Exosomes are nano-sized extracellular vesicles released by many cells that contain molecules characteristic of their cell of origin, including microRNA. Exosomes released by glioblastoma cross the blood–brain barrier into the peripheral circulation and carry molecular cargo distinct to that of “free-circulating” miRNA. In this pilot study, serum exosomal microRNAs were isolated from glioblastoma (n = 12) patients and analyzed using unbiased deep sequencing. Results were compared to sera from age- and gender-matched healthy controls and to grade II–III (n = 10) glioma patients. Significant differentially expressed microRNAs were identified, and the predictive power of individual and subsets of microRNAs were tested using univariate and multivariate analyses. Additional sera from glioblastoma patients (n = 4) and independent sets of healthy (n = 9) and non-glioma (n = 10) controls were used to further test the specificity and predictive power of this unique exosomal microRNA signature. Twenty-six microRNAs were differentially expressed in serum exosomes from glioblastoma patients relative to healthy controls. Random forest modeling and data partitioning selected seven miRNAs (miR-182-5p, miR-328-3p, miR-339-5p, miR-340-5p, miR-485-3p, miR-486-5p, and miR-543) as the most stable for classifying glioblastoma. Strikingly, within this model, six iterations of these miRNA classifiers could distinguish glioblastoma patients from controls with perfect accuracy. The seven miRNA panel was able to correctly classify all specimens in validation cohorts (n = 23). Also identified were 23 dysregulated miRNAs in IDHMUT gliomas, a partially overlapping yet distinct signature of lower-grade glioma. Serum exosomal miRNA signatures can accurately diagnose glioblastoma preoperatively. miRNA signatures identified are distinct from previously reported “free-circulating” miRNA studies in GBM patients and appear to be superior.
Malignant gliomas, particularly glioblastoma (GBM), represent the most lethal primary brain tumors, owing in part to their highly infiltrative growth patterns. The World Health Organization (WHO) guidelines sub-categorize glioma by histopathologic evaluation into tumor grades I–IV, where GBM (grade IV) is the most aggressive and also the most common. Despite surgery, radiation, and chemotherapy, essentially all GBM tumors recur, at which point patients have reduced treatment options and worsening prognoses. Compounding this aggressive cancer phenotype are challenges in monitoring responses to treatment and tumor progression. While recent revisions to the Response Assessment in Neuro-Oncology criteria helps to standardize glioma tumor monitoring,1 radiographic measurements can be unreliable and insensitive to early signs of treatment failure and tumor relapse. Moreover, there are still difficulties deciphering pseudo-progression and pseudo-responses in some patients. Brain biopsy and histologic analysis can provide definitive diagnoses and evaluation of disease progression; however, serial biopsies are impractical given the cumulative surgical risk, and biopsied tissue may not reflect the heterogeneity of GBM tumors.
An important step toward the provision of personalized GBM patient care is the ability to assess tumors in situ. As such, there is a real need for biomarkers that can measure disease burden and treatment responses in GBM patients in a safe, accurate, and timely manner and preferably before changes become clinically apparent. The recently popularized idea of “liquid biopsy” presents an ideal approach to monitor GBM tumor load and evolution in response to treatment. If developed and implemented alongside new treatments, such tests would provide useful surrogate endpoints and allow clinical trial protocols to be more dynamic and adaptive.
Exosomes are nano-sized (30–100 nm) membrane-bound extracellular vesicles released by all cells in both health and disease, and there is growing interest in their use as non-invasive biomarkers for disease diagnosis and monitoring of disease recurrence.2 GBM-derived exosomes circulate in the peripheral blood of patients and can contain diagnostic nucleic acid.3 We recently described GBM exosome protein signatures4,5 and also showed that GBM exosomes contain abundant, selectively packaged small non-coding RNAs (sncRNAs).6 Using unbiased sncRNA deep sequencing, we identified several unusual and/or completely novel sncRNAs within GBM exosomes in vitro as well as an enrichment of microRNA (miRNA) implicated in oncogenesis, including miR-23a, miR-30a, miR-221, and miR-451.6 Thus, while GBM exosomal miRNA contents broadly reflect their cell of origin, there is a unique profile of miRNAs within exosomes.
