Sporadic Creutzfeldt-Jakob disease (sCJD) presents as a rapidly progressive dementia which is usually fatal within six months. No clinical blood tests are available for diagnosis or disease monitoring. Here, we profile blood microRNA (miRNA) expression in sCJD. Sequencing of 57 sCJD patients, and healthy controls reveals differential expression of hsa-let-7i-5p, hsa-miR-16-5p, hsa-miR-93-5p and hsa-miR-106b-3p. Downregulation of hsa-let-7i-5p, hsa-miR-16-5p and hsa-miR-93-5p replicates in an independent cohort using quantitative PCR, with concomitant upregulation of four mRNA targets. Absence of correlation in cross-sectional analysis with clinical phenotypes parallels the lack of association between rate of decline in miRNA expression, and rate of disease progression in a longitudinal cohort of samples from 21 patients. Finally, the miRNA signature shows a high level of accuracy in discriminating sCJD from Alzheimer’s disease. These findings highlight molecular alterations in the periphery in sCJD which provide information about differential diagnosis and improve mechanistic understanding of human prion diseases.
Sporadic Creutzfeldt–Jakob disease (sCJD) is a transmissible neurodegenerative condition, which typically develops in late middle age, is currently untreatable, and usually results in death within six months of symptom onset. Its characteristic pathological features are the development of spongiform change in the cerebral grey matter associated with deposition of abnormal forms of prion protein (PrP)1. sCJD is thought to be caused by the spontaneous formation of prions, an infectious agent comprised of multimeric assemblies of misfolded PrP2,3. Susceptibility to, and progression of, the disease is known to be strongly influenced by a common polymorphism at codon 129 of the prion protein gene (PRNP)4,5, and additionally, several different strains of misfolded PrP are known to exist which can influence the course of the disease6. Prions are highly concentrated in brain tissue at post mortem examination of sCJD, but are also detectable in peripheral tissues, with no apparent biological consequences7,8,9,10. Specific diagnostic tests are available including brain magnetic resonance imaging (MRI) and cerebrospinal fluid (CSF) analyses; however, no simple blood assay has been developed. Here, we investigate blood microRNA (miRNA) profiles to explore whether these would disclose accessible biomarkers or insights into the peripheral pathobiology of the most common human prion disease.
Small non-coding RNAs, such as miRNAs, are highly conserved oligonucleotides (19–22 bases), which can inhibit translation of targeted messenger RNA (mRNA) transcripts and tag them for degradation11. miRNAs are powerful regulators of gene expression because one miRNA can target multiple coding genes. Due to their remarkable stability in body fluids12, miRNAs represent attractive biomarkers and drug targets, and their dysregulation has been widely described in disease states13,14,15. Moreover, since miRNAs in blood often originate from other tissues, the study of miRNAs can provide insights into pathological mechanisms in inaccessible tissues such as the brain12. miRNAs have been extensively studied in Alzheimer’s disease (AD), Parkinson’s disease (PD), Huntington’s disease (HD) and Amyotrophic lateral sclerosis (ALS)16,17,18,19.
In prion disease, only a few studies have investigated the contribution of miRNAs to disease initiation and progression, and most of the work has focused on animal models and brain tissue, limiting existing knowledge in humans to the end-stage of the disease20. Recently, Slota et al.21 profiled serum miRNAs in chronic wasting disease, a prion disease of deer, demonstrating their potential as biomarkers in animals. Here, we profile miRNA expression levels in whole blood by case–control study. Small RNA-sequencing (RNA-seq) identifies four differentially expressed (DE) miRNAs. Using quantitative PCR (qPCR) in an independent cohort, we validate and replicate the finding that hsa-let-7i-5p, hsa-miR-16-5p and hsa-miR-93-5p are downregulated in sCJD. To gain further insight into the potential use of the signature in differential diagnosis, we measure levels of these miRNAs in whole blood from patients with AD, and show that the miRNA signature differentiates sCJD from AD with a high level of accuracy. We also observe that expression of downstream mRNA targets of these miRNAs are affected in sCJD blood. Further, by interrogating 50 longitudinal samples from a group of 21 sCJD patients, we show that the rate of change of DE miRNA expression does not correlate with the rate of disease progression.
Small RNA-seq identifies five DE miRNAs in sCJD blood
To investigate whether miRNA profiles could discriminate patients with sCJD from healthy controls, we designed a case–control study using blood from 57 sCJD cases and 48 controls (Table 1). Using next-generation sequencing, we measured expression of miRNAs in all samples. Across all sequencing runs, the mean percentage of clusters passing filter was 84.43%, and the mean percentage of bases with Q > 30 was 84.80%. Across all samples, 94.73% of reads were successfully aligned to the genome, and 94.72% of these reads aligned uniquely. The mean Q score for aligned reads was 36.6. After alignment, quantification and normalisation of reads, 866 unique miRNAs were detected. To represent the overall expression pattern of the miRNAs in all 105 samples, we performed principal component analysis (PCA) (Supplementary Fig. 1).
A total of 101 miRNAs that passed low expression filtering were analysed for differential expression (Supplementary Data 1). Figure 1a and Supplementary Data 1 show that four miRNAs were found to have a statistically significant fold change (FC) between cases and controls after false discovery rate (FDR) correction for multiple testing. Figure 1b shows that hsa-miR-16-5p (FC −2.76, adjusted p = 1.48 × 10−4), hsa-miR-93-5p (FC −2.34, adjusted p = 0.001), hsa-miR-106b-3p (FC −1.74, adjusted p = 0.008) and hsa-let-7i-5p (FC −2.49, adjusted p = 0.011), were downregulated in sCJD compared to healthy controls. hsa-let-7d-3p was also included because its levels were elevated in sCJD blood, albeit with borderline significance (FC 1.94, adjusted p = 0.053). Age was included as a covariate in the regression test, although none of these five miRNAs showed a significant correlation with age in controls. Because sCJD does not alter blood cell counts22, normalisation of the sequencing data using cell count data was not done. Although the RNA we were able to obtain for a proportion of sCJD patients in our study was sub-optimal for mRNA analysis in terms of RNA integrity number (RIN), miRNA is highly resistant to degradation23. An independent analysis of the small RNA-seq data, excluding RNA samples where RIN < 4, did not alter the findings reported here (Supplementary Table 1). Because a small number of the sCJD cases had a ‘probable’ diagnosis rather than definite (Table 1), we also carried out a third analysis in which we excluded these three ‘probable’ patients (Supplementary Table 2). This did not affect the findings. Finally, 36 samples (14 sCJD cases and 22 controls) yielded more than 1.5 million reads. Given that a small number of miRNAs make up the majority of read counts in blood, we analysed these 36 samples in order to take lower abundance miRNAs into account. This added another 30 miRNAs to the list of those tested for differential expression between sCJD and controls. None of these low abundance miRNAs were significantly differentially expressed in this analysis (Supplementary Table 3). We therefore only followed up the five above-mentioned miRNAs in our downstream analyses.
