Next Article in Journal
Polymorphic Characterization, Pharmacokinetics, and Anti-Inflammatory Activity of Ginsenoside Compound K Polymorphs
Next Article in Special Issue
Analytical Problems with Preparation of Paraspinal Tissues from Patients with Spinal Fusion for Analysis of Titanium
Previous Article in Journal
Structural Evidence for Pnictogen-Centered Lewis Acidity in Cationic Platinum-Stibine Complexes Featuring Pendent Amino or Ammonium Groups
 
 
Search for Articles:
Title / Keyword
Author / Affiliation / Email
Journal
Article Type
 
 
Advanced Search
 
Section
Special Issue
Volume
Issue
Number
Page
 
Journals
Molecules
Volume 26
Issue 7
10.3390/molecules26071989
molecules-logo
Submit to this Journal Review for this Journal Propose a Special Issue
► Article Menu

Article Menu

share Share announcement Help format_quote Cite question_answer Discuss in SciProfiles thumb_up
...
Endorse textsms
...
Comment
first_page
settings
Order Article Reprints
Font Type:
Arial Georgia Verdana
Font Size:
Aa Aa Aa
Line Spacing:
Column Width:
Background:
Article

Impact of Collection Volume and DNA Extraction Method on the Detection of Biomarkers and HPV DNA in First-Void Urine

by
Laura Téblick
1,*,
Severien Van Keer
1,
Annemie De Smet
1,
Pierre Van Damme
1,
Michelle Laeremans
2,
Alejandra Rios Cortes
2,
Koen Beyers
2,
Vanessa Vankerckhoven
1,2,
Veerle Matheeussen
3,4,5,
Renee Mandersloot
6,
Arno Floore
6,
Chris J. L. M. Meijer
6,7,
Renske D. M. Steenbergen
7 and
Alex Vorsters
1
1
Centre for the Evaluation of Vaccination (CEV), Vaccine & Infectious Disease Institute (VAXINFECTIO), Faculty of Medicine and Health Sciences, University of Antwerp, 2610 Wilrijk-Antwerp, Belgium
2
Novosanis nv, 2110 Wijnegem, Belgium
3
Department of Microbiology, Antwerp University Hospital (UZA), 2650 Edegem-Antwerp, Belgium
4
Department of Medical Microbiology (LMM), Vaccine & Infectious Disease Institute (VAXINFECTIO), Faculty of Medicine and Health Sciences, University of Antwerp, 2610 Wilrijk-Antwerp, Belgium
5
Department of Medical Biochemistry, Faculty of Pharmaceutical, Biomedical and Veterinary Sciences, University of Antwerp, 2610 Wilrijk-Antwerp, Belgium
6
Self-Screen B.V, 1098 RX Amsterdam, The Netherlands
7
Amsterdam UMC, Pathology, Cancer Center Amsterdam, Vrije Universiteit Amsterdam, 1081 HV Amsterdam, The Netherlands
*
Author to whom correspondence should be addressed.
Molecules 2021, 26(7), 1989; https://doi.org/10.3390/molecules26071989
Submission received: 16 February 2021 / Revised: 22 March 2021 / Accepted: 27 March 2021 / Published: 1 April 2021
(This article belongs to the Special Issue Sample Preparation for Bioanalysis)
Browse Figures
Versions Notes

Abstract

:
The potential of first-void (FV) urine as a non-invasive liquid biopsy for detection of human papillomavirus (HPV) DNA and other biomarkers has been increasingly recognized over the past decade. In this study, we investigated whether the volume of this initial urine stream has an impact on the analytical performance of biomarkers. In parallel, we evaluated different DNA extraction protocols and introduced an internal control in the urine preservative. Twenty-five women, diagnosed with high-risk HPV, provided three home-collected FV urine samples using three FV urine collection devices (Colli-Pee) with collector tubes that differ in volume (4, 10, 20 mL). Each collector tube was prefilled with Urine Conservation Medium spiked with phocine herpesvirus 1 (PhHV-1) DNA as internal control. Five different DNA extraction protocols were compared, followed by PCR for GAPDH and PhHV-1 (qPCR), HPV DNA, and HBB (HPV-Risk Assay), and ACTB (methylation-specific qPCR). Results showed limited effects of collection volume on human and HPV DNA endpoints. In contrast, significant variations in yield for human endpoints were observed for different DNA extraction methods (p < 0.05). Additionally, the potential of PhHV-1 as internal control to monitor FV urine collection, storage, and processing was demonstrated.