Some studies of exosomal miRNA in GBM patients have already been reported; these studies utilized methods that focused on predefined and relatively small groups of miRNA species. One previous study found that miR-21 levels in cerebrospinal fluid exosomes of GBM patients were upregulated ten-fold compared to controls,7 while another reported that serum exosomal miR-320, miR-547-3p, and RNU6-1 were significantly associated with GBM diagnosis, as well as outcome (RNU6-1).8 However, to date no comprehensive analysis of the entire miRNA repertoire of serum exosomes in glioma patients has been performed. Here we have used unbiased next-generation sequencing and an integrative bioinformatics pipeline9 to assay the complete repertoire of exosomal-associated miRNAs in the serum of patients with GBM, lower-grade gliomas, and healthy controls. We describe a novel miRNA signature within serum exosomes that is highly predictive of preoperative GBM diagnosis. Furthermore, we show that this approach has the potential for describing unique miRNA signatures for distinct glioma entities.
Characterization of serum exosomes isolated prior to miRNA sequencing
Serum exosomes were isolated by size exclusion chromatography. The combined elution fractions 8–10 showed particle sizes with a mean diameter 89.1 ± 2.5 nm and modal diameter of 81.7 ± 5.5 nm (Fig. 1a). Transmission electron microscopy (TEM) confirmed the presence of similarly sized particles with vesicular morphologies, characteristic of exosomes (Fig. 1b). Mass spectrometric analysis confidently identified 1167, 861, and 636 proteins in qEV elution fractions 8, 9, and 10 from healthy serum, respectively (Supp. Table 2). Overall, 87 of the top 100 proteins commonly identified in exosomes were confidently sequenced across the three fractions, including all top 10 exosomal proteins (Fig. 1c-1). Primary sub-cellular localizations included significant enrichments of “exosome” and “blood microparticle” related proteins across all fractions, with minimal contamination from other compartments, including the nucleolus (Fig. 1c-2) where certain miRNAs show specific nuclear enrichment.10 Prior to RNA extraction, serums were treated with RNaseA to remove circulating RNAs that may confound measurements of exosomal RNAs.9 RNA extracted from each sample yielded profiles typical for exosomes, showing an absence of ribosomal RNA and enrichment of small ( <200 nt) RNA species (Fig. 1d).
Differentially expressed exosomal miRNAs in GBM patient sera
Circulating exosomal miRNA profiles from patients with histopathologically confirmed IDHWT GBM (n = 12) were compared to age- and gender-matched healthy controls (n = 12; see Table 1 for discovery cohorts and Table 2 for validation cases). We employed three statistical approaches (Student’s t test, Fisher’s exact, Wilcoxon rank sum) to identify a discovery set of differentially expressed miRNA biomarkers. miRNA biomarkers were identified if their differential expression met a fold change ≥2 in either direction and unadjusted p values ≤0.05 in all statistical tests applied. Using this approach, we identified 26 miRNAs significantly dysregulated between healthy controls and GBM patients (Table 3; Fig. 2a; normalized miRNA counts are available in Supp. Table 3 and differential expression analysis in Supp. Table 4A).
Functional analysis of dysregulated miRNAs in GBM
We explored biological and canonical pathways associated with exosomal miRNAs changing in GBM patient sera relative to healthy controls. The identities of 44 miRNAs (p value ≤ 0.05 in all three tests; no fold change restriction) were uploaded into the Ingenuity Pathway Analysis environment to analyze molecular pathways overrepresented in their targets. The dysregulated miRNAs target mRNAs that are significantly associated with “cancer” (1.96E−06 < p -value < 1.52E−16) and “neurological disease” (1.72E−06 < p -value < 8.76E−13) with around half of targeted mRNAs implicated in GBM (p value = 3.36E−12) and glioma signaling pathways (p value = 1.25E−09; Fig. 2b, Suppl. Fig. 1).
