Maitra, A. & Koay, E. Intraductal papillary mucinous neoplasms of the pancreas: current understanding and future directions for stratification of malignancy risk. Pancreas 47, 272–279 (2018).
Elta, G., Enestvedt, B., Sauer, B. & Lennon, A. ACG clinical guideline: diagnosis and management of pancreatic cysts. Am. J. Gastroenterol. 113, 464–479 (2018).
Ballehaninna, U. K. & Chamberlain, R. S. The clinical utility of serum CA 19-9 in the diagnosis, prognosis and management of pancreatic adenocarcinoma: an evidence based appraisal. J. Gastrointest. Oncol. 3, 105–119 (2012).
Lal, G. et al. Inherited predisposition to pancreatic adenocarcinoma: role of family history and germ-line p16, BRCA1, and BRCA2 mutations. Cancer Res. 60, 409–416 (2000).
Biankin, A. V. et al. Pancreatic cancer genomes reveal aberrations in axon guidance pathway genes. Nature 491, 399–405 (2012).
Waddell, N. et al. Whole genomes redefine the mutational landscape of pancreatic cancer. Nature 518, 495–501 (2015).
Jones, S. et al. Core signaling pathways in human pancreatic cancers revealed by global genomic analyses. Science 321, 1801–1806 (2008).
Bailey, P. et al. Genomic analyses identify molecular subtypes of pancreatic cancer. Nature 531, 47–52 (2016).
Collisson, E. A. et al. Subtypes of pancreatic ductal adenocarcinoma and their differing responses to therapy. Nat. Med. 17, 500–503 (2011).
Moffitt, R. A. et al. Virtual microdissection identifies distinct tumor- and stroma-specific subtypes of pancreatic ductal adenocarcinoma. Nat. Genet. 47, 1168–1178 (2015).
Marazzi, I., Greenbaum, B. D., Low, D. H. P. & Guccione, E. Chromatin dependencies in cancer and inflammation. Nat. Rev. Mol. Cell Biol. 19, 245–261 (2017).
Feinberg, A. Epigenetic stochasticity, nuclear structure and cancer: the implications for medicine. J. Intern Med 276, 5–11 (2014).
Curradi, M., Izzo, A., Badaracco, G. & Landsberger, N. Molecular Mechanisms of Gene Silencing Mediated by DNA Methylation. Mol. Cell. Biol. 22, 3157–3173 (2002).
Yang, X. et al. Gene body methylation can alter gene expression and is a therapeutic target in cancer. Cancer Cell 26, 577–590 (2014).
Kriaucionis, S. & Heintz, N. The nuclear DNA base 5-hydroxymethylcytosine is present in Purkinje neurons and the brain. Science 324, 929–930 (2009).
Tahiliani, M. et al. Conversion of 5-methylcytosine to 5-hydroxymethylcytosine in mammalian DNA by MLL partner TET1. Science 324, 930–935 (2009).
Nestor, C. E. et al. 5-Hydroxymethylcytosine Remodeling Precedes Lineage Specification during Differentiation of Human CD4+ T Cells. Cell Rep. 16, 559–570 (2016).
Song, C.-X. et al. 5-Hydroxymethylcytosine signatures in cell-free DNA provide information about tumor types and stages. Cell Res 27, 1231–1242 (2017).
Zhang, J. et al. 5-Hydroxymethylome in circulating cell-free DNA as a potential biomarker for non-small-cell lung cancer. Genomics, Proteom. Bioinforma. 16, 187–199 (2018).
Li, W. et al. 5-Hydroxymethylcytosine signatures in circulating cell-free DNA as diagnostic biomarkers for human cancers. Cell Res 27, 1243–1257 (2017).
Zhang, Y. et al. Model-based analysis of ChIP-Seq (MACS). Genome Biol. 9, R137 (2008).
Szulwach, K. E. et al. Integrating 5-hydroxymethylcytosine into the epigenomic landscape of human embryonic stem cells. Plos Genet 7, e1002154 (2011).
Ernst, J. & Kellis, M. ChromHMM: automating chromatin-state discovery and characterization. Nat. Methods 9, 215–216 (2012).
Huang, L. et al. Ductal pancreatic cancer modeling and drug screening using human pluripotent stem cell- and patient-derived tumor organoids. Nat. Med. 21, 1364–1371 (2015).
Burke, Z. & Oliver, G. Prox1 is an early specific marker for the developing liver and pancreas in the mammalian foregut endoderm. Mechanisms Dev. 118, 147–155 (2002).
Zhang, H. et al. Multiple, temporal-specific roles for HNF6 in pancreatic endocrine and ductal differentiation. Mechanisms Dev. 126, 958–973 (2009).
Swift, G. H. et al. An endocrine-exocrine switch in the activity of the pancreatic homeodomain protein PDX1 through formation of a trimeric complex with PBX1b and MRG1 (MEIS2). Mol. Cell Biol. 18, 5109–5120 (1998).
Rozengurt, E., Sinnett-Smith, J. & Eibl, G. Yes-associated protein (YAP) in pancreatic cancer: at the epicenter of a targetable signaling network associated with patient survival. Signal Transduct. Target. Ther. 3, 11 (2018).
Saukkonen, K. et al. PROX1 and β-catenin are prognostic markers in pancreatic ductal adenocarcinoma. BMC Cancer 16, 472 (2016).
