- Open Access
Detection of cryptogenic malignancies from metagenomic whole genome sequencing of body fluids
Genome Medicine volume 13, Article number: 98 (2021)
Metagenomic next-generation sequencing (mNGS) of body fluids is an emerging approach to identify occult pathogens in undiagnosed patients. We hypothesized that metagenomic testing can be simultaneously used to detect malignant neoplasms in addition to infectious pathogens.
From two independent studies (n = 205), we used human data generated from a metagenomic sequencing pipeline to simultaneously screen for malignancies by copy number variation (CNV) detection. In the first case-control study, we analyzed body fluid samples (n = 124) from patients with a clinical diagnosis of either malignancy (positive cases, n = 65) or infection (negative controls, n = 59). In a second verification cohort, we analyzed a series of consecutive cases (n = 81) sent to cytology for malignancy workup that included malignant positives (n = 32), negatives (n = 18), or cases with an unclear gold standard (n = 31).
The overall CNV test sensitivity across all studies was 87% (55 of 63) in patients with malignancies confirmed by conventional cytology and/or flow cytometry testing and 68% (23 of 34) in patients who were ultimately diagnosed with cancer but negative by conventional testing. Specificity was 100% (95% CI 95–100%) with no false positives detected in 77 negative controls. In one example, a patient hospitalized with an unknown pulmonary illness had non-diagnostic lung biopsies, while CNVs implicating a malignancy were detectable from bronchoalveolar fluid.
Metagenomic sequencing of body fluids can be used to identify undetected malignant neoplasms through copy number variation detection. This study illustrates the potential clinical utility of a single metagenomic test to uncover the cause of undiagnosed acute illnesses due to cancer or infection using the same specimen.
Pathogen identification using metagenomic testing has recently been clinically implemented for patient care by our group and others [1,2,3,4,5,6,7,8]. While clinical metagenomic sequencing is often performed for patients who lack a definitive diagnosis to search for an infectious organism, the underlying disease may also be rooted in a non-infectious cause such as a malignant neoplasm. Detection of malignancies in various body fluids is primarily based on cytological analysis as the gold standard test. However, the estimated sensitivity for cytology is 60% for pleural fluid , 67% for peritoneal fluid in the context of ovarian carcinoma , and approaching undetectable for liver masses without concurrent peritoneal carcinomatosis .
By repurposing the residual human reads in metagenomic sequencing data from non-circulating fluids (e.g., pleural, peritoneal, respiratory fluids), we hypothesized that we would concurrently detect cancer associated CNVs using a depth of coverage method [12,13,14,15,16,17]. This method was previously used to detect fetal aneuploidy in non-invasive prenatal testing (NIPT)  and later cytogenetic aberrations in cancer (Fig. 1A) [13,14,15,16]. CNVs are ubiquitous in solid tumors, with aneuploidy alone present in ~ 90% of malignant tumors , making this an appealing broad range marker.
The first study incorporated residual body fluid samples sent to the UCSF Clinical Laboratories (San Francisco, CA, USA) between 2017 to 2019 for flow cytometry, cell count, chemistries, and microbiological testing. All samples matching inclusion criteria (see below) in a recent metagenomics study were used, except five samples were excluded because they had less than 450,000 reads . Serial dilutions of the sample input and downsampling of sequencing reads suggested that results are interpretable down to 1.6 pg input and 276,000 reads (Additional file 1). A total of 65 cancer-positive and 59 cancer-negative samples were collected. The samples consisted of 62 (50%) pleural fluid, 31 (25%) peritoneal fluid, 24 (19%) bronchoalveolar lavage fluid, and 7 (6%) other body fluids. The positive cases were included from patients with a clinical diagnosis of cancer established either by definitive laboratory testing (cytology and/or flow cytometry of a body fluid), tissue biopsy (“histologically confirmed”), or by the treating physician on the basis of history, presentation, radiographic imaging, and supportive laboratory testing results (“histologically unconfirmed”). Patients lacking a clear diagnosis after long-term follow-up were excluded. Patients who were being actively treated for malignancy at the time of sample collection and not positive by cytology or cytometry were excluded. Negative controls were taken from the prior metagenomics study , and we included patients with a microbiologically proven infection, who lacked clinical history of cancer, and who were negative for malignancy by cytology and cytometry.
The second study analyzed all consecutively available body fluid samples sent to Stanford clinical laboratories over 2.5 months in 2020 for cytologic testing. There was a total of 81 consecutive cases comprised of 56% pleural, 19% peritoneal, 14% bronchoalveolar lavage, 4% pericardial, and 2% fine needle aspirate. The residual samples were categorized similarly to the first study for positive cases and negative controls. However, the negative controls also included non-microbiological diagnoses by the treating physician. All available samples from cytology were included, except for those with insufficient volumes of less than 0.5 mL and those received outside of working hours.
Body fluid sample extraction
Body fluid specimens were centrifuged at 16,000g for 10 min, and the supernatant was stored at – 80 °C. In the first study, nucleic acid extraction was performed by the EZ1 Advanced XL BioRobot using the EZ1 Virus Mini Kit v2.0 (QIAGEN) with 400 μL input and 60 μL output. In the second study, nucleic acid extraction was performed using the Maxwell RSC ccfDNA Plasma Kit (Promega) with 1000 μL input and 50 μL output.