Unsupervised hierarchical clustering analysis using these five differentially expressed miRNAs yielded two major clusters of samples, with most healthy individuals clustering tightly together (Fig. 1c). When the data were stratified based on PRNP codon 129 (either MM, MV or VV) (Supplementary Fig. 2) or PrPSc strain type (the prion protein disease isoform typed by the London classification, types 2 or 3, n = 22), no significant differences were observed, suggesting that these factors have little or no effect on expression of these miRNAs.
In a subset of the 866 detected miRNAs with sufficient data for analysis (including those excluded from differential expression analysis by the low expression filter), expression in sCJD patients was tested for correlation with clinical parameters (age of onset, duration of disease, MRC Scale score and MRC Scale slope). No significant associations were observed after correction for multiple testing.
The sCJD DE signature is replicated in an independent cohort
Having identified a blood-based miRNA signature for sCJD, we aimed to validate and replicate these results using an independent cohort and technique. The replication cohort comprised 29 sCJD patients and 30 healthy age and sex-matched control individuals (Table 1). Reverse transcription quantitative PCR (RT-qPCR) was used to measure the relative levels of expression of the five differentially expressed miRNAs. hsa-miR-484, which was not differentially expressed in the discovery study (FC 1.13, adjusted p = 0.521), was also included. Having determined that levels of endogenous controls did not vary between cases and controls (Supplementary Fig. 3d), we used RNU6-2, SNORD42B, SNORD95 and SNORD72 to normalise miRNA expression levels. Lower levels of hsa-let-7i-5p, hsa-miR-16-5p and hsa-miR-93-5p were found in sCJD blood, whilst hsa-miR-484 remained unchanged as expected (Fig. 2a; Supplementary Fig. 3a–c), thereby replicating the findings from the discovery study. Of the remaining two miRNAs tested, hsa-miR-106b-3p amplified poorly, while hsa-let-7d-3p was not replicated (Fig. 2a; Supplementary Fig. 3a–c).
miRNA targets are altered in blood from sCJD patients
Next, we hypothesised that if differential miRNA expression has a role in the peripheral pathophysiology of sCJD, relevant mRNA targets should also be altered in sCJD blood. We identified these mRNA targets using TarBase with stringent criteria (validated using luciferase assays and/or validated by immunoprecipitation; expressed in whole blood) (Supplementary Table 4). Using RT-qPCR, we measured the expression of six transcripts reported to be under the control of hsa-let-7i-5p, hsa-miR-16-5p and hsa-miR-93-5p in the replication cohort: CCND3, VEGFA, NAP1L1, ZFP36, CDKN1A and RNF44. Figure 2b shows that blood samples from sCJD patients display higher levels of four of these transcripts in comparison to blood from controls, which is consistent with a reduction of miRNA silencing of target mRNA. Mean endogenous control Ct values showed no significant differences between control and sCJD groups (Supplementary Fig. 4). Finally, to gain insight into biological processes by which these miRNAs may contribute to sCJD, we performed pathway enrichment analysis using the six targets of the differentially expressed (DE) miRNAs and found no significant enrichment. Altogether, these results demonstrate that hsa-let-7i-5p, hsa-miR-16-5p and hsa-miR-93-5p are downregulated in sCJD blood, and concomitantly, levels of their selected mRNA targets are elevated.
let-7i, miR-16 and miR-93 downregulation is specific to sCJD
To further investigate the relevance of this blood-based miRNA signature to sCJD, we next set out to profile levels of hsa-let-7i-5p, hsa-miR-16-5p and hsa-miR-93-5p in blood collected from the first specialist assessment of patients with AD (equivalent to sampling at the first opportunity in sCJD patients). A group of 30 AD patients were matched by sex and age to the control group used for the replication analysis (Table 1). RT-qPCR data presented in Fig. 3 and Supplementary Fig. 5a–c show that in marked contrast to sCJD, hsa-let-7i-5p, hsa-miR-16-5p and hsa-miR-93-5p were upregulated in AD patients. Mean endogenous control Ct values showed no significant differences between control and AD groups (Supplementary Fig. 5d). These results demonstrate that levels of hsa-let-7i-5p, hsa-miR-16-5p and hsa-miR-93-5p in blood establish a signature, which enables discrimination between healthy controls, AD and sCJD.
Longitudinal evaluation of DE miRNA expression in sCJD blood
Although there was no cross-sectional correlation between disease metrics and DE miRNAs, we asked whether the rate of decrease in miRNA expression could be related to the speed of decline observed in individual patients with sCJD. High inter-individual variation might obscure intra-individual longitudinal effects over time. To this end, 50 bloods were collected longitudinally from 21 individuals with sCJD (Table 1; Supplementary Table 5). At time of sampling, each patient’s condition was assessed using the MRC Prion Disease Rating Scale, allowing for disease progression to be monitored (% loss of function per day by mixed effects regression). Levels of expression for hsa-let-7i-5p, hsa-miR-16-5p, hsa-miR-93-5p and hsa-miR-484 (which was found to be unaltered in sCJD blood) were quantified by RT-qPCR, and values were converted into rate of expression decline (reduction in expression per day). Figure 4a–d and Supplementary Figs. 6 and 7 show that the rate of decline in levels of hsa-let-7i-5p, hsa-miR-16-5p and hsa-miR-93-5p did not correlate with rate of disease progression (% loss of function per day).