1. Introduction

The potential of first-void (FV) urine as a suitable, non-invasive liquid biopsy for detection of human papillomavirus (HPV) DNA and other biomarkers to detect high-grade cervical abnormality, has already been reported [1,2,3,4,5,6,7,8]. High correlates between urinary HPV DNA and cervical infections have been established and studies have confirmed the presence of HPV specific antibodies in FV urine [9,10,11,12,13,14,15,16]. Urine is considered the preferred choice of self-sampling compared to the currently available self-sampling methods used for screening; brush, lavage, spatula, swab and tampon [17,18,19,20,21,22,23,24]. Especially during the current COVID-19 (Coronavirus Disease 2019) pandemic, at-home self-sampling will provide a more accessible means for screening or follow-up than attending health care facilities. However, to use FV urine as custom liquid biopsy for cervical cancer screening, potential optimization of the sample collection and DNA extraction workflow should be considered.
The rationale behind the use of FV urine is based on the fact that the initial stream of urine – first-void– washes away secretions that accumulate between the small labia and around the urethra opening, including mucus and debris from exfoliated cells from the vagina, cervix, and uterus [25]. This explains why the first fraction of a urine void contains significantly more HPV DNA than the subsequent part [12]. However, the optimal volume of the initial urine stream to provide the highest concentration of biomarkers of interest has not been established yet. The currently used FV urine collection device (Colli-Pee®, Novosanis, Wijnegem, Belgium), prefilled with Urine Conservation Medium (UCM), collects the first fraction of urine in a total volume of 20 mL (one part UCM and two parts FV urine). The UCM buffer has already shown to positively influence detectable HPV DNA by avoiding degradation of cell-free DNA by nucleases [1]. The ideal FV urine volume would provide optimal concentration of HPV and human DNA for accurate detection of clinically relevant high risk (HR)-HPV infections. In addition, use of customized tubes, like the routinely used 10 mL tubes, could allow fully automated high-throughput testing.
An internal process control is another important factor to validate a sample for analysis. This internal control needs to be able to monitor the presence of sufficient preservative, demonstrate that the extraction was well performed, and show that no degradation of DNA/biomarker of interest took place. Earlier research in our lab showed that human DNA is not entirely sufficient as an internal process control since inappropriately stored samples still had detectable human DNA, while the HPV DNA test became false negative [1]. In addition, the amount of human DNA is very variable between samples/individuals. As detection of cell-free viral DNA is also essential, the most suitable internal control would be DNA from a whole virus preparation.
To date, there are numerous adequate DNA extraction methods on the market, each having its own advantages and limitations [2]. However, it has not yet been investigated whether the extraction method used in combination with different FV urine volumes influences the yield of recovered human DNA, HPV DNA, and other biomarkers of interest. The evaluation of the distinct DNA extraction methods and FV urine collection volumes in combination with the introduction of an internal process control offers additional opportunities for the use of FV urine as a suitable sample for the detection of HPV.
In many European Union (EU) countries, cervical cancer screening is based on cytology. This requires a physician-taken cervical scrape and is challenged by low sensitivity (30% false-negatives) and high non-attendance (63% EU coverage) [26]. The combination of a FV urine collector and an integrated diagnostic approach for both HPV detection and triage after an HPV positive result to identify women with cervical cancer or precursor lesions could maximize screening participation.
In this study, we investigated whether the FV urine collection volume affects the detection of human and viral endpoints (i.e., glyceraldehyde 3-phosphate dehydrogenase (GAPDH), β-actin (ACTB), β-globin (HBB), HPV) by comparing three different FV urine collection volumes (4, 10, and 20 mL). In addition, we evaluated different DNA extraction protocols and introduced a universal non-human control (i.e., DNA from phocine herpesvirus 1 (PhHV-1) [27,28]) in the urine preservative to monitor sample collection, transport, storage, and DNA extraction.