Selection of signature miRNA classifiers for preoperative GBM diagnosis
The predictive power of each miRNA was estimated using logistic regression (LR) models, in which individual miRNA expression profiles were used as predictors. Receiver operator characteristic (ROC) curves were determined and area under the ROC curve (AUROC) measures were ≥0.74 across the 26 dysregulated miRNAs. The 95% confidence intervals (CIs) corresponding to AUROC estimates did not contain the null hypothesis value (AUROC = 0.5 for a random prediction), indicating that all 26 miRNAs are statistically accurate univariate diagnostic predictors of GBM (Table 2; Supp. Fig. 2). In silico validation by leave-one-out cross-validation (LOO-CV) correctly identified the test sample on average 83% of the time (range 77–89%). We then used partitioning (70% training and 30% test) and Random Forest (RF) multivariate modeling to determine whether expression patterns of a subset of differentially expressed miRNAs could improve the predictive power. Using these methods, seven miRNAs (miR-182-5p, miR-328-3p, miR-339-5p, miR-340-5p, miR-485-3p, miR-486-5p, and miR-543) distinguished GBM patients from healthy subjects in >75% of the random data partitions and were selected as the most “stable” miRNA classifiers (Fig. 3a, b). The RF model was repeated using all iterations of the seven most stable miRNAs and achieved an overall predictive power of 91.7% for classifying GBM patients from healthy controls (Fig. 3c). The diagnostic efficiencies of all possible combinations of the seven miRNAs were determined using AUROC measures along with the corresponding 95% CIs (Fig. 3d; Supplementary Table 5). Strikingly, six miRNA combinations were able to distinguish GBM patients from healthy controls with perfect accuracy (Fig. 3e).
To assess the temporal stability of the GBM miRNA signature in the same patients, we tested preoperative sera collected at a GBM recurrence (GBM1 patient relapsed and required additional surgery after 8 months) and from an earlier GBM lesion (excised 4.6 months before GBM12; Table 1B). Using the panel of seven exosomal miRNAs, both GBM1-relapse and GBM12-prior were classified as GBM, in line with diagnostic histopathology. We also tested two independent samples, including a patient diagnosed with IDHMUT GBM (GBM13) and a patient diagnosed with “high-grade glioma” based on repeat magnetic resonance imagings and overall survival of 8.1 months (GBM14; see Table 1B). Both GBM13 and GBM14 were classified as GBM using the miRNA panel.
To further test the specificity of the GBM miRNA signature, we assessed its ability to distinguish GBM patients from additional healthy subjects and non-glioma disease controls. The panel accurately classified all additional healthy subjects (n = 9; Table 1B) as well as a patient with ganglioglioma WHO (2016) grade I, a slow-growing, benign brain tumor with glioneuronal components (GIC-1). Next, we assessed the impact of neuroinflammatory disease processes on the specificity of our exosomal miRNA panel ability. The bioinformatics analysis above showed that dysregulated miRNAs also target mRNAs significantly associated with autoimmune rheumatoid arthritis and broadly with “neurological disease” (Fig. 2b). Our GBM miRNA panel was used to discriminate patients with the inflammatory autoimmune disease, multiple sclerosis (MS). Sera were sampled from MS patients with active gadolinium enhancing demyelinating lesions, either untreated or receiving immunomodulatory therapies (n = 9; Table 1B). All MS patients were classified as controls, indicating the robustness of our exosomal miRNA signature for GBM identification.
miRNAs dysregulated in IDH-mutant grade II–III gliomas provide additional markers for glioma severity and IDH mutational status
We then compared serum exosome miRNA profiles between IDHMUT grade II-III glioma patients (n = 10; mean age = 42.7) and matched healthy controls (n = 10; mean age = 42.9 years; see Table 1B) and identified 23 differentially expressed miRNAs (fold change ≥2; unadjusted p < 0.05 in all three tests; Supp. Table 4b). Of these, 12 miRNAs were shared with the GBM analysis and showed the same direction of change (Fig. 4a). AUROC curve measures were ≥0.78 (average 0.88) across the 23 dysregulated miRNAs, and LOO-CV correctly identified the test sample on average 83% of the time (range 77–88%; Supp. Table 5a; Supp. Fig. 3a-b). RF modeling performed on partitioned data selected miR-7d-3p, miR-98-5p, miR-106b-3p, miR-130b-5p, and miR-185-5p as the most stable features for classifying grade II–III glioma patients from healthy participants, with a predictive power of 75.0% (Fig. 4c-1; Supp. Fig. 3c). The most stable miRNAs for classifying GII-III IDHMUT from healthy controls were distinct from GBM IDHWT signature miRNAs (Fig. 4b-1, b-2).