Body fluid library preparation
Whole genome sequencing (WGS) library preparation was performed using the NEBNext Ultra II DNA Library Prep Kit (New England Biolabs) on a liquid handler (first study: epMotion 5075 Eppendorf, second study: Hamilton STARlet) using the manufacturer’s protocol unless otherwise stated. All reagent usage was halved, and the input was also halved to 25 μL of extracted DNA. For bead purification, we used Ampure XP beads (Beckman Coulter) or Mag-Bind TotalPure beads (Omega Biotek) in the first and second study respectively. PCR amplification of the adapter ligated DNA was up to 26 cycles using the manufacturer’s protocol, and we used primers with dual indexing. Sequencing was performed on an Illumina HiSeq 1500/2500, Nextseq 550, or Novaseq using the single-end or paired-end rapid run configuration set at 1 × 140 bp or 2 × 140 bp. Only samples with more than 450 thousand reads were considered for this study.
Tissue extraction and library preparation
Formalin fixed paraffin blocks were used to obtain correlated CNV data from cancer tissue obtained from the same patient. All archival tissue was no longer needed for clinical care. A pathologist (J.S.) identified regions of high tumor content on correlated tissue section(s). A disposable dermal punch was used to either punch out or scrape tissue from regions of interest. This fixed tissue was extracted for nucleic acids using the Quick-DNA FFPE Miniprep kit (Zymo Research). Each sample was sheared using focused acoustics to approximately 250 bp in a microTUBE (Covaris) and quantified on a spectrometer (Nanodrop, Thermo Fisher). About 100 ng was used for WGS library preparation as described above.
Abbott Vysis LSI D7S486/CEP7, CEP8, and D20S108 probe sets were used for detecting deletion of chromosome 7q/loss of a chromosome 7, gain of a chromosome 8, and deletion of chromosome 20q, respectively. These probes were ordered from Abbott Molecular (Des Plaines, IL). FISH was performed following a standard protocol (https://www.molecular.abbott/us/en/vysis-fish-knowledge-center). Interphase cells were counterstained using DAPI II (Abbott Molecular) and FISH results were analyzed using the CytoVision system (Leica Microsystems, San Jose, CA).
Raw data was demultiplexed to raw FASTQ files and adapter trimmed with cutadapt (v1.16). The metagenomic pipeline used SURPI [2, 18] for pathogen detection from metagenomic sequencing data. Raw copy ratio plots were created by deduplicating metagenomic reads with BWA  (v0.7.12) and aligning deduplicated reads to the human genome hg38 and. CNVkit  (v0.9.1) was used to display a log2 copy ratio across all genomic bins and infer discrete copy number segments using the default circular binary segmentation algorithm (orange in plots). Body fluid samples were normalized to a plasma sample from a healthy male. Correlated tissue samples were normalized to a resected tonsil from an otherwise healthy boy undergoing tonsillectomy due to an infection.
To determine NGS positives, a molecular pathologist (JT) was blinded to and not involved with gold standard determination, sample collection, preparation, and copy ratio plotting. The pathologist identified samples with copy ratio plots showing at least one significant CNV(s) (> 10 Mbp) across all chromosomes with the exception of the entirety of the sex chromosomes (differences in sex were not accounted for) and chromosome 19 due to its GC rich content and known tendency to appear more noisy than all other chromosomes [12, 22]. Chromosome 19 was used as a metric for the extent of noise on a per sample basis, typically for samples with low DNA content. Smaller telomere and centromere regions and deviations from diploid that are gradual rather than abrupt were both interpreted with caution. Individually binned copy ratios (gray dots in plots) were primarily used rather than the results of segmentation algorithms (orange/red line in plots). Before interpreting the second study, the interpreter was able to review the gold standard for the first study that was already interpreted.
The tumor fraction (Equation 1) was estimated from the log 2 ratio of the sample to the diploid control copy number. An assumption is made that certain deletions were haploid (e.g., monosomy) or that certain gains were haploid (e.g., trisomy).
Test performance study
A total of 65 cancer-positive and 59 cancer-negative samples were collected from University of California San Francisco (UCSF) Medical Center. The samples consisted of 62 (50%) pleural fluid, 31 (25%) peritoneal fluid, 24 (19%) bronchoalveolar lavage fluid, and 7 (6%) other body fluids (Fig. 1B). Samples were from patients who were hospitalized (78% of positives and 94% of negatives) and who all presented with symptoms that warranted a diagnostic workup, including cytology and other laboratory testing of the body fluid. Metagenomic whole genome sequencing was performed on physiologically fragmented DNA yielding a median of 7.6 million reads (IQR 4.6–11.2 M) per sample with the vast majority of reads (> 95%) consistently aligning to human host cell-free DNA.