Diagnostic potential of miRNA markers
Finally, to assess the capabilities of miRNAs to discriminate between sCJD cases and healthy controls, we applied receiver operating characteristic (ROC) analysis. Using the data from the discovery study, the normalised read count of each of the three replicated DE miRNAs was log-transformed to ensure normal distribution, and Z-scores were calculated (distance from the mean in SDs) across the 105 samples in the discovery study. This analysis was performed for each miRNA individually, and for the aggregated mean of the three sCJD-specific miRNAs (hsa-let-7i-5p, hsa-miR-16-5p, hsa-miR-93-5p). In the discovery dataset, comparing sCJD to healthy controls, the area under the curves (AUCs) ranged from 0.736 (has-let-7i-5p) to 0.762 (hsa-miR-16-5p) and reached 0.788 when all three miRNAs were combined (Fig. 5a; Supplementary Table 6). Using the same approach in the replication set, all three miRNAs aggregated performed better than each of them individually (Fig. 5b; Supplementary Table 6). Because we found that hsa-let-7i-5p, hsa-miR-16-5p and hsa-miR-93-5p were upregulated in AD patients (as opposed to downregulated in sCJD), we next performed the same analysis (i.e. comparing AD to healthy controls) using the three miRNAs individually, and aggregated. Supplementary Table 6 and Figure 5c show that AUC values ranged from 0.810 (hsa-miR-93-5p) to 0.859 (hsa-miR-16-5p) and reached 0.860 for the three miRNAs together, indicating good diagnostic discrimination. Finally, given the lack of biomarkers to specifically and selectively discriminate sCJD patients from AD patients in blood, we calculated AUCs for the sCJD versus AD comparisons. Strikingly, AUC values ranged from 0.897 (hsa-miR-93-5p) to 0.934 (hsa-let-7i-5p). Combining the 3 miRNAs together yielded AUC value of 0.924 and 100% specificity (Fig. 5d; Supplementary Table 6). These results were not only seen when normalising to RNU6-2. Similar findings were made using SNORD42B, SNORD95 and SNORD72 endogenous controls (Supplementary Figs. 8–10). Altogether, these results suggest that these blood miRNA expression markers can be used to discriminate AD from healthy controls and sCJD from AD.
Sporadic Creutzfeldt–Jakob disease, the most common human prion disease and the archetypal rapidly progressive dementia, presents with neurological and/or neuropsychiatric features, and diagnosis is supported by abnormalities of brain imaging, neurophysiology or CSF analysis. Currently available blood tests do not help to distinguish sCJD from other neurodegenerative disorders. Here, for the first time, we show replicated evidence of specific dysregulation of miRNAs in the peripheral blood of sCJD patients. Using next-generation sequencing to profile miRNA expression in peripheral blood, we identified, validated and replicated three miRNAs (hsa-let-7i-5p, hsa-miR-16-5p and hsa-miR-93-5p) whose expression is significantly lower in the blood of sCJD patients than in healthy individuals. Furthermore, we report that the levels of these three miRNAs distinguish patients with sCJD from patients with AD. These findings suggest there is a peripheral blood molecular signature in sCJD that could be explored for potential future applications as a biomarker for diagnosis.
Each dysregulated miRNA could plausibly have implications for the pathobiology of sCJD. hsa-miR-93-5p is a member of the miR-106b-25 miRNA cluster (comprising hsa-miR-106b, hsa-miR-93 and hsa-miR-25), located on chromosome 7 within the MCM7 gene. Expression of both the miR-106b-25 cluster and MCM7 (which is also downregulated in sCJD blood, Supplementary Fig. 11) is regulated by the transcription factor E2F1, a cell cycle regulator, which has been associated with neurotoxicity in neurodegenerative disease24,25,26. In the discovery cohort, the other two members of the cluster, hsa-miR-106b-3p and hsa-miR-25-3p, were also downregulated in sCJD patients. However, expression of hsa-miR-106b-3p was too low to allow replication by qPCR, and the adjusted p-value for hsa-miR-25-3p fell short of significance (p = 0.125, Supplementary Data 1). Repression of this cluster has previously been shown to be required for endoplasmic reticulum (ER) stress-induced apoptosis, a common feature of neurodegenerative diseases27,28. It is unsurprising to find that members of this cluster are dysregulated in sCJD as alterations in hsa-miR-93-5p expression have been previously linked to AD and ALS18,29, and the prion protein gene, PRNP, has been identified as a potential target of hsa-miR-93-5p30,31,32.
hsa-let-7i-5p has also been implicated in neurodegenerative disorders. In ALS, Liguori et al.18 reported downregulation of hsa-let-7i-5p in whole blood. Conversely, in AD, elevated levels of hsa-let-7i-5p were found in brain, plasma and CSF33,34. These findings are consistent with our observations of hsa-let-7i-5p’s downregulation in sCJD blood but upregulation in AD whole blood (Figs. 2a and 3). More relevant is the report that levels of hsa-let-7i-5p were found to be elevated in exosomes from neurons of prion-infected mice35, and in sera from elk with chronic wasting disease21.
hsa-miR-16-5p features prominently in existing literature on miRNA and neurodegeneration, and prion disease in particular. Studies in prion-infected mice have shown a distinct temporal pattern of dysregulation of hsa-miR-16-5p as disease progresses, whereby expression is upregulated in cultured primary neurons in the pre-symptomatic phase but downregulated in the clinically established disease phase36,37. Recently, Slota et al.21 reported decreased miR-16-5p abundance in serum from scrapie infected hamsters. Our observations of downregulation of hsa-miR-16-5p in blood from patients with clinically established sCJD concur with these findings. In humans, Llorens and colleagues38 reported increased levels of hsa-miR-16-5p in sCJD frontal cortex. In ALS, hsa-miR-16-5p was found to be downregulated in whole blood18, and in AD, several clinical and mechanistic studies have suggested that hsa-miR-16-5p has a role in pathogenesis39,40,41. Whether altered abundance in the blood is related to the mechanism by which it is differentially expressed in neurons or in neurodegeneration remains to be investigated.