The sncRNA data was further interrogated to ascertain whether a subset of miRNAs showed potential for distinguishing glioma disease severity or IDH mutational status. Direct comparisons between GBM IDHWT and GII–III IDHMUT patients revealed 13 differentially expressed miRNAs (fold change ≥2; unadjusted p < 0.05 in all three tests; (Fig. 4c-1; Supp. Table 4c). AUROC curve measurements were ≥0.78 (average 0.84) across the 13 dysregulated miRNAs and LOO-CV correctly identified the test sample on average 80% of the time (range 76–86%; Supp. Table 5b; Supp. Fig. 4a-b). Numbers of significant miRNA were too few to perform partitioning, so a single RF model was constructed from all 13 dysregulated miRNAs that showed an estimated predictive power of 77.4% (Fig. 4c-2) Interestingly, three of the top four features that discriminate GBM IDHWT from GII–III IDHMUT are members of the GBM miRNA signature (i.e., miR-543, miR-485-3p, and miR-486-3p), changing only in GBM patient sera relative to healthy participants (indicated by asterisks in Fig. 4).
Using unbiased high-throughput next-generation sequencing and an integrative bioinformatics pipeline,9 we have identified differentially expressed serum exosomal miRNAs that discriminate GBM patients from healthy controls. Machine-learning approaches on miRNAs were used to examine their individual and shared predictive abilities for a preoperative GBM diagnosis via a blood test. Of the 26 differentially expressed miRNAs in GBM patients’ relative to healthy controls, we selected a stable signature panel of seven miRNAs. Together, the expression levels of miR-182-5p, miR-328-3p, miR-339-5p, miR-340-5p, miR-485-3p, miR-486-5p, and miR-543 predicted a preoperative GBM diagnosis with a 91.7% accuracy. Within this multivariate model, a combination of just four miRNAs (miR-182-5p, miR-328-3p miR-485-3p, miR-486-5p) distinguished GBM patients from healthy controls with perfect accuracy (100.0%).
There have been multiple studies examining “free-circulating” miRNAs in glioma patients with varying success. A recent meta-analysis of these studies found the specificity and sensitivity of circulating miRNAs to be 0.87 and 0.86, respectively, while noting the large heterogeneity of circulating miRNAs within the included studies.11 The heterogeneity is likely due to differences in data normalization used in quantitative reverse transcriptase–PCR studies, with no universally accepted endogenous housekeeping control.11 Interestingly, the majority of miRNAs identified in our exosomal signature have not been previously identified in “free-circulating” studies. This is consistent with the notion that exosomes represent a distinct pathway of nucleic acid release from cells and contain selectively packaged miRNA species.6 We have previously shown the effects of RNAse pretreatment of serum prior to exosome isolation, as performed in this study, drastically alters the miRNA profiles identified, presumably due to eradication of co-precipitated “free-circulating” miRNAs.9 Moreover, normalization of deep sequencing data is not dependent on comparison to a reference signal or housekeeping gene, potentially reducing variability in data analysis.
Functional pathway analysis of mRNA species targeted by exosomal miRNAs dysregulated in GBM patient sera showed highly significant associations with specific GBM molecular pathways. This provides confidence that the miRNA biomarkers resolved by our methods are relevant to this particular disease setting. Previous studies have identified roles for all seven GBM miRNA classifiers in various aspects of glioma and GBM biology. miR-182, detected here in significantly higher levels in GBM sera, was proposed as a marker of glioma progression, critical for glioma tumorigenesis, tumor growth, and survival in vitro,12,13 with high miR-182 tissue expression observed in GBM14 and associated with poor overall survival.15 Also in line with observations here, the upregulation of miR-486 was shown to promote glioma aggressiveness both in vitro and in vivo.16 Exosomal miRNAs identified with lower expression levels in GBM patient sera are also substantiated by the literature. Functional assays indicate tumor-suppressive roles of miR-328,17 miR-340,18,19 miRNA-485-5p,20 and miR-54321 with low levels observed in tumor tissues relative to normal brain17,19,20,21 and low tissue expression levels significantly associated with poor patient outcomes.17,19 While miR-339 (decreased levels in GBM patients here) was shown to contribute to immune evasion of GBM cells by modulating T cell responses,22 inhibitory roles for miR-339 were reported in acute myeloid leukemia,23 hepatocellular carcinoma,24 gastric,25 colorectal,26 breast,27 and ovarian cancers.28
The GBM miRNA signature was able to accurately classify all additional specimens in the validation sets (healthy, n = 9; non-glioma, n = 10), including patients with gadolinium enhancing active demyelinating lesions. Tumefactive demyelination is a well-recognized mimic of GBM.29 The GBM signature also correctly classified four additional GBM specimens, including two serial collections from patients within the discovery cohort as well as two independent patients. This pilot study utilized a relatively small patient group, and further testing is needed to determine whether the miRNA panel can reliably diagnose GBM in large, independent patient cohorts. Moreover, the correlation between a positive GBM classification and tumor burden needs to be addressed. To this end, longitudinal studies should be pursued to assess whether the GBM miRNA panel can detect time critical GBM tumor recurrences.