To provide an initial assessment of the test sensitivity, we analyzed the genomic human DNA reads for large (> 10 Mbp) CNVs in 36 cases that were positive for malignancy based on the conventional testing of the sample using cytology and/or flow cytometry. CNVs were called based on blinded interpretation of algorithmically generated copy ratio plots while considering the deviation of the copy ratio from diploid against background noise among other factors (see the “Methods” section). Of these cases, 31 of these had detectable CNVs at a sensitivity of 86% (95% CI 71–95%, Clopper-Pearson method) (Fig. 1C, Additional file 2: Table S1). The median tumor fraction of all 36 cases was 43% (IQR 25–59%) based on Equation 1 in the “Methods” section (Fig. 1D).
To better estimate the diagnostic sensitivity of body fluid CNV testing in the undiagnosed patient population, we analyzed additional cases where (i) cytology and/or flow cytometry results were negative (benign) or inconclusive (e.g., atypical cells), and (ii) a malignancy was eventually diagnosed through a subsequent tissue biopsy or as a histologically unconfirmed clinical diagnosis (Table 1). Patients lacking a diagnosis after long-term follow-up or were actively treated for malignancy at the time of sample collection were also excluded. Out of 29 such cases, CNVs were still detected in 19 at a sensitivity of 66% (95% CI 46–82%) (Fig. 1C, Table 1). The median tumor fraction was 30% (IQR 1.4–56%) (Fig. 1D). Both the sensitivity and the tumor fraction were lower when cytology/cytometry were negative, but unexpectedly high considering that conventional testing was not able to detect the malignancy. We therefore sought to confirm the positive CNV findings further by matching the CNVs in the body fluid and correlated cancer tissue from the same patient. In all 12 cases (out of these 19) for which clinical cytogenetic or molecular testing of the tumor was available, the CNVs found in the body fluid matched those in the associated cancer tissue (Additional file 1).
To evaluate test specificity, we ran the CNV test on 59 body fluids from acutely ill hospitalized patients with microbiologically proven (culture, serology, antigen, PCR) infection but without evidence of malignancy (Additional file 3: Table S2, Additional file 4: Table S3). All 59 fluids were all negative for detection of CNVs, placing the estimated specificity at 94–100% (95% CI, Clopper-Pearson).
An adult patient presented with fever, dyspnea, weakness, and weight loss and was found to have eosinophilia and a > 3-cm lung mass. The patient underwent several non-diagnostic thoracic procedures, including bronchoscopies, mediastinoscopy, thoracentesis, and a surgical biopsy (Fig. 2A). The patient’s bone marrow biopsy revealed increased eosinophils and precursors, and chronic eosinophilic leukemia (CEL) was suspected based on an abnormal karyotype . CEL is a rare entity with diagnostic criteria that include (i) eosinophilia (eosinophil count ≥ 1.5 × 109/L) (criteria not met) and (ii) clonal cytogenetic or molecular genetic abnormality or increase in BM or peripheral blood blasts (criteria met). However, her lung disease was unexplained as eosinophils detected in the thoracic biopsies did not appear dysplastic morphologically (Fig. 2B–D). It was uncertain whether the eosinophils were reactive secondary to pulmonary infection and/or inflammation or myeloid neoplasm.
The bronchoalveolar lavage (BAL) fluid underwent mNGS. Bacteria, but not fungi, viruses, and parasites, were detected by mNGS, and the bacterial profile, consisting predominantly of reads from Enterobacter cloacae, matched Gram stain and culture results from the BAL fluid (Fig. 2E). However, this bacterial infection was not considered as the underlying cause for the patient’s initial clinical presentation nor her ongoing pulmonary symptoms. The CNV analysis showed gains in chromosome 1q, 8, and 17q and losses in 7q, 17p, and 20q and indicated that this clonal process comprised up to 94% (range 90–96%) of the total DNA (Fig. 2F). Fluorescent in situ hybridization (FISH) analysis of resected lung tissue confirmed the same cytogenetic abnormalities (Fig. 2G). The CNV and cytogenetic profile found in BAL fluid and lung tissue matched the clone found in the patient’s bone marrow biopsy (Fig. 2H), implicating leukemic infiltration of the lung as the most likely cause of the patient’s lung mass and acute illness.
Second verification cohort
To further verify our findings, we performed a secondary verification study at a separate medical site (Stanford Medical Center), comprised of 81 consecutive cases (56% pleural, 19% peritoneal, 14% bronchoalveolar lavage, 4% pericardial, 2% fine needle aspirate). These were available residual samples used for testing by cytology from a single laboratory, and no available samples with sufficient volume were excluded.
Using the criteria in the test performance study, there were 32 total positive cases. The sensitivity of the 27 cases that were positive by cytology or flow cytometry was 89% (95% CI 71–98%), with a median tumor fraction of 34% (IQR 14–46%). Of the 5 positive cases that were negative by cytology, 4 were detectable by NGS. The specificity of all 18 cases with no cancer diagnosis and an alternative diagnosis made by the treating physician was 100% (95% CI 81–100%).
The remaining cases (n = 22) that did not match the inclusion criteria for positives and negatives were composed of patients with an unclear gold standard. These cases either had an actively treated cancer or did not have at least a working diagnosis that prompted treatment. Six of the 22 cases (27%) were positive. Of the 9 cases with no history of cancer and had an unclear diagnosis, one was positive.