The question of whether dysregulated miRNAs are shared between neurodegenerative disorders is crucial because of the unmet need for the treatment of these diseases. Therefore, lifting the veil on molecular mechanisms involved in neurodegeneration could help provide evidence for better disease classification and drug design. Together with the literature, our results suggest that the same small group of miRNAs is consistently altered in neurodegenerative disorders, with effect size and direction of effect being tissue and disease-stage specific. miRNA profiling may, in the future, help with disease classification and diagnosis for several reasons. Firstly, because our signature allows us to clearly distinguish sCJD from AD using whole blood: the decrease in hsa-let-7i-5p, hsa-miR-16-5p and hsa-miR-93-5p in sCJD blood contrasts markedly with their upregulation in AD blood (Figs. 2a and 3), and also AD serum, CSF and brain tissue33,34,42. Secondly, because the profiles of dysregulated miRNAs are highly variable between disease stages and disease models. Kanata et al.20 recently conducted a comprehensive review of changes in miRNAs reported in mouse and primate models of prion disease. The authors pointed out that the variability in direction of effects reported could be caused by the wide variety of models studied, technologies used and tissues analysed (e.g. post mortem brain versus whole blood from living patients), as well as disease state (pre-clinical and clinical)37,38,43. Consistent with this, the sCJD miRNA signature we identified here is also found in sporadic ALS when the same tissue is analysed18. There are significant parallels between the two conditions in terms of pathology associated with deposits of aggregated misfolded protein, and heterogeneous clinical phenotypes44,45,46. The finding that dysregulated miRNAs are shared between these two diseases suggests that common mechanisms might be involved, but does not negate any potential diagnostic relevance of the sCJD signature, since the two diseases are clinically very different (ALS is predominantly a disorder of motor neurons, whilst sCJD presents with pervasive brain dysfunction). Also of note is the study from Llorens et al.38, whose findings demonstrated widespread dysregulation of miRNA levels in several brain regions affected by sCJD and implicated the miRNA biosynthesis pathway in sCJD pathogenesis.
Insights into molecular mechanisms that can contribute to the disease process may also be provided by investigation of transcripts known to be targeted by the sCJD signature: the increased expression of several hsa-let-7i-5p, hsa-miR-16-5p and hsa-miR-93-5p target genes (Fig. 2b) demonstrates that the observed downregulation of these three miRNAs in sCJD patients has concomitant effects on target gene regulation. By performing analysis of DE miRNA target-binding sequences, we excluded the possibility that the observed downregulation in miRNAs resulted from Target RNA-directed microRNA degradation (TDMD)47. Intriguingly, ZFP36 (in protein form known as tristetraprolin, TTP), which was the most highly overexpressed target gene we tested in sCJD compared with controls (Fig. 2b), is a stress granule associated RNA-binding protein which has been linked with AD pathology in mice and humans48,49.
A major strength of this study was our ability to access longitudinal samples for 21 sCJD patients, which enabled us to test for association with disease progression. Absolute expression levels of the signature did not associate with disease severity, nor did the rate of decline of expression and rate of disease progression (Fig. 4a–d; Supplementary Figs. 6a–d and 7a–d). Although the use of patient samples is desirable, it does however pose multiple caveats and limitations: confounding factors associated with disease status such as sample handling and storage prior to extraction, RNA degradation, age, environmental exposure and interactions with drugs could lead to changes in miRNA expression profiles. We addressed concerns about RNA degradation by conducting a further analysis of the discovery cohort data to show that RIN number for total RNA did not have an impact on our findings (Supplementary Table 1). This is not surprising, as miRNA is known to be highly resistant to degradation in comparison to mRNA, and therefore RIN measured from total RNA does not reflect the degradation status of miRNA23. Another potential limitation of our study is that it uses next-generation sequencing, a technology based on direct counts. Less abundant miRNAs could be missed, therefore masking some disease-specific patterns. Sequencing coverage in the discovery study is not high, but as hsa-miR-106b-3p could not be replicated by qPCR due to its low expression, inclusion of miRNAs expressed at lower levels by resequencing would have been unlikely to yield additional DE miRNAs that could be validated by qPCR. Finally, our results on the diagnostic potential of blood miRNA biomarkers remain preliminary and future work might compare their performance with that of other established blood biomarkers such as tau or NfL50,51.
Haemolysis is another potential confounding factor when profiling miRNA expression in patient blood samples52. This is because a number of miRNAs are known to be present at high levels in red blood cells, and their release could be masking disease related patterns. Here, we found that hsa-miR-484, whose levels are known to increase in hemolysed serum53, remained unchanged between sCJD and controls (both in sequencing and qPCR datasets). Our results are therefore unlikely to be caused by red blood cell contamination. Interestingly, Ludwig et al.54 recently showed that miRNAs with lower abundance in AD were enriched in monocytes and T-helper cells, while those upregulated in AD were enriched in serum, exosomes, cytotoxic t-cells and B-cells.
To our knowledge, this study is the first to evaluate the use of blood miRNA expression as biomarkers in sCJD. This study revealed diagnostic potential of blood miRNAs, and particularly high accuracy, in discriminating AD patients from healthy controls, and sCJD patients from AD. Therefore, blood miRNA expression could potentially be used as a non-invasive marker to help differentiate between prion infection and other neurodegenerative diseases in humans. Future work will look at other differential diagnoses and help establish whether miRNA profiles used in combination with other biomarkers, and demographic and clinical features, improve diagnostic accuracy in neurodegenerative diseases.