There is more than one pathological route to a GBM; primary and secondary GBMs are distinct entities with IDH mutations considered a genetic signpost.30 The only patients where early detection of a GBM tumor is likely are arguably those with diffuse and anaplastic (grade II–III) gliomas who progress with a secondary GBM recurrence (IDHMUT). Accordingly, the identification of reliable and readily accessible circulating progression markers is an important step toward precision medicine for patients diagnosed with low-grade gliomas. While the GBM miRNA signature was described in serum exosomes from IDHWT GBM patients, it was also able to categorize a patient with IDHMUT GBM (GBM13) from healthy participants. It is worth noting that miRNA members of the GBM signature panel (specifically, increased miR-182-5p, decreased miR339-5p and miR-340-5p) were also identified in the IDHMUT GII–III comparative analysis. Whether these miRNA changes are related to IDH mutational status, glioma grade, or a combination of the two cannot be delineated here. However, our multivariate modeling did identify distinct panels of miRNAs for classifying GBM and glioma patients from their corresponding matched healthy control cohorts. Moreover, three GBM signature panel miRNAs that were unique to the GBM vs control comparative analysis (increased miR-486-5p and decreased miR-485-3p and miR-543) were among the top four features that distinguish GBM IDHWT from GII–III IDHMUT and therefore might be specific for GBM IDHWT (indicated by asterisks in Fig. 4). These encouraging results demonstrate the potential for exosomal miRNA profiles to be used for glioma subtyping and grading, including the determination of mutational states. Expansion of these discovery analyses to include well-defined cohorts of glioma subtypes with sufficient n will likely resolve biomarkers of more nuanced specificity.
In summary, we have described a serum exosomal miRNA signature that can accurately predict a GBM diagnosis, preoperatively. This pilot study demonstrates that exosomal-associated miRNAs have exceptional utility as biomarkers in the glioma disease setting. If these exosomal biomarkers are able to offer non-invasive, early indications of tumor progression and/or recurrence, they are likely to have significant clinical utility. These exciting findings have significant potential to transform current diagnostic paradigms, as well as provide distinct surrogate endpoints for clinical trials. Assessment of serum exosomal miRNAs in larger longitudinal cohorts of patients with GBM are required to definitely determine their utility in clinical practice, and these studies are currently underway.
Serum (1 mL) was accessed from the Neuropathology Tumor and Tissue Bank at Royal Prince Alfred Hospital, New South Wales, Australia (Sydney Local Health District HREC approval, X014-0126 & HREC/09RPAH/627). Twenty-six serum specimens were collected preoperatively from patients with histologically confirmed glioma tumors, including 16 with GBM, IDH-wild-type (IDHWT) WHO (2016) grade IV and 10 patients with grade II–III IDH-mutant (IDHMUT) gliomas (refer to Table 1; Supp. Table 1 for more detailed information). Age- and gender-matched healthy control sera (n = 16) were used for discovery miRNA analyses. Sera from an additional 9 healthy controls and 10 non-glioma patients (including active MS, n = 9 and ganglioglioma, n = 1) were used to test the GBM miRNA signature. This study was performed under RPAH, and USYD HREC approved protocols (#X13-0264 and 2012/1684), and all participants provided written informed consent. All methods were performed in accordance with the relevant guidelines and regulations.
Exosome purification and characterization
Exosomes were isolated from serum as previously described.9 Briefly, serum (1 mL from each subject) was treated with RNase A (37 °C for 10 min; 100 ng/mL; Qiagen, Australia) before exosome purification by size exclusion chromatography (qEV iZONE Science). Ten fractions (500 μL) were eluted in phosphate-buffered saline, as per the manufacturer’s instructions. Fractions 8–10 were previously shown to contain purified exosome populations9 and were collected and stored at −80 °C. Captured exosomes were characterized in accordance with the criteria outlined by the International Society for Extracellular Vesicles.31 Specifically, we identified more than three exosome-enriched proteins by mass spectrometry (MS) proteome profiling and characterized vesicle heterogeneity using two technologies, TEM, and nanoparticle tracking analysis (NTA).