2. Results

2.1. Sample Collection

Three samples, all different volumes at random order, were received from 25 women aged between 19 and 62 years old (overview in Figure 1). The median age in the cohort was 31 (interquartile range (IQR): 27–35). Median (IQR) estimated collection volumes were 4.1 (3.8–4.4) mL, 9.8 (9.4–10.3) mL, and 20.3 (19.8–20.8) mL with collector tubes estimated to collect 4 mL, 10 mL, and 20 mL, respectively. The three samples were collected within a median (IQR) time interval of 3h 2min (2:30–4:26). Two women collected one sample on another day than the other two samples. Data for GAPDH, PhHV-1, ACTB, HBB, and HPV DNA was generated from 3 × 25 FV urine samples.

2.2. Evaluation of PhHV-1 as Internal Process Control

Internal control quantification cycle (Cq) value results of the 25 women included in the study were generated by qPCR (Figure 2). Since spiked PhHV-1 concentrations in the different FV urine collection volumes were identical and no significant differences in Cq values were observed between the different collection volumes when using the same extraction method (p ≥ 0.36), cut-offs were calculated for each DNA extraction method separately, but on all volumes combined (cut-offs; AM_EM: 36.26, EM: 35.83, CF800_EM: 36.40, CF800_QIA: 40.00, CF3000_EM: 35.81). Comparing three different collection volumes using EM and four extraction methods on 20 mL, three IDs (1, 8, and 19) exceeded the calculated cut-offs. Comparing two collection volumes using CF800_EM and three extraction methods on 10 mL, also three samples (8, 15, and 19) exceeded the calculated cut-offs. Since the sample size is too low to validate the exploratory defined cut-off, all samples were included in further analyses. The distribution of Cq values varied between different extraction methods. A linear model was used to investigate the effect of time (days) between sample collection and freezing of aliquoted samples on the DNA yield of PhHV-1, GAPDH, HBB, and ACTB using extraction method EM (Figure A1). For none of the human endpoints, a significant effect was found (all p ≥ 0.05). However, there was a significant effect of time between collection and freezing on the PhHV-1 Cq values (p = 0.017). For each extra day between FV urine collection and storage at −80 °C for samples extracted with EM, the median Cq value increased by 0.19 (Figure A2).

2.3. Comparison of DNA and Biomarker Yields between FV Urine Collection Volumes

2.3.1. Human Endpoints

PCR Cq value results, inversely proportional to concentrations, for GAPDH, HBB, and ACTB were generated for all three FV urine collection volumes using extraction method EM and on 10 mL, and 20 mL samples using CF800_EM. Results are presented as boxplots (Figure 3). Using EM, we observed no significant differences between the three FV urine collection volumes for all human endpoints (GAPDH: p ≥ 0.07, ACTB: p ≥ 0.40, HBB: p ≥ 0.28) (Figure 3). In addition, similar and all highly significant (p ≤ 3.9 × 10−4) Pearson correlations were found between all three housekeeping genes; GAPDH, HBB, and ACTB, for all collection volumes (Figure A3). The timing of the three FV urine collections did also not have a significant effect on the DNA Cq value for all three human endpoints (data not shown). For CF800_EM, there was no significant Cq difference for HBB (p = 0.85) and ACTB (p = 0.083) between 10 and 20 mL collections. We did observe significant differences in Cq for GAPDH (p = 0.033). Here median Cq value for 20 mL (28.3) was higher than for 10 mL (27.6). However, the same Pearson correlation trend between all housekeeping genes was seen for CF800_EM (p ≤ 1.36 × 10−12) compared to EM (Figure A4).

2.3.2. Viral Endpoints

HPV DNA results for different volumes were compared using the DNA extraction method EM (Table 1). Samples were classified as HR-HPV positive when HR-HPV DNA was present. Here, no samples showed presence of HPV-16 or -18 DNA. However, in total 37% (28/75) of the DNA samples extracted with EM and 44% (23/50) with CF800_EM contained HPV DNA of an HR-HPV type included in the HPV-Risk assay. Using EM, FV urine samples collected with the 4 mL device showed 32% (8/25) HR-HPV positivity, the 10 mL device 44% (11/25), and the 20 mL 36% (9/25). No significant differences were found (p ≥ 0.14). Concordance of the HR-HPV positivity results over the different FV urine collection volumes are K4/10 = 0.58 and K4/20 = 0.91, K10/20 = 0.67. For CF800_EM, FV urine samples collected with the 10 mL device showed 52% (13/25) HR-HPV positivity and the 20 mL 40% (10/25). Here, Cohen’s Kappa value is 0.60. While not all volumes gave HR-HPV positive results, the Cq values were high (34.71; 28.89–38.78) in the sample where HR-HPV DNA was detected.