Our work was conducted in whole blood which has the advantage of being an accessible tissue, which therefore enabled us to study a large group of patients from early disease stages, and longitudinally. It will be important to establish whether the findings reported here are replicated in other tissues and body fluids such as CSF and brain tissue in order to determine whether the miRNA signature we have identified in blood is present in the brain, with potential additional effects on brain-specific mRNA targets. Based on GTEx datasets55, four of the mRNA targets of the three altered miRNAs are expressed in normal brain. Investigating the expression of both miRNAs and their targets in sCJD brain tissues will provide more evidence for a potential role in disease pathogenicity. Other future analyses might consider the impact of sex, ethnicity, co-morbidities, subtypes of disease and specific symptoms on the miRNA profile. In conclusion, our analysis of a large cohort of sCJD patients and controls has revealed that sCJD affects miRNA expression profiles in peripheral blood, and that these changes are a signal in the periphery rather than just a consequence of brain degeneration. In addition, we identified a three miRNA signature whose expression can discriminate patients with AD from controls and sCJD from AD cases. These findings provide the basis for a better mechanistic understanding of sCJD and represent an opportunity to open much needed avenues for improved disease diagnosis and therapeutic intervention.
Patients with a definite (i.e. neuropathologically confirmed) or probable diagnosis of sCJD (Table 1) according to World Health Organization criteria were recruited by the National Prion Clinic (London, UK). sCJD patients in the longitudinal cohort were participants in the UK National Prion Monitoring Cohort56. MRC Prion Disease Rating Scale scores (on a scale of 0–20, where 20 is unaffected) were derived for patients as described in Thompson et al.56, and rates of decline (% loss of function per day) calculated for patients in the longitudinal cohort according to the linear mixed model method described in Mead et al.4.
Healthy control donors were recruited from spouses or relatives of patients by the National Prion Clinic (London, UK), and the UCL Dementia Research Centre (London, UK). Patients diagnosed with AD according to International Working Group-2 criteria57 were recruited by the UCL Dementia Research Centre (London, UK) and other referrers in the UK from 2012 to 2018. The study was approved by the London—Harrow Research Ethics Committee (reference 05/Q0505/113). Samples were obtained with written informed consent from controls, patients, or a patient’s consultee in accordance with applicable UK legislation and Codes of Practice.
Sample collection and RNA extraction
Whole blood from patients and controls was collected into PAXgene tubes (PreAnalytiX, Hombrechtikon, Switzerland) and stored at −80 °C prior to RNA extraction. Total RNA was extracted from 1 ml whole blood using the Preserved Blood RNA Purification Kit II (Norgen Biotek, Thorold, Canada) followed by DNAse I digestion and concentration using RNA Clean & Concentrator-5 columns (Zymo Research, Irvine, US) according to manufacturer’s instructions. All RNA samples were subsequently run on a TapeStation 2200 (Agilent, Santa Clara, US) using High Sensitivity RNA ScreenTapes. RNA integrity number (RIN) was measured from total RNA, and samples with RIN < 2.5 were excluded from the study.
Small RNA library preparation, sequencing and analysis
Small RNA libraries were prepared from total RNA using the TruSeq Small RNA Library Prep Kit (Illumina, San Diego, US) according to the manufacturer’s instructions up to and including the PCR Amplification step. Size selection was then carried out using the PippinPrep size selection system (Sage Science, Beverly, US) with 2% dye free agarose gel cassettes with Marker L, run using the programme for 3% DF Marker F gel cassette. The upper and lower size selection thresholds were 137 and 200 bp, respectively. The eluted size fractions were concentrated using DNA Clean and Concentrator-5 columns (Zymo Research, Irvine, US). Successful library preparation and size selection was confirmed using High Sensitivity D1000 ScreenTapes and the TapeStation 2200 (both Agilent, Santa Clara, US). Libraries were normalised to 2 nM using 10 mM Tris-HCL, pH 8.5 and 12 libraries were pooled by combining equal volumes of each library. Illumina’s pooling guidelines were followed regarding index combinations. Pooled libraries were single end sequenced (120 cycles) with the MiSeq Reagent Kit v3 on a MiSeq sequencer (Illumina, San Diego, US) located in the University College London Genomics Laboratory (UCL Genomics) at the Institute of Child Health, London UK according to the manufacturer’s instructions. PhiX DNA was added to pooled libraries prior to sequencing to give a final concentration of 5% in order to increase the sequence diversity of the libraries.
Each MiSeq run was subjected to quality control (QC): successful runs were considered to have passed QC if the percentage of clusters passing filter, and average percentage of bases with quality (Q) score >30/40 both exceeded 80%, and cluster density >800 K/mm2 with even pooling. FastQ files from all MiSeq runs passing QC were uploaded into Partek Flow (Partek Inc, St. Louis, US), along with metadata. Samples yielding less than one million reads were excluded. Adapter sequences were removed and reads trimmed to a minimum length of 15 bp with a minimum quality score of 25. Reads were aligned to the human genome (hg38) using Bowtie 2 v2.2.5 with a seed length of 10 with 1 mismatch, quantified for annotated miRNAs (miRBase v21) and normalised using Cufflinks v2.2.1 default settings (total hits normalisation). Gene Specific Analysis (GSA) was carried out using a proxy for sample age, and sampling age as covariates determined by post-normalisation principal component analysis (PCA), and a lowest average coverage filter of 5000 determined using a shrinkage plot.
Relative quantification of miRNAs by quantitative PCR (qPCR)
Power calculations based on the outcome of the small RNA-seq study determined that n = 30 for both patient and control groups would be required for replication of results in an independent sample set. To this end, 10 ng total RNA from all samples was reverse transcribed using the miScript II RT Kit (Qiagen, Hilden, Germany) followed by qPCR carried out using the miScript SYBR Green PCR Kit and miScript Primer Assays (both Qiagen, Hilden, Germany) according to the manufacturer’s instructions. MiScript PCR Controls RNU6-2, SNORD42B, SNORD72 and SNORD95 were used as endogenous controls, and all samples were run in duplicate on a QuantStudio 12K Flex (Life Technologies, Carlsbad, US) with dissociation curves to check for specific amplification. Data were analysed using the ∆Ct method to generate ratios of expression of test miRNA compared to endogenous controls, and the ∆∆Ct method to generate fold changes between patient and control groups. MiScript Primer Assay reference numbers were as follows: hsa-miR-16-5p MS00031493; hsa-miR-93-5p MS00003346; hsa-let-7i-5p MS00003157; hsa-miR-106b-3p MS00008400; hsa-let-7d-3p MS00008302; hsa-miR-484 MS00004277; RNU6-2 MS00033740; SNORD42B MS00055090; SNORD72 MS00033719; SNORD95 MS00033726.
miRNA target identification and expression
Target genes for hsa-miR-16-5p, hsa-miR-93-5p and hsa-let-7i-5p were selected using TarBase v8 from DIANA tools58. Genes validated by luciferase assay were prioritised. Where no luciferase data was available (hsa-let-7i-5p), targets validated by immunoprecipitation in >5 publications were selected. Shortlisted targets for each miRNA with the highest level of expression in whole blood (GTEx, https://gtexportal.org/home/)55 were then selected for expression analysis in the replication cohort (Supplementary Table 4).