Transmission electron microscopy
Combined qEV-captured fractions 8–10 were loaded onto carbon-coated, 200 mesh Cu formvar grids (#GSCU200C; ProSciTech Pty Ltd, QLD, Australia), fixed (2.5% glutaraldehyde, 0.1 M phosphate buffer, pH7.4), negatively stained with 2% uranyl acetate for 2 min, and dried overnight. Exosomes were visualized at ×40,000 magnification on a Philips CM10 Biofilter TEM (FEI Company, OR, USA) equipped with an AMT camera system (Advanced Microscopy Techniques, Corp., MA, USA) at an acceleration voltage of 80 kV.
Nanoparticle tracking analysis
Particle size distributions and concentrations were measured by the NTA software (version 3.0) using the NanoSight LM10-HS (NanoSight Ltd, Amesbury, UK), configured with a 532-nm laser and a digital camera (SCMOS Trigger Camera). Video recordings (60 s) were captured in triplicate at 25 frames/s with default minimal expected particle size, minimum track length, and blur setting, a camera level of 10 and detection threshold of 5.
Proteome analysis of exosomal preparations
Serum exosome fractions 8–10 were prepared for MS-based proteomic analysis. Proteomes were concentrated using chloroform–methanol precipitation, dissolved in 90% formic acid (FA), their concentrations estimated at 280 nm using a Nanodrop (ND-1000, Thermo Scientific, USA), and aliquots dried using vacuum centrifugation. Proteomes were then processed and quantified as before.32 Peptides from each fraction were desalted using C18 ZipTipsTM, concentrations estimated by Qubit quantitation (Invitrogen), dried by vacuum centrifugation, and re-suspended in 3% acetonitrile (v/v)/0.1% FA (v/v). Samples (0.5 μg) from exosome elution fractions 8–10 were separated by nanoLC using an Ultimate nanoRSLC UPLC and autosampler system (Dionex) before analyzed on a QExactive Plus mass spectrometer (Thermo Electron, Bremen, Germany) as previously described.32 MS/MS data were analyzed using Mascot (Matrix Science, London, UK; v2.4.0) with a fragment ion mass tolerance of 0.1 Da and a parent ion tolerance of 4.0 PPM. Peak lists were searched against a SwissProt database (2017_11), selected for Homo sapiens, trypsin digestion, max. two missed cleavages, and variable modifications methionine oxidation and cysteine carbamidomethylation. Exosome proteins were annotated using Vesiclepedia (http://microvesicles.org)33 and Functional Enrichment Analysis Tool (FunRich; v2.1.2; http://funrich.org).34
RNA extraction and small RNA sequencing
Serum exosomes were processed for RNA extraction using the Plasma/Serum Circulating & Exosomal RNA Purification Mini Kit (Norgen Biotek, Cat. 51000) according to the manufacturer’s protocol. Extracted total RNA samples were analyzed with a Eukaryote Total RNA chip on an Agilent 2100 Bioanalyzer (Agilent Technologies, United States) to confirm sufficient yield, quality, and size of RNA. Exosome RNA sequencing libraries were then constructed using the NEBNext Multiplex Small RNA Library Prep Kit for Illumina (BioLabs, New England) according to the manufacturer’s instructions. Yield and size distribution of resultant libraries were validated using Agilent 2100 Bioanalyzer on a High-sensitivity DNA Assay (Agilent Technologies, United States). Libraries were then pooled with an equal proportion for multiplexed sequencing on Illumina HiSeq. 2000 System at the Ramaciotti Centre for Genomics.