2.4. Comparison of DNA and Biomarker Yields between DNA Extraction Methods

2.4.1. Human Endpoints

DNA yield results for GAPDH, HBB, and ACTB on the different DNA extraction methods were generated and presented as boxplots (Figure 4). Comparing four DNA extraction methods (AM_EM, EM, CF800_EM, and CF800_QIA) used on 20 mL FV urine samples, GAPDH Cq values were significantly higher for EM in comparison to all other methods (p ≤ 0.12 × 10−3). In addition, AM_EM had a lower Cq value for GAPDH than CF800_EM (p = 0.04). The HBB Cq values for EM were significantly higher than for AM_EM (p = 0.21 × 10−2), CF800_EM (p = 0.26 × 10−3), and CF800_QIA (p = 0.79 × 10−2)). The quantitative Methylation-Specific PCR (qMSP) results for ACTB showed significantly lower yield for EM (p = 0.16 × 10−3) and CF800_QIA (p = 0.52 × 10−2) compared to results for AM_EM. Moreover, CF800_EM had significantly lower Cq-values than EM (p = 7.40 × 10−5) and CF800_QIA (p = 0.01), but no significant difference was observed between CF800_EM and AM_EM (p = 1.00). There was a significant Pearson correlation between all human endpoint combinations (p ≤ 1.80 × 10−10) for all extraction methods (Figure A5). Since extraction method CF800_EM showed promising results and a smaller collection volume has transport and storage advantages, the remaining volume of the 10 mL FV urine sample was used to compare two centrifugation speeds (CF800_EM and CF3000_EM). In total, three different DNA extraction methods (EM, CF800_EM, and CF3000_EM) were compared using 10 mL FV urine samples. Here, GAPDH Cq values were significantly lower, using CF800_EM or CF3000_EM compared to EM (p ≤ 0.35 × 10−2). The HBB Cq values showed no significant differences for all methods (p ≤ 0.08). Results for ACTB showed significantly higher yield for EM compared to CF3000_EM (p = 0.016). Other observed variations were not significant (Figure 4). For all three extraction methods, there was a significant Pearson correlation between all human endpoint combinations (p ≤ 3.91 × 10−4) (Figure A6). For the 4 mL FV urine samples, only extraction method EM was used since there was not enough volume left to perform additional extractions.

2.4.2. Viral Endpoints

Results for different extraction methods were evaluated on 20 mL and 10 mL samples (Table 1). No samples showed the presence of HPV16 or -18 DNA. HR-HPV infections were found in 39% (39/100) of the 20 mL FV urine DNA extracts. DNA extracted with AM_EM showed 44% (11/25) HR-HPV positivity, with EM 36% (9/25), with CF800_EM 40% (10/25), and with CF800_QIA 36% (9/25). No significant differences were found (p ≥ 0.09). Here, the Fleiss Kappa value is 0.87. In total 48% (36/75) of the 10 mL FV urine DNA extracts contained HPV DNA of an HR-HPV type included in the HPV-Risk assay. DNA extracted with EM showed 44% (11/25) HR-HPV positivity, CF800_EM 52% (13/25), and CF3000_EM 48% (12/25). Concordance of the HR-HPV positivity results over the different DNA extraction methods on 10 mL samples was 0.78. Whenever not all methods gave HR-HPV positive results, the Cq values were high (36.39; 30.83–39.24) in the extracts where HR-HPV DNA was detected.

3. Discussion

The use of FV urine as a self-sample for HPV DNA testing has already proven promising and high correlates between urinary HPV DNA and cervical infections have been established [3]. Combining this non-invasive and user-friendly sample with a tailored molecular assay for the detection of pre-cancer biomarkers in urine [8,29,30,31] could provide an alternative for the current non-attendees of screening programs and ultimately the entire screening population. We studied several sample collection and extraction workflows (i.e., internal control, collection volume, DNA extraction method) to investigate if we could improve the performance of FV urine as a liquid biopsy.