For analysis of target genes, cDNA preparation and qPCR analysis were performed as follows: 200 ng of total RNA was reverse transcribed using the QuantiTect Reverse Transcription Kit (Qiagen, Hilden, Germany) according to the manufacturer’s instructions. qPCR was then carried out using the QuantiTect SYBR Green PCR kit and QuantiTect Primer Assays (both Qiagen, Hilden, Germany) to determine the expression levels of CCND3, VEGFA, CDKN1A, ZFP36, NAP1L1, RNF44, MCM7, ACTB, B2M and ALAS1. ACTB, B2M and ALAS1 were amplified as endogenous controls and all reactions were performed in duplicate on an Applied Biosystems 7500 Real Time PCR machine (Life Technologies, Carlsbad, US) with dissociation curves to check for specific amplification. The ΔΔCt method was used for analysis. Gene expression changes are presented as a combined endogenous control relative fold change in patients compared to controls (set at 1.0). QuantiTect Primer Assays were purchased for CCND3 (hsa-miR-16-5p target), VEGFA (hsa-miR-16-5p and hsa-miR-93-5p target), CDKN1A (hsa-miR-93-5p target), ZFP36, NAP1L1 and RNF44 (hsa-let-7i-5p targets), B2M, ALAS1 and ACTB (endogenous controls), and MCM7. Qiagen reference numbers were as follows: CCND3 QT00096796; VEGFA QT01010184; CDKN1A QT00062090; ZFP36 QT00091357; NAP1L1 QT00085635; RNF44 QT00051793; MCM7 QT00053228; ACTB QT01680476; B2M QT00088935; ALAS1 QT00073122. Gene set enrichment analysis was performed using the ENRICHR program (http://amp.pharm.mssm.edu/Enrichr/)59,60.
ROC curves were plotted, and AUCs calculated, in SPSS v26 (IBM, Armonk, US) using Z-scores calculated from either log-transformed normalised small RNA-seq read counts, or from log-transformed qPCR ratios of miRNA expression measured relative to endogenous control miRNAs. For combined analysis of hsa-let-7i-5p, hsa-miR-16-5p and hsa-miR-93-5p, mean Z-scores for these miRNAs were calculated and used to plot the ROC curve. The sCJD versus AD comparison was carried out indirectly, using qPCR data from each group obtained using a common set of control samples (Figs. 2a and 3; Supplementary Figs. 3a–d and 5a–d). Youden’s indices were calculated using ROC curve coordinates, in order to determine sensitivity and specificity at the point where test performance is optimal.
Small RNA-seq differential expression p-values were adjusted for multiple testing using the Benjamini–Hochberg false discovery rate (FDR) method. miRNA expression data from the discovery cohort sCJD group was subjected to Pearson or Spearman correlation (as appropriate) with clinical parameters after first checking data for normality. Clinical parameters tested were age of onset, duration of disease, MRC Scale score and MRC Scale slope, and correlation p-values were Bonferroni-corrected for multiple testing. For miRNA and mRNA qPCR data, statistical comparisons between groups were carried out using Prism v5.03 (GraphPad, San Diego, US) by two-tailed Mann–Whitney test, or one-tailed Mann–Whitney test where there was prior knowledge of the direction of effect, e.g. for qPCR replication of discovery cohort data. Longitudinal data was analysed by linear regression using Prism.
Further information on research design is available in the Nature Research Reporting Summary linked to this article.
All sequencing data that support the findings of this study have been deposited in the National Center for Biotechnology Information Gene Expression Omnibus (GEO) and are accessible through the GEO Series accession number GSE140069. Source data are provided with this paper.
Collinge, J. Prion diseases of humans and animals: their causes and molecular basis. Annu. Rev. Neurosci.24, 519–550 (2001).
Bolton, D. C., McKinley, M. P. & Prusiner, S. B. Identification of a protein that purifies with the scrapie prion. Science218, 1309–1311 (1982).
Terry, C. et al. Ex vivo mammalian prions are formed of paired double helical prion protein fibrils. Open Biol. 6, https://doi.org/10.1098/rsob.160035 (2016).
Mead, S. et al. Clinical trial simulations based on genetic stratification and the natural history of a functional outcome measure in Creutzfeldt-Jakob disease. JAMA Neurol.73, 447–455 (2016).
Windl, O. et al. Genetic basis of Creutzfeldt-Jakob disease in the United Kingdom: a systematic analysis of predisposing mutations and allelic variation in the PRNP gene. Hum. Genet.98, 259–264 (1996).
Parchi, P. et al. Classification of sporadic Creutzfeldt-Jakob disease based on molecular and phenotypic analysis of 300 subjects. Ann. Neurol.46, 224–233 (1999).
Glatzel, M., Abela, E., Maissen, M. & Aguzzi, A. Extraneural pathologic prion protein in sporadic Creutzfeldt-Jakob disease. N. Engl. J. Med.349, 1812–1820 (2003).
Head, M. W. et al. Abnormal prion protein in the retina of the most commonly occurring subtype of sporadic Creutzfeldt-Jakob disease. Br. J. Ophthalmol.89, 1131–1133 (2005).
Orru, C. D. et al. Prion seeds distribute throughout the eyes of sporadic Creutzfeldt-Jakob disease patients. MBio9, https://doi.org/10.1128/mBio.02095-18 (2018).