Across the two studies, the overall sensitivity was 87% (95% CI 77–94%) for cytology/cytometry-positive cases and 68% (95% CI 49–83%) for cytology/cytometry-negative cases but were ultimately diagnosed with an adjacent malignancy (Fig. 1C, D). The overall specificity using only negative controls was 100% (95% CI 95–100%).
We performed three microbiological evaluations of the current data. First, we evaluated all positive cancer cases for oncoviruses. In three of the 97 cancer-positive cases (65 from test performance study and 32 from the verification cohort), Epstein-Barr virus (EBV)/human herpesvirus 4 (HHV4), a gammaherpesvirus human oncovirus , was detected by mNGS. The cases were angioimmunoblastic T cell lymphoma (P13), Hodgkin lymphomas (P45), and a presumptive lymphoproliferative disorder, otherwise not classified (P42). In one case, CNV detection alone was negative (PC13). In 2 of 3 EBV positive cases with sufficient EBV reads for further characterization, both had cfDNA length distributions consistent with oncovirus integration into the human genome (as opposed to EBV reactivation), based on criteria previously reported for cfDNA from EBV-positive nasopharyngeal carcinoma  (Additional file 1). Alphapapillomavirus 9, which includes human papillomavirus (HPV) type 16, was positive in two cases (PC50, 3134) related to the patient’s squamous cell carcinoma of the anus and vulva, the latter of which was known to express HPV p16 on immunohistochemistry.
The performance characteristics for microbial detection of the first study were reported previously . However, in the second analysis, we found 10 cases (11 microbial pathogens) across all cases in the first study that had a gold standard pathogen as previously reported and with non-specific clinical presentations that could be associated with infection or cancer (e.g., fever, lymphadenopathy, weight loss, mass) (Additional file 3: Table S2). When assessing the positive gold standard organisms, all but one had more organisms than all other samples in the first study (Additional file 6: Figure S1).
In the third analysis, we analyzed all new cases in the second cohort without a clear diagnosis prior to the NGS result (n = 9) and found 2 significant pathogens based on past criteria . Case 3026 was a transplant patient with a B cell deficiency and a remote cancer history who presented with hemoptysis and was found to have pulmonary consolidations and eosinophilia. Microbial analysis showed that Haemophilus influenzae as a significant occult pathogen at 1412 species-specific reads, and all reads compatible with H. influenzae declassified up to the taxonomic Family level accounted for 95% of all of the bacterial and fungi reads. The patient had a history of H. influenzae infection and previously received amoxicillin for presumed pneumonia, which may not have been an adequate treatment initially. The patient improved under empiric therapy that included a third-generation cephalosporin. In our experience with metagenomic NGS, H. influenzae is an organism often missed by conventional methods [20, 26, 27]. Anelloviruses were also found, consistent with the patient’s known immunocompromised status. Case 3095 was a transplant patient with bilateral pleural effusions of uncertain etiology that was attributed to acute respiratory distress syndrome (ARDS). Microbial analysis showed 7434 EBV reads and degraded human DNA precluded analysis for oncovirus integration. The patient was known to be immunocompromised with a low level of EBV viremia in the past year.
In this study, we show that residual data from metagenomic and whole genome sequencing can provide reliable CNV data and detect 68% (23 of 34) of malignant body fluids when they were undetectable through conventional testing provided by cytology and flow cytometry. Detection of missed cases highlights the potential of sequencing-based tests in finding malignancies earlier or less invasively in cases without a clear diagnosis. Surprisingly, these NGS-positive body fluids were high in tumor fraction (median 32%, IQR 27–58%) despite negative conventional testing by cytology and flow cytometry. These cases, including the case PC63, underscore the challenges in the diagnosis of malignancy or infection in acutely ill patients who have overlapping clinical presentations. Both conditions can present with B-symptoms (fever , night sweats, weight loss), lymphadenopathy, eosinophilia , exudative effusions , and nodules/masses/cavitations . Notably, over 25% of pulmonary nodule biopsies are non-diagnostic and 21% of those had a final diagnosis that was malignant . Across both studies, whole genome testing detected 7 of 10 of such pulmonary nodule/masses in cases not found by conventional testing. As another example, 25% of cryptogenic hepatocellular carcinoma had ascites as part of their presentation  whereas few are positive based on traditional testing including cytology . Whole genome testing detected 4 of 5 (80%) of such liver mass cases not found by conventional testing.
Here we demonstrate dual use of metagenomic sequencing of cfDNA in body fluids to simultaneously screen for infection and cryptogenic malignancy. Previous groups have detected incidental malignancies in pregnant women by non-invasive prenatal testing (NIPT) of blood . However, the incidence of malignancy in asymptomatic pregnant women is ~ 0.1%, which is low compared to the 20–25% incidence in hospitalized patients with non-specific acute illness [30, 31]. We and other groups have also previously demonstrated the presence of tumor cfDNA in body fluids [33,34,35,36], but these studies have not focused on broad-based screening for cryptogenic malignancies nor the potential repurposing of metagenomic data used for pathogen identification for cancer diagnosis.