3.1. Internal Process Control

As part of the optimization process, we introduced phocine herpesvirus type 1 (PhHV-1) as internal process control in the UCM and observed degradation in PhHV-1 DNA when samples were stored for 12 days at ambient temperature (Figure A1) whereas this was not seen for GAPDH when samples were stored with UCM. This difference can be due to the fact that GAPDH concentrations are subsidiary to interpersonal variation and PhHV-1 DNA is spiked in a constant concentration. PhHV-1 Cq values furthermore linearly increased with an average of 0.19 Cq per additional day passed between sample collection and storage at −80 °C in this specific sample set of 75 FV urine extracts (extraction method EM on all three collection volumes), confirming its potential as an internal control for sample storage. The selection of a cell-free internal control is based upon previous studies where it was shown that non-cell associated DNA in FV urine samples is most vulnerable to degradation [1,2]. Since the buffer is spiked with PhHV-1, not detecting this control will indicate inappropriate sample collection. Due to PhHV-1 DNA being cell-free, and thus not able to pellet, it is impossible to combine this control with an extraction method that only uses the pellet for qPCR (CF800_QIA). Small fluctuations between PhHV-1 Cq values within the same DNA extraction method can be due to different sample composition and storage conditions [2,32]. The internal control cut-off calculated in this pilot sample set will be evaluated in a larger external validation set (CASUS, clinicaltrials.gov: NCT04530201). Combining the UCM [1] with an internal process control will allow laboratories to set up a strict sample control quality system, confirming the presence of the preservative and absence of substantial nucleic acid degradation.

3.2. FV Urine Collection Volume

The most widely used method for urine collection to screen for infectious agents or other biomarkers is the use of a urine collection cup. However, these cups are not designed to collect the first urine fraction, making it more difficult to confidently collect the initial urine stream with high concentrations of certain biomarkers [12,32]. Colli-Pee® is a commercially available device that collects a standardized, pre-defined volume of FV urine without the need to interrupt the urine current. With a view toward volume optimization, different FV urine collection devices collecting a fixed volume of the initial urine stream were evaluated. Results of the experimental arms compared in this study show limited differences between the FV urine collection volumes for all human endpoints using EM. The human endpoints evaluated within this study represent the sample quality for both HPV DNA testing and biomarker testing and are therefore important factors to evaluate. Since HPV DNA detection using the 20 mL collection device already provided promising analytical and clinical accuracy results [1,17,32,33,34]. These additional results also support the potential of the 4- and 10- mL collection volume. For CF800_EM, there was a significant difference between 10- and 20-mL samples for GAPDH. When comparing HPV DNA Cq values, more HR-HPV infections were detected using Colli-Pee® for the collection of 10 mL compared to 4- and 20-mL. Based on these results, we can conclude that collecting only 10 ml could provide an increased sample quality for the detection of HPV DNA. In addition, we hypothesize that 4 mL of FV urine (approximately 2.33 mL when taking the buffer into account), is not sufficient to wash away all secretions that have accumulated between the urethra and small labia. Since there is a clear biological link between HPV infection and cervical pre-cancer and cancer, the highest HPV DNA concentration will also be a good representation for the highest amount of biomarkers, including methylation markers [35,36,37,38]. Besides, the smaller collector tube of the 10 ml in contrast to the 20 mL device has advantages in transport (by, e.g., postal mail), storage, and high-throughput testing if a fully integrated nucleic acid extraction and testing platform is used.

3.3. DNA Extraction Method

To date, there has not been a comparison between DNA extraction methods in combination with different FV urine collection volumes. Since the DNA extraction can most likely influence the concentration of a certain biomarker, we compared five different extraction methods overall, including a direct comparison of four methods on 20 mL FV urine samples. Almost all differences in Cq value can directly be linked to the difference in implemented volumes. Variation in centrifugal forces did not cause different DNA yields (CF800_EM vs. CF3000_EM). For both human and viral endpoints using only the pellet for extraction (CF800_QIA) gave similar DNA yields in comparison to other methods. However, this extraction method is not compatible with the selected internal control given that cell-free viral DNA is not concentrated by the pellet. Considering all factors, including costs and amount of laboratory work, which are higher for AM_EM and CF800_QIA and lower yields of human and viral endpoints for EM; preference is given to CF800_EM.