Friedman, J., Hastie, T. & Tibshirani, R. Regularization paths for generalized linear models via coordinate descent. J. Stat. Softw. 33, 1–22 (2010).
Boël, P. et al. BAGE: a new gene encoding an antigen recognized on human melanomas by cytolytic T lymphocytes. Immunity 2, 167–175 (1995).
Nasir, A. et al. RUNX1T1: a novel predictor of liver metastasis in primary pancreatic endocrine neoplasms. Pancreas 40, 627–633 (2011).
Gieger, C. et al. New gene functions in megakaryopoiesis and platelet formation. Nature 480, 201–208 (2011).
Stamenkovic, I. & Seed, B. The B-cell antigen CD22 mediates monocyte and erythrocyte adhesion. Nature 345, 74–77 (1990).
Siegel, R. L., Miller, K. D. & Jemal, A. Cancer statistics, 2020. Ca Cancer J. Clin. 70, 7–30 (2020).
Moss, J. et al. Comprehensive human cell-type methylation atlas reveals origins of circulating cell-free DNA in health and disease. Nat. Commun. 9, 5068 (2018).
Shen, S. Y. et al. Sensitive tumour detection and classification using plasma cell-free DNA methylomes. Nature 563, 579–583 (2018).
Kang, S. et al. CancerLocator: non-invasive cancer diagnosis and tissue-of-origin prediction using methylation profiles of cell-free DNA. Genome Biol. 18, 53 (2017).
Yang, H. et al. Tumor development is associated with decrease of TET gene expression and 5-methylcytosine hydroxylation. Oncogene 32, 663–669 (2012).
Morris, J. P. et al. α-Ketoglutarate links p53 to cell fate during tumour suppression. Nature 573, 595–599 (2019).
Tian, X. et al. Circulating tumor DNA 5-hydroxymethylcytosine as a novel diagnostic biomarker for esophageal cancer. Cell Res. 28, 597–600 (2017).
Morgan, M. A. & Shilatifard, A. Chromatin signatures of cancer. Genes Dev. 29, 238–249 (2015).
Calo, E. & Wysocka, J. Modification of enhancer chromatin: what, how, and why? Mol. Cell 49, 825–837 (2013).
Raphael, B. J. et al. Integrated genomic characterization of pancreatic ductal adenocarcinoma. Cancer Cell 32, 185–203.e13 (2017).
Baumgart, S. et al. Inflammation-induced NFATc1-STAT3 transcription complex promotes pancreatic cancer initiation by KrasG12D. Cancer Disco. 4, 688–701 (2014).
Roe, J.-S. et al. Enhancer reprogramming promotes pancreatic cancer metastasis. Cell 170, 875–888.e20 (2017).
Lee, K. & Pausova, Z. Cigarette smoking and DNA methylation. Front. Genet. 4, 132 (2013).
Li, H. & Durbin, R. Fast and accurate long-read alignment with Burrows-Wheeler transform. Bioinformatics 26, 589–595 (2010).
Institute, B. “Picard Toolkit.” Broad Institute, GitHub Repository. http://broadinstitute.github.io/picard/ (Broad Institute, 2019).
Li, H. et al. The sequence alignment/Map format and SAMtools. Bioinformatics 25, 2078–2079 (2009).
Quinlan, A. R. & Hall, I. M. BEDTools: a flexible suite of utilities for comparing genomic features. Bioinformatics 26, 841–842 (2010).
Robinson, J. T. et al. Integrative genomics viewer. Nat. Biotechnol. 29, 24 (2011).
Law, C. W., Alhamdoosh, M., Su, S., Smyth, G. K. & Ritchie, M. E. RNA-seq analysis is easy as 1-2-3 with limma, Glimma and edgeR. F1000Research 5, 1408 (2016).
Team, R. C. R: A language and environment for statistical computing. R Foundation for Statistical Computing, Vienna, Austria. https://www.R-project.org/ (2017).
Benjamini, Y. & Hochberg, Y. Controlling the false discovery rate: a practical and powerful approach to multiple testing. J. R. Stat. Soc. Series B (Methodological) 57, 289–300 (1995).
G.D.G., F.C., Y.N., C.-J.K., T.P., E.M., C.E., A.B., P.L., A.S., M.A., W.W., K.C., and S.L. are employees and shareholders of Bluestar Genomics. A.A. and S.Q. are advisors and shareholders of Bluestar Genomics.
Peer review information Nature Communications thanks the anonymous reviewers for their contribution to the peer review of this work.
Publisher’s note Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
About this article
Cite this article
Guler, G.D., Ning, Y., Ku, CJ. et al. Detection of early stage pancreatic cancer using 5-hydroxymethylcytosine signatures in circulating cell free DNA. Nat Commun 11, 5270 (2020). https://doi.org/10.1038/s41467-020-18965-w
This article is cited by
EBS-seq: enrichment-based method for accurate analysis of 5-hydroxymethylcytosine at single-base resolution
Clinical Epigenetics (2023)
Coagulation parameters for the differential diagnosis of pancreatic cancer in the early stage: a retrospective study
European Journal of Medical Research (2023)
Nature Biotechnology (2023)
Cell-selective proteomics segregates pancreatic cancer subtypes by extracellular proteins in tumors and circulation
Nature Communications (2023)
Signal Transduction and Targeted Therapy (2023)