The advantages of CNV body fluid testing to screen for malignancies include (i) leveraging of clinical mNGS data already generated for infectious disease diagnosis [1,2,3], (ii) rapid turnaround time (< 48 h) that is crucial for critically ill patients, (iii) straightforward interpretation compared to cancer gene panel testing , (iv) increase in diagnostic yield over conventional testing (detection of 66% of cases not found by conventional testing), and (v) high analytical specificity (no false positives out of 59 samples). High specificity was also illustrated in 3 large NIPT studies [13,14,15] involving 124,000, 450,000, and 1.93 million patients, where the frequency of CNV abnormal cases (multiple aneuploidies) in plasma was only 0.031%, 0.012%, and 0.033%, with confirmation of maternal cancer in 18%, 47%, and 7.6% of those positives respectively. Another advantage is the addition of cytogenetic and viral (e.g., EBV) driver characterization of the tumor to facilitate diagnosis, provide prognostic information, and potentially guide targeted therapy (Table 1, Additional file 2: Table S1). Finally, body fluids are often available in ample quantities and are both easier and less invasive to collect than tissue biopsies. The CNV test presented here uses only 0.4 mL of body fluid input and can be performed on discarded supernatant byproducts of traditional cell-based assays such as cytology, flow cytometry, or microbiological culture.
Limitations of this testing approach include the lack of CNVs in a minority (< 10%) of malignant neoplasms even though > 90% of solid tumors have CNVs  and the analytical requirement for approximately > 5% tumor fraction, similar to NIPT . Although cancer gene panels are capable of detection at lower tumor fractions, often down to 1% , there is potential concern for false-positive results of low burden pathogenic mutations that can be incidentally detected in normal controls [39,40,41,42] and benign growths [43, 44]. Using subsequent targeted gene panels is not ruled out by this testing approach, but rather informed by the rapid assessment for positive cancer samples, which can also have higher tumor fractions than tissue biopsies (e.g., PC46, Additional file 1). In the current study, the median tumor fractions in laboratory-confirmed and unconfirmed cancer samples were 43% and 26%, respectively, well above the minimum threshold.
The dual ability to screen for cryptogenic malignancies and pathogens by metagenomic whole genome sequencing of body fluids simultaneously on the same patient specimen may reduce time to diagnosis and increase diagnostic accuracy. Early diagnosis of malignancy and/or infection may enable further workup and guide more timely treatment, while the availability of high tumor fraction material in the body fluids allows for further molecular testing to classify the cancer and find actionable driver mutations (e.g., KIT  in the index case). Clinical validation and prospective diagnostic trials will be needed to investigate the clinical utility and ethical ramifications of this test for simultaneous cancer diagnosis and pathogen detection.
Availability of data and materials
CNVkit (https://cnvkit.readthedocs.io/)  and SURPI+ v.1.0 (https://github.com/chiulab/SURPI-plus-dist) software  for CNV and pathogen detection are both available for free online. CNV data, Metagenomic Fastq data, image data, and data analysis scripts were deposited or linked to on Zenodo (https://0-doi-org.brum.beds.ac.uk/10.5281/zenodo.4697549) . The CNV datasets can be read with a text editor or CNVkit . Metagenomic sequencing data (FASTQ files) with human genomic reads removed were also deposited as a NCBI SRA under Bioproject PRJNA707099, https://www.ncbi.nlm.nih.gov/bioproject/?term=PRJNA707099 .
Fine needle aspirate
Copy number variation
Diffuse large B cell lymphoma
Acute myeloid leukemia
Fluorescence in situ hybridization
Cancer panels based on NGS
Wilson MR, Sample HA, Zorn KC, Arevalo S, Yu G, Neuhaus J, et al. Clinical metagenomic sequencing for diagnosis of meningitis and encephalitis. N Engl J Med. 2019;380(24):2327–40. https://0-doi-org.brum.beds.ac.uk/10.1056/NEJMoa1803396.
Miller S, Naccache SN, Samayoa E, Messacar K, Arevalo S, Federman S, et al. Laboratory validation of a clinical metagenomic sequencing assay for pathogen detection in cerebrospinal fluid. Genome Res. 2019; Available from: http://genome.cshlp.org/content/early/2019/03/07/gr.238170.118. [cited 2019 May 31].
Blauwkamp TA, Thair S, Rosen MJ, Blair L, Lindner MS, Vilfan ID, et al. Analytical and clinical validation of a microbial cell-free DNA sequencing test for infectious disease. Nat Microbiol. 2019;4(4):663–74. https://0-doi-org.brum.beds.ac.uk/10.1038/s41564-018-0349-6.
Goggin KP, Gonzalez-Pena V, Inaba Y, Allison KJ, Hong DK, Ahmed AA, et al. Evaluation of plasma microbial cell-free DNA sequencing to predict bloodstream infection in pediatric patients with relapsed or refractory cancer. JAMA Oncol. 2019; Available from: https://jamanetwork.com/journals/jamaoncology/fullarticle/2757390. [cited 2020 Jan 4]
Thoendel MJ, Jeraldo PR, Greenwood-Quaintance KE, Yao JZ, Chia N, Hanssen AD, et al. Identification of prosthetic joint infection pathogens using a shotgun metagenomics approach. Clin Infect Dis. 2018;67(9):1333–8. https://0-doi-org.brum.beds.ac.uk/10.1093/cid/ciy303.