3.4. Limitations of the Study

A number of limitations regarding this study need to be acknowledged. First, the relatively small sample size making it necessary to be cautious while interpreting the results. Second, samples exceeding the internal control cut-offs were not excluded from the data since calculations were only performed on this training set and need further evaluation in an independent validation set. Third, since all women self-reported to have an HR-HPV infection in the previous six months, no documentation concerning their infection was provided to the study team and could therefore not be verified. We also did not receive information on whether the HPV infection was associated with a cervical intraepithelial lesion (CIN). Only 13 out of 25 women still had a detectable HR-HPV infection in at least one of the three collected samples. However, the objective of this study was not to compare urinary and cervical HR-HPV infections but to develop a reproducible optimal urine sampling and DNA extraction protocol. As this study is the first study to optimize the combination of FV urine collection volume, DNA extraction methods, and introduction of an internal control we are confident that these limitations will not have a major effect on the study outcomes.

4. Materials and Methods

4.1. Identification of the Internal Control Spiking Concentration

To investigate the accuracy of PhHV-1 DNA as internal control, four FV urine samples were used. All four healthy female volunteers collected ±25 mL of urine using a standard urine collection vial. These samples were divided into two falcon tubes; one tube containing 10 mL urine without UCM preservative, another one containing a total volume of 10 mL urine, and UCM in a ratio of 2:1 urine/UCM. DNA from PhHV-1 was extracted from 200 µL MEM culture medium of a PhHV-1 infected Crandell Rees Feline kidney cell line using the NucliSENS® EasyMag® (bioMérieux, off-board lysis protocol) and eluted in 100 µl. All eight samples were spiked with 25 µL of a 1:1000 dilution of this DNA eluate (stored at 4 °C). To investigate the quantity and stability of PhHV-1 DNA in the samples, 5 mL of each sample was used for DNA extractions (Figure A1). The remaining 5 mL of each sample was stored 7 days at 4 °C and an additional 5 days at room temperature after which DNA extractions using NucliSENS EasyMag on both FV urine concentrate after Amicon filtration of 4 mL (AM_EM) and 1 ml of neat FV urine (EM) were repeated for these samples. All samples were analyzed using semi-quantitative PCR (qPCR) for human DNA (GAPDH) and internal control DNA (PhHV-1) (see Section 4.5). Using this spiking volume, the initial Cq value for each UCM/FV urine combination would be 30–33, dependent on the DNA extraction method.

4.2. Study Population

In total, 25 women, age 19–62 years, were included between August and November 2019 (clinicaltrials.gov ID: NCT04480866) (Figure 1). Each woman self-reported to have an HR-HPV infection, which was identified during a gynecological visit in the previous six months. Informed consent was obtained from all women before sample collection.

4.3. Sample Collection and Storage

Women were notified about the study by email (University of Antwerp employees) or via social media. Women interested to participate in the trial first subscribed online via the Centre for the Evaluation of Vaccination (CEV) web page. Next, the study team contacted eligible women by phone and sent an additional e-mail to complete their registration if all inclusion criteria were met. Subsequently, a package with the information brochure, informed consent form, and collection devices with instructions for use was sent to the participants by postal mail. Each participant collected three consecutive samples at home, using prototype FV urine devices (Colli-Pee®, Novosanis) with collector tubes that differ in size, prefilled with 1/3 UCM (Novosanis) spiked with 25 µL of a 1:1000 dilution of PhHV-1 DNA extract as an internal control. This allowed us to collect an average of approximately 2.67, 6.67, and 13.33 mL urine in total volumes of 4, 10, and 20 mL respectively. Women were requested not to wash their genitals before collection, collect all samples on the same day, and not to urinate at least 2 h (h) before each collection. All samples were collected in random order, alternating the collection volumes to eliminate potential bias associated with sampling order. Earlier research already confirmed that morning FV urine does not contain higher (HPV) DNA concentrations than FV urine collected later during the day, eliminating this potential bias [32,39]. The same day of collection (or at the latest, one day after collection), the urine samples were sent back to the University of Antwerp via postal mail where they were aliquoted and stored at −80 °C (Biobank Antwerpen, Antwerp, Belgium; ID: BE 71030031000) prior to further analysis [40].