Orru, C. D. et al. Prion seeding activity and infectivity in skin samples from patients with sporadic Creutzfeldt-Jakob disease. Sci. Transl. Med. 9, https://doi.org/10.1126/scitranslmed.aam7785 (2017).
He, L. & Hannon, G. J. MicroRNAs: small RNAs with a big role in gene regulation. Nat. Rev. Genet.5, 522–531 (2004).
Rayner, K. J. & Hennessy, E. J. Extracellular communication via microRNA: lipid particles have a new message. J. Lipid Res.54, 1174–1181 (2013).
Correia, C. N. et al. Circulating microRNAs as potential biomarkers of infectious disease. Front. Immunol.8, 118 (2017).
Kai, K., Dittmar, R. L. & Sen, S. Secretory microRNAs as biomarkers of cancer. Semin. Cell Dev. Biol.78, 22–36 (2018).
Viswambharan, V., Thanseem, I., Vasu, M. M., Poovathinal, S. A. & Anitha, A. miRNAs as biomarkers of neurodegenerative disorders. Biomark. Med.11, 151–167 (2017).
Abe, M. & Bonini, N. M. MicroRNAs and neurodegeneration: role and impact. Trends Cell Biol.23, 30–36 (2013).
Hebert, S. S. & De Strooper, B. Alterations of the microRNA network cause neurodegenerative disease. Trends Neurosci.32, 199–206 (2009).
Liguori, M. et al. Dysregulation of microRNAs and target genes networks in peripheral blood of patients with sporadic. Amyotroph. Lateral Scler. Front. Mol. Neurosci.11, 288 (2018).
Tan, L., Yu, J. T. & Tan, L. Causes and consequences of microRNA dysregulation in neurodegenerative diseases. Mol. Neurobiol.51, 1249–1262 (2015).
Kanata, E. et al. MicroRNA alterations in the brain and body fluids of humans and animal prion disease models: current status and perspectives. Front. Aging Neurosci.10, 220 (2018).
Slota, J. A. et al. Identification of circulating microRNA signatures as potential biomarkers in the serum of elk infected with chronic wasting disease. Sci. Rep.9, 19705 (2019).
Choi, E. M. et al. Prion proteins in subpopulations of white blood cells from patients with sporadic Creutzfeldt-Jakob disease. Lab. Invest.89, 624–635 (2009).
Jung, M. et al. Robust microRNA stability in degraded RNA preparations from human tissue and cell samples. Clin. Chem.56, 998–1006 (2010).
Giovanni, A. et al. E2F1 mediates death of B-amyloid-treated cortical neurons in a manner independent of p53 and dependent on Bax and caspase 3. J. Biol. Chem.275, 11553–11560 (2000).
Hoglinger, G. U. et al. The pRb/E2F cell-cycle pathway mediates cell death in Parkinson’s disease. Proc. Natl Acad. Sci. USA104, 3585–3590 (2007).
Ranganathan, S. & Bowser, R. Alterations in G(1) to S phase cell-cycle regulators during amyotrophic lateral sclerosis. Am. J. Pathol.162, 823–835 (2003).
Gupta, S. et al. Perk-dependent repression of miR-106b-25 cluster is required for ER stress-induced apoptosis. Cell Death Dis.3, e333 (2012).
Stefani, I. C., Wright, D., Polizzi, K. M. & Kontoravdi, C. The role of ER stress-induced apoptosis in neurodegeneration. Curr. Alzheimer Res.9, 373–387 (2012).
Dong, H. et al. Serum microRNA profiles serve as novel biomarkers for the diagnosis of Alzheimer’s disease. Dis. Markers2015, 625659 (2015).
Balakrishnan, I. et al. Genome-wide analysis of miRNA-mRNA interactions in marrow stromal cells. Stem Cells32, 662–673 (2014).
Boudreau, R. L. et al. Transcriptome-wide discovery of microRNA binding sites in human brain. Neuron81, 294–305 (2014).
Kishore, S. et al. A quantitative analysis of CLIP methods for identifying binding sites of RNA-binding proteins. Nat. Methods8, 559–564 (2011).
Lau, P. et al. Alteration of the microRNA network during the progression of Alzheimer’s disease. EMBO Mol. Med.5, 1613–1634 (2013).
Sorensen, S. S., Nygaard, A. B. & Christensen, T. miRNA expression profiles in cerebrospinal fluid and blood of patients with Alzheimer’s disease and other types of dementia - an exploratory study. Transl. Neurodegener.5, 6 (2016).
Bellingham, S. A., Coleman, B. M. & Hill, A. F. Small RNA deep sequencing reveals a distinct miRNA signature released in exosomes from prion-infected neuronal cells. Nucleic Acids Res.40, 10937–10949 (2012).
Burak, K. et al. MicroRNA-16 targets mRNA involved in neurite extension and branching in hippocampal neurons during presymptomatic prion disease. Neurobiol. Dis.112, 1–13 (2018).
Majer, A. et al. Early mechanisms of pathobiology are revealed by transcriptional temporal dynamics in hippocampal CA1 neurons of prion infected mice. PLoS Pathog.8, e1003002 (2012).
Llorens, F. et al. Regional and subtype-dependent miRNA signatures in sporadic Creutzfeldt-Jakob disease are accompanied by alterations in miRNA silencing machinery and biogenesis. PLoS Pathog.14, e1006802 (2018).
Hebert, S. S., Sergeant, N. & Buee, L. MicroRNAs and the regulation of tau. Metab. Int. J. Alzheimers Dis.2012, 406561 (2012).
Liu, W. et al. MicroRNA-16 targets amyloid precursor protein to potentially modulate Alzheimer’s-associated pathogenesis in SAMP8 mice. Neurobiol. Aging33, 522–534 (2012).
McKeever, P. M. et al. MicroRNA expression levels are altered in the cerebrospinal fluid of patients with young-onset Alzheimer’s disease. Mol. Neurobiol.55, 8826–8841 (2018).