Gu W, Lee M, Arevalo S, Federman S, Whitman J, Khan L, et al. Pathogen detection by metagenomic next generation sequencing of purulent body fluids. J Mol Diagn. 2017;19:943–1067.
Chiu CY, Miller SA. Clinical metagenomics. Nat Rev Genet. 2019;20(6):341–55. https://0-doi-org.brum.beds.ac.uk/10.1038/s41576-019-0113-7.
Schlaberg R, Chiu CY, Miller S, Procop GW, Weinstock G. Validation of metagenomic next-generation sequencing tests for universal pathogen detection. Arch Pathol Lab Med. 2017;141(6):776–86. https://0-doi-org.brum.beds.ac.uk/10.5858/arpa.2016-0539-RA.
Porcel JM, Esquerda A, Vives M, Bielsa S. Etiology of pleural effusions: analysis of more than 3,000 consecutive thoracenteses. Arch Bronconeumol. 2014;50(5):161–5. https://0-doi-org.brum.beds.ac.uk/10.1016/j.arbres.2013.11.007.
Allen VA, Takashima Y, Nayak S, Manahan KJ, Geisler JP. Assessment of false-negative ascites cytology in epithelial ovarian carcinoma: a study of 313 patients. Am J Clin Oncol. 2017;40(2):175–7. https://0-doi-org.brum.beds.ac.uk/10.1097/COC.0000000000000119.
Runyon BA, Hoefs JC, Morgan TR. Ascitic fluid analysis in malignancy-related ascites. Hepatol Baltim Md. 1988;8(5):1104–9. https://0-doi-org.brum.beds.ac.uk/10.1002/hep.1840080521.
Fan HC, Blumenfeld YJ, Chitkara U, Hudgins L, Quake SR. Noninvasive diagnosis of fetal aneuploidy by shotgun sequencing DNA from maternal blood. Proc Natl Acad Sci. 2008;105(42):16266–71. https://0-doi-org.brum.beds.ac.uk/10.1073/pnas.0808319105.
Bianchi DW, Chudova D, Sehnert AJ, Bhatt S, Murray K, Prosen TL, et al. Noninvasive prenatal testing and incidental detection of occult maternal malignancies. JAMA. 2015;314(2):162–9. https://0-doi-org.brum.beds.ac.uk/10.1001/jama.2015.7120.
Dharajiya NG, Grosu DS, Farkas DH, McCullough RM, Almasri E, Sun Y, et al. Incidental Detection of Maternal Neoplasia in Noninvasive Prenatal Testing. Clin Chem. 2018;64:329–35.
Ji X, Li J, Huang Y, Sung P-L, Yuan Y, Liu Q, et al. Identifying occult maternal malignancies from 1.93 million pregnant women undergoing noninvasive prenatal screening tests. Genet Med. 2019;21:2293–302.
Amant F, Verheecke M, Wlodarska I, Dehaspe L, Brady P, Brison N, et al. Presymptomatic identification of cancers in pregnant women during noninvasive prenatal testing. JAMA Oncol. 2015;1(6):814–9. https://0-doi-org.brum.beds.ac.uk/10.1001/jamaoncol.2015.1883.
Talevich E, Shain AH, Botton T, Bastian BC. CNVkit: Genome-wide copy number detection and visualization from targeted DNA sequencing. PLOS Comput Biol. 2016;12(4):e1004873. https://0-doi-org.brum.beds.ac.uk/10.1371/journal.pcbi.1004873.
Naccache SN, Federman S, Veeeraraghavan N, Zaharia M, Lee D, Samayoa E, et al. A cloud-compatible bioinformatics pipeline for ultrarapid pathogen identification from next-generation sequencing of clinical samples. Genome Res. 2014; Available from: http://genome.cshlp.org/content/early/2014/05/16/gr.171934.113. [cited 2017 Nov 7]
Taylor AM, Shih J, Ha G, Gao GF, Zhang X, Berger AC, et al. Genomic and functional approaches to understanding cancer aneuploidy. Cancer Cell. 2018;33:676–689.e3.
Gu W, Deng X, Lee M, Sucu YD, Arevalo S, Stryke D, et al. Rapid pathogen detection by metagenomic next-generation sequencing of infected body fluids. Nat Med. 2021;27(1):115–24. https://0-doi-org.brum.beds.ac.uk/10.1038/s41591-020-1105-z.
Li H, Durbin R. Fast and accurate short read alignment with Burrows-Wheeler transform. Bioinforma Oxf Engl. 2009;25(14):1754–60. https://0-doi-org.brum.beds.ac.uk/10.1093/bioinformatics/btp324.
Grimwood J, Gordon LA, Olsen A, Terry A, Schmutz J, Lamerdin J, et al. The DNA sequence and biology of human chromosome 19. Nature. 2004;428(6982):529–35. https://0-doi-org.brum.beds.ac.uk/10.1038/nature02399.
Helbig G, Soja A, Bartkowska-Chrobok A, Kyrcz-Krzemień S. Chronic eosinophilic leukemia-not otherwise specified has a poor prognosis with unresponsiveness to conventional treatment and high risk of acute transformation. Am J Hematol. 2012;87(6):643–5. https://0-doi-org.brum.beds.ac.uk/10.1002/ajh.23193.