4.4. DNA Extraction from FV Urine Samples

Before every extraction, buffered aliquots of urine samples were thawed (after storage for 1–2 months). For this study, five different DNA extraction methods were used (overview in Figure 1). For four out of five methods (AM_EM, EM, CF800_EM, and CF3000_EM), the NucliSENS® EasyMag® (bioMérieux, off-board lysis generic protocol) was used and DNA was eluted in 65 µL for further analysis. The first DNA extraction method (AM_EM) used an in-house protocol [1]. Briefly, 4 mL of the FV urine aliquot was centrifuged at 3820 g for 20 min at 20 °C in an Amicon Ultra-4 50 K filter device (Merck Millipore, Belgium). Next, 2 mL NucliSENS Lysis Buffer (bioMérieux Benelux, Schaarbeek, Belgium) was added to the concentrate retained on the filter. After incubation of at least 10 min at room temperature, all material was transferred to the NucliSENS Lysis buffer vial and DNA extraction was performed on the buffered concentrate. For the second method (EM), direct DNA extraction was performed on 1 mL of the FV urine sample in 2 mL lysis buffer. The third extraction method (CF800_EM) started with centrifuging 4 mL of the FV urine sample at 800 g for 10 min at room temperature. The pellet and 1 mL of supernatant were suspended in 2 mL lysis buffer and used for DNA extraction. The fourth extraction method (CF3000_EM) used almost the same protocol as CF800_EM, the only difference was centrifugation at 3000 g instead of 800 g. For the last extraction method (CF800_QIA), 4 mL of the FV urine sample was centrifugated at 800 g for 10 min at room temperature. The pellet was resuspended in 200 µL of supernatant. DNA was extracted using the QIAamp DNA Blood Mini kit, according to the manufacturer’s protocol (Qiagen GmbH, Germany) and eluted in 65 µL H2O [1]. Different DNA extraction methods were compared for collection volumes; for 4 mL samples, extraction method EM was used; for 10 mL samples, extraction methods EM, CF800_EM, and CF3000_EM were used; for 20 mL samples, extraction methods AM_EM, EM, CF800_EM, and CF800_QIA were used (Figure 1).

4.5. Semi-Quantitative PCR for GAPDH and PhHV-1

All DNA extracts obtained from FV urine samples were analyzed using semi-quantitative PCR (qPCR) for human DNA (GAPDH) and internal control DNA (PhHV-1). This qPCR technique is based on TaqMan technology and performed with the LightCycler480 Real-Time PCR instrument (Roche Diagnostics, Machelen, Belgium) as described by Vorsters et al. (2014) [1]. Briefly, a 20-µL portion of the GAPDH PCR mixture containing 1× LightCycler® 480 Probes Master (Roche Diagnostics, Machelen, Belgium), 0.5 μM concentrations of each primer, 0.1 μM concentrations of probe, and 5 μL of DNA solution was loaded into the LightCycler. Primers and probes for GAPDH are defined by Payan et al. (2007) [41]. For PhHV-1 qPCR was performed on 20 µL of the following mixture; 1 × LightCycler® 480 Probes Master (Roche Applied Science, Belgium), 0.05 µM forward primer, 0.2 µM reverse primer, 0.1 μM probe, and 5 μL of DNA solution. PhHV-1 primers and probes are described by Van Doornum et al. (2002) [27]. The thermal cycles were as follows: an initial 10 min at 95 °C for FastStart Taq DNA Polymerase activation, followed by 45 cycles of 10 s of denaturing at 95 °C, 15 s of annealing at 60 °C. Both positive and negative controls were used on each run to confirm reproducibility.