Cheng, L. et al. Prognostic serum miRNA biomarkers associated with Alzheimer’s disease shows concordance with neuropsychological and neuroimaging assessment. Mol. Psychiatry20, 1188–1196 (2015).
Boese, A. S. et al. MicroRNA abundance is altered in synaptoneurosomes during prion disease. Mol. Cell Neurosci.71, 13–24 (2016).
Polymenidou, M. & Cleveland, D. W. The seeds of neurodegeneration: prion-like spreading in ALS. Cell147, 498–508 (2011).
Smethurst, P. et al. In vitro prion-like behaviour of TDP-43 in ALS. Neurobiol. Dis.96, 236–247 (2016).
Smethurst, P., Sidle, K. C. & Hardy, J. Review: Prion-like mechanisms of transactive response DNA binding protein of 43 kDa (TDP-43) in amyotrophic lateral sclerosis (ALS). Neuropathol. Appl. Neurobiol.41, 578–597 (2015).
Fuchs Wightman, F., Giono, L. E., Fededa, J. P. & de la Mata, M. Target RNAs Strike Back on MicroRNAs. Front. Genet.9, 435 (2018).
Ash, P. E., Vanderweyde, T. E., Youmans, K. L., Apicco, D. J. & Wolozin, B. Pathological stress granules in Alzheimer’s disease. Brain Res.1584, 52–58 (2014).
Vanderweyde, T. et al. Contrasting pathology of the stress granule proteins TIA-1 and G3BP in tauopathies. J. Neurosci.32, 8270–8283 (2012).
Staffaroni, A. M. et al. Association of blood and cerebrospinal fluid tau level and other biomarkers with survival time in sporadic Creutzfeldt-Jakob disease. JAMA Neurol.76, 969–977 (2019).
Thompson, A. G. B. et al. Neurofilament light chain and tau concentrations are markedly increased in the serum of patients with sporadic Creutzfeldt-Jakob disease, and tau correlates with rate of disease progression. J. Neurol. Neurosurg. Psychiatry89, 955–961 (2018).
Blondal, T. et al. Assessing sample and miRNA profile quality in serum and plasma or other biofluids. Methods59, S1–S6 (2013).
Kirschner, M. B. et al. The impact of hemolysis on cell-free microRNA biomarkers. Front. Genet.4, 94 (2013).
Ludwig, N. et al. Machine learning to detect Alzheimer’s disease from circulating non-coding RNAs. Genomics Proteom. Bioinformatics17, 430–440 (2019).
Consortium, G. T. The Genotype-Tissue Expression (GTEx) project. Nat. Genet.45, 580–585 (2013).
Thompson, A. G. et al. The Medical Research Council prion disease rating scale: a new outcome measure for prion disease therapeutic trials developed and validated using systematic observational studies. Brain136, 1116–1127 (2013).
Dubois, B. et al. Advancing research diagnostic criteria for Alzheimer’s disease: the IWG-2 criteria. Lancet Neurol.13, 614–629 (2014).
Karagkouni, D. et al. DIANA-TarBase v8: a decade-long collection of experimentally supported miRNA-gene interactions. Nucleic Acids Res.46, D239–D245 (2018).
Chen, E. Y. et al. Enrichr: interactive and collaborative HTML5 gene list enrichment analysis tool. BMC Bioinformatics14, 128 (2013).
Kuleshov, M. V. et al. Enrichr: a comprehensive gene set enrichment analysis web server 2016 update. Nucleic Acids Res.44, W90–W97 (2016).
We are very grateful to patients and volunteers who have made this study possible by donating blood samples and their time to research; Holger Hummerich for helpful discussions; Tony Brooks, Paola Niola, and Mark Kristiansen from UCL Genomics for technical assistance with MiSeq; Tracy Campbell and Joanna Field for help with metadata acquisition; Richard Newton for help with preparation of figures. This study was funded by the UK Medical Research Council and the National Institute of Health Research (NIHR) Biomedical Research Centre at UCL Hospitals NHS Foundation Trust. S.M. and J.C. are NIHR Senior Investigators. J.M.S. is supported by the NIHR University College London Hospitals Biomedical Research Centre, Wolfson Foundation, Engineering and Physical Sciences Research Council, MRC Dementias Platform UK, Alzheimer’s Research UK (ARUK), Brain Research UK, Weston Brain Institute and European Union’s Horizon 2020 research and innovation programme. R.W.P. is funded by an NIHR clinical lectureship, A.G.B.T. was funded by clinical lectureships from NIHR and ARUK, L.C.D. was supported by a Leonard Wolfson Foundation PhD fellowship, A.N. is a MRC Clinical Research Training Fellow, F.G. is funded by a grant from the National Institute for Health Research, and T.H.M. is funded by a clinical research fellowship from the Alzheimer’s Society. The sponsor provided financial support for the research but was not involved in the design and conduct of the study; collection, management, analysis and interpretation of the data; preparation, review or approval of the manuscript; and decision to submit the manuscript for publication.
Prof. Collinge is a director and shareholder of D-Gen Limited (London), an academic spinout company working in the field of prion disease diagnosis, decontamination and therapeutics. Prof. Schott has received research funding and PET tracer from AVID Radiopharmaceuticals (a wholly owned subsidiary of Eli Lilly); has consulted for Roche, Eli Lilly, Biogen and Merck, GE; received royalties from Oxford University Press and Henry Stewart Talks; given education lectures sponsored by Eli Lilly, Biogen and GE; and serves on a Data Safety Monitoring Committee for Axon Neuroscience SE. All other authors declare no competing interests.
Peer review informationNature Communications thanks Karl Frontzek and other, anonymous, reviewers for their contributions to the peer review of this work. Peer review reports are available.
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Norsworthy, P.J., Thompson, A.G.B., Mok, T.H. et al. A blood miRNA signature associates with sporadic Creutzfeldt-Jakob disease diagnosis. Nat Commun 11, 3960 (2020). https://doi.org/10.1038/s41467-020-17655-x
Distribution of microRNA profiles in pre-clinical and clinical forms of murine and human prion disease
Communications Biology (2021)