Klein E, Kis LL, Klein G. Epstein-Barr virus infection in humans: from harmless to life endangering virus-lymphocyte interactions. Oncogene. 2007;26(9):1297–305. https://0-doi-org.brum.beds.ac.uk/10.1038/sj.onc.1210240.
Lam WKJ, Jiang P, Chan KCA, Cheng SH, Zhang H, Peng W, et al. Sequencing-based counting and size profiling of plasma Epstein–Barr virus DNA enhance population screening of nasopharyngeal carcinoma. Proc Natl Acad Sci. 2018;115(22):E5115–24. https://0-doi-org.brum.beds.ac.uk/10.1073/pnas.1804184115.
Langelier C, Kalantar KL, Moazed F, Wilson MR, Crawford ED, Deiss T, et al. Integrating host response and unbiased microbe detection for lower respiratory tract infection diagnosis in critically ill adults. Proc Natl Acad Sci. 2018;115(52):E12353–62. https://0-doi-org.brum.beds.ac.uk/10.1073/pnas.1809700115.
Zinter MS, Dvorak CC, Mayday MY, Iwanaga K, Ly NP, McGarry ME, et al. Pulmonary metagenomic sequencing suggests missed infections in immunocompromised children. Clin Infect Dis. 2019;68(11):1847–55. https://0-doi-org.brum.beds.ac.uk/10.1093/cid/ciy802.
Vanderschueren S, Knockaert D, Adriaenssens T, Demey W, Durnez A, Blockmans D, et al. From prolonged febrile illness to fever of unknown origin: the challenge continues. Arch Intern Med. 2003;163(9):1033–41. https://0-doi-org.brum.beds.ac.uk/10.1001/archinte.163.9.1033.
Shomali W, Gotlib J. World Health Organization-defined eosinophilic disorders: 2019 update on diagnosis, risk stratification, and management. Am J Hematol. 2019;94(10):1149–67. https://0-doi-org.brum.beds.ac.uk/10.1002/ajh.25617.
Lee KH, Lim KY, Suh YJ, Hur J, Han DH, Kang M-J, et al. Nondiagnostic percutaneous transthoracic needle biopsy of lung lesions: a multicenter study of malignancy risk. Radiology. 2018;290:814–23.
Hsu C-Y, Lee Y-H, Liu P-H, Hsia C-Y, Huang Y-H, Lin H-C, et al. Decrypting cryptogenic hepatocellular carcinoma: clinical manifestations, prognostic factors and long-term survival by propensity score model. Plos One. 2014;9(2):e89373. https://0-doi-org.brum.beds.ac.uk/10.1371/journal.pone.0089373.
Pavlidis NA. Coexistence of pregnancy and malignancy. Oncologist. 2002;7(4):279–87. https://0-doi-org.brum.beds.ac.uk/10.1634/theoncologist.2002-0279.
Pan W, Gu W, Nagpal S, Gephart MH, Quake SR. Brain tumor mutations detected in cerebral spinal fluid. Clin Chem. 2015;61(3):514–22. https://0-doi-org.brum.beds.ac.uk/10.1373/clinchem.2014.235457.
Wang Y, Sundfeldt K, Mateoiu C, Shih I-M, Kurman RJ, Schaefer J, et al. Diagnostic potential of tumor DNA from ovarian cyst fluid. eLife. 5. Available from: https://0-www-ncbi-nlm-nih-gov.brum.beds.ac.uk/pmc/articles/PMC4946896/. [cited 2018 Jul 24]
Springer SU, Chen C-H, Rodriguez Pena MDC, Li L, Douville C, Wang Y, et al. Non-invasive detection of urothelial cancer through the analysis of driver gene mutations and aneuploidy. eLife. 7. Available from: https://0-www-ncbi-nlm-nih-gov.brum.beds.ac.uk/pmc/articles/PMC5860864/. [cited 2019 Apr 29]
Liu X, Lu Y, Zhu G, Lei Y, Zheng L, Qin H, et al. The diagnostic accuracy of pleural effusion and plasma samples versus tumour tissue for detection of EGFR mutation in patients with advanced non-small cell lung cancer: comparison of methodologies. J Clin Pathol. 2013;66(12):1065–9. https://0-doi-org.brum.beds.ac.uk/10.1136/jclinpath-2013-201728.
Li MM, Datto M, Duncavage EJ, Kulkarni S, Lindeman NI, Roy S, et al. Standards and guidelines for the interpretation and reporting of sequence variants in cancer: a joint consensus recommendation of the Association for Molecular Pathology, American Society of Clinical Oncology, and College of American Pathologists. J Mol Diagn JMD. 2017;19(1):4–23. https://0-doi-org.brum.beds.ac.uk/10.1016/j.jmoldx.2016.10.002.
Norton ME, Jacobsson B, Swamy GK, Laurent LC, Ranzini AC, Brar H, et al. Cell-free DNA analysis for noninvasive examination of trisomy. N Engl J Med. 2015;372(17):1589–97. https://0-doi-org.brum.beds.ac.uk/10.1056/NEJMoa1407349.