Data preprocessing, differential expression analysis, and pathway analysis
Data preprocessing was performed using a pipeline comprising of adapter trimming (cutadapt), followed by genome alignment to human genome hg 19 using Bowtie (18 bp seed, 1 error in seed, quality score sum of mismatches <70). Where multiple best strata alignments existed, tags were randomly assigned to one of those coordinates. Tags were annotated against mirBase 20 and filtered for at most one base error within the tag. Counts for each miRNA were tabulated and adjusted to counts per million miRNAs passing the mismatch filter. All samples achieved miRNA read counts >45,000 read counts and miRNAs with low abundance (<50 read counts across >20% of samples) were removed. Differential expression analysis was performed using three different two-sided statistical hypothesis tests including a non-parametric two-sample Wilcoxon test and two parametric tests—Student’s t test and Exact test (implemented in Bioconductor EdgeR), which tests for differences between the means of two groups of negative binomially distributed counts. Benjamini and Hochberg adjusted p values were also calculated. Data preprocessing and differential expression analysis were performed using Bioconductor and R statistical packages. Pathway analysis was performed using the Ingenuity® software (Ingenuity Systems, USA; http://analysis.ingenuity.com). miRNA target filters were applied to significant, differentially expressed miRNAs (unadjusted p value ≤0.05 in all three statistical methods) and mRNA target lists were generated based on highly predicted or experimentally observed confidence levels. Core expression analyses were performed with default criteria to determine the most significant functional associations (biological and canonical pathways) of mRNAs targeted by dysregulated miRNAs.
We performed LR and ROC analysis to assess the predictive power of individual miRNAs between the two groups of interest. LR was used to identify linear predictive models with each miRNA as the univariate predictor. The quality of each model was depicted by the corresponding ROC curve, which plots the true-positive rate (i.e., sensitivity) against the false-positive rate (i.e., 1 − specificity). AUROC was then computed as a measure of how well each LR model can distinguish between two diagnostic groups. The 95% CI of AUROC measures were estimated using the Delong method35 to assess the significance of a model’s predictive power as compared to a random trial (i.e., AUROC = 0.5). We then used LOO-CV to estimate the prediction errors of the LR models. LOO-CV learns the model on all samples except one and tests the learnt model on the left-out sample. The process is repeated for each sample and the error rate is the proportion of misclassified samples. Overall, cross-validation is a powerful model validation technique for assessing how the results of a statistical analysis can be generalized to an independent dataset.36 These analyses were performed using R stats (glm) and boot (cv.glm) packages.
To assess the predictive power of multiple miRNAs as disease signatures, samples were first randomly partitioned into two disjoint sets of discovery (70% of samples) and validation (30% of samples). miRNAs differentially expressed in the discovery set (i.e., changes increased or decreased by fold change ≥2 and unadjusted p value ≤0.05 in all three statistical hypothesis tests) were then selected as features/predictors of RF multivariate predictive model. RF is a multivariate nonlinear classifier that operates by constructing a multitude of decision trees at training time in order to correct for the overfitting problem.37 RF was trained on the discovery set and the resultant predictive model was then used to predict GBM or GII–III patients vs healthy controls based on the read count values of identified miRNAs in validation samples. For statistical rigour, to account for random partitioning of the samples into discovery and validation sets, the whole process was repeated 100 times. We then chose stable miRNAs—i.e., those identified to be differentially expressed in >75% of iterations—as predictors of an RF model using all samples and the AUROC with 95% CI as well as out-of-bag error was reported as an unbiased estimates of the model predictive power. The “importance” or relative contribution of each feature (differentially expressed miRNAs) in the RF performance was then estimated based on the “mean decrease accuracy” measure as discussed in ref. 38. All analyses were performed using R “caret” and “RandomForest” packages.
This article was previously published as a preprint on bioRxiv https://doi.org/10.1101/342154
Exosomal miRNA raw data are accessible at NCBI Gene Expression Omnibus (GEO accession no. GSE122488). All R codes used in this study are available at https://github.com/VafaeeLab/glioblastoma_exosomal_miR_markers. Normalized data used for statistical analysis are provided in Supplementary Table 3.
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Many thanks to the wonderful and dedicated staff at RPAH, with special thanks to Mary Lordan, Jane Raftesath, Audrey Caudon, Shu Wang, and Ladan Noroozi. We thank the Neuropathology Tumor and Tissue Bank at Royal Prince Alfred Hospital and MS clinic at the Brain and Mind Centre for the provision of blood specimens and associated information. This work was enabled by access to several facilities of the University of Sydney, including the Bosch Institute Molecular Biology Facility, Sydney Mass Spectrometry, and Advanced Microscopy Facility. This work was supported by grants provided by Brainstorm, Brain Foundation and Pratten Foundation as well as career support from Australian Postgraduate Awards (to S.E. and S.H.), Australian Rotary Health Postgraduate Award (S.H.), and Cancer Institute New South Wales (K.L.K.).