Krimmel JD, Schmitt MW, Harrell MI, Agnew KJ, Kennedy SR, Emond MJ, et al. Ultra-deep sequencing detects ovarian cancer cells in peritoneal fluid and reveals somatic TP53 mutations in noncancerous tissues. Proc Natl Acad Sci U S A. 2016;113(21):6005–10. https://0-doi-org.brum.beds.ac.uk/10.1073/pnas.1601311113.
Newman AM, Bratman SV, To J, Wynne JF, Eclov NCW, Modlin LA, et al. An ultrasensitive method for quantitating circulating tumor DNA with broad patient coverage. Nat Med. 2014;20(5):548–54. https://0-doi-org.brum.beds.ac.uk/10.1038/nm.3519.
Razavi P, Li BT, Brown DN, Jung B, Hubbell E, Shen R, et al. High-intensity sequencing reveals the sources of plasma circulating cell-free DNA variants. Nat Med. 2019;25(12):1928–37. https://0-doi-org.brum.beds.ac.uk/10.1038/s41591-019-0652-7.
Jaiswal S, Ebert BL. Clonal hematopoiesis in human aging and disease. Science. 2019;366. Available from: https://science.sciencemag.org/content/366/6465/eaan4673. [cited 2020 Jan 8]
Mäkinen N, Mehine M, Tolvanen J, Kaasinen E, Li Y, Lehtonen HJ, et al. MED12, the Mediator Complex Subunit 12 Gene, Is Mutated at High Frequency in Uterine Leiomyomas. Science. 2011;334(6053):252–5. https://0-doi-org.brum.beds.ac.uk/10.1126/science.1208930.
Bean GR, Joseph NM, Gill RM, Folpe AL, Horvai AE, Umetsu SE. Recurrent GNAQ mutations in anastomosing hemangiomas. Mod Pathol. 2017;30(5):722–7. https://0-doi-org.brum.beds.ac.uk/10.1038/modpathol.2016.234.
Iurlo A, Gianelli U, Beghini A, Spinelli O, Orofino N, Lazzaroni F, et al. Identification of kit(M541L) somatic mutation in chronic eosinophilic leukemia, not otherwise specified and its implication in low-dose imatinib response. Oncotarget. 2014;5(13):4665–70. https://0-doi-org.brum.beds.ac.uk/10.18632/oncotarget.1941.
Gu W, Talevich E, Hsu E, Qi Z, Urisman A, Federman S, et al. Detection of cryptogenic malignancies from metagenomic whole genome sequencing of body fluids. Zenodo; 2021 doi: https://0-doi-org.brum.beds.ac.uk/10.5281/zenodo.4697549
Gu W, Talevich E, Hsu E, Qi Z, Urisman A, Federman S, et al. Cryptogenic malignancies in body fluids. NCBI; 2021. Available from: https://0-www-ncbi-nlm-nih-gov.brum.beds.ac.uk/bioproject/?term=PRJNA707099. Access 5 Mar 2021.
We thank the members of the UCSF Clinical Microbiology, Immunology, Hematology, and Chemistry Laboratories and the Clinical Cancer Genomics Laboratory, as well as the Stanford Cytopathology, Molecular Genetic Pathology, and Clinical Genomics Laboratories for their help. We thank Drs. Edward Pham and Scott Bauer for critical feedback on this manuscript. We thank members of the Chiu, Miller, and DeRisi laboratories for their support.
This work was funded by an NIH K08 grant and Burroughs-Wellcome Award to WG, Abbott Laboratories (CYC), NIH/NHLBI grant R01-HL105704 (CYC), NIH/NIAID grant R33-AI129455 (CYC), the California Initiative to Advance Precision Medicine (CYC), and the Charles and Helen Schwab Foundation (CYC), and funding from the Department of Laboratory Medicine at UCSF.
Ethics approval and consent to participate
Archival material at UCSF was retrospectively analyzed under no-patient-contact protocols approved by the UCSF Institutional Review Board (#15-15823, #10-01116, #18-25287). A written consent given prior to the procedure used to obtain the sample covered the use of residual samples for research. Samples were originally collected for routine clinical use and not discarded. Similarly, samples at Stanford for the verification cohort were also residual material enrolled under a no-patient-contact protocol approved by the Stanford Institutional Review Board (#58461) and with a written consent prior to the procedure. All research has been performed in accordance with the Declaration of Helsinki.
Consent for publication
ET was employed by DNAnexus, Inc. during the duration of the study and by Karius, Inc. prior to publication. The remaining authors declare that they have no competing interests.
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. Body fluid samples from patients positive for malignancy by cytology and/or flow cytometry.
. Select microbiological cases that have overlapping features with cancer presentations.
. Microbiological cases - all other cases.
. Verification cohort.
. Microbiological cases with overlapping features with cancer presentations.
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Gu, W., Talevich, E., Hsu, E. et al. Detection of cryptogenic malignancies from metagenomic whole genome sequencing of body fluids. Genome Med 13, 98 (2021). https://0-doi-org.brum.beds.ac.uk/10.1186/s13073-021-00912-z