4.6. HPV-Risk Assay

High-risk HPV testing was done using the HPV-Risk assay (Self-screen B.V., Amsterdam), which is a multiplex, real-time PCR assay targeting the E7 region of 15 (probably) HR-HPV types (HPV16, -18, -31, -33, -35, -39, -45, -51, -52, -56, -58, -59, -66, -67, and -68), and providing additional genotype information for HPV16 and HPV18 [42]. The assay includes amplification of the reference gene HBB to assess DNA quality and quantity. The assay was performed using 5 µL of the DNA extract according to the manufacturer’s instructions, on a Rotor-Gene Q MDx 5plex HRM instrument (Qiagen GMBH, Hilden, Germany). The Cq value cut-offs of the assay for calling a sample HPV-positive were not used. Samples were scored HPV positive when there was a Cq value for any of the HPV targets.

4.7. Semi-Quantitative PCR on Bisulfite Converted DNA

For testing the suitability of the DNA for quantitative Methylation-Specific PCR (qMSP), DNA extracted from FV urine was treated with bisulfite and amplified using primers and probes in the ACTB gene area containing at least three cytidines, as described previously [43,44,45,46]. Bisulfite-conversion was performed with the EZ DNA Methylation kit (Zymo Research, Orange, CA, USA) according to the manufacturer’s specifications. Standard DNA input for bisulfite-conversion was 250 ng. Elution was done with 12.5 µL M-elution buffer yielding 20 ng/µL bisulfite-converted DNA. For samples with insufficient DNA yield to accomplish an input of 250 ng (around 50% of the samples), a standard amount of 45 µL was used.

4.8. Statistical Analysis

For the statistical analysis, we used R statistical software version 3.6.0. The data were first checked for their normality using Shapiro–Wilk test. If the data were normally distributed, significant differences between different collection volumes and DNA extraction methods were examined using paired t-test, otherwise non-parametric Wilcoxon signed-rank testing was used. Statistical significance was defined as p-adjusted < 0.05 (using Holm–Bonferroni method for p-value adjustment). To analyze possible correlations between housekeeping genes (GAPDH, ACTB, HBB), Pearson correlation coefficients were calculated. To investigate HPV positivity agreement between different FV urine collection volumes and DNA extraction methods, Cohen’s Kappa (K) when maximum three conditions were compared and Fleiss Kappa values when more than three conditions were compared, were calculated. For the calculation of cut-off within the internal control data, the mean Cq plus two standard deviations were used [27]. To check whether there was an effect of time between collection and freezing on DNA yield for all endpoints, including internal control, we used a linear regression model on all EM data.

5. Conclusions

In conclusion, we have evaluated a potential internal control of which the exact cut-off concentrations for sample validity will need to be determined in a validation study (NCT04530201). Good agreement between the three different FV urine collection volumes was found for all human endpoints. Because of the advantages of a lower collection volume in high-throughput testing and the highest percentage of HPV DNA-positive DNA extracts, the 10 mL collection volume is preferred. Overall, the preferred collection and processing combination within this study would be a 10 mL collection device, prefilled with UCM containing PhHV-1 as internal control, together with DNA extraction using 4 mL of the collected FV urine for centrifugation at 800 g whereof the pellet and 1 mL of supernatant will be used for NucliSENS EasyMag extraction (CF800_EM).

Author Contributions

Conceptualization, S.V.K., A.V., V.V., C.J.L.M.M. and R.D.M.S.; methodology, L.T., S.V.K., M.L., A.R.C., A.F. and R.M.; formal analysis, L.T.; resources, K.B., V.V., C.J.L.M.M., R.D.M.S. and V.M.; data curation, L.T., A.D.S. and A.F.; writing—original draft preparation, L.T.; writing—review and editing, L.T., S.V.K., A.D.S., P.V.D., M.L., V.M., A.F., C.J.L.M.M., R.D.M.S., V.V. and A.V.; visualization, L.T.; supervision, A.V. and R.D.M.S.; project administration, S.V.K., A.V., V.V., C.J.L.M.M. and R.D.M.S.; funding acquisition, S.V.K., A.V., V.V., C.J.L.M.M. and R.D.M.S. All authors have read and agreed to the published version of the manuscript.

Funding

This research was funded by H2020 Eurostars, grant number 12396. The funder did not play a role in this research. S. Van Keer is supported by a postdoctoral fellowship of the Research Foundation-Flanders (1240220N).

Institutional Review Board Statement

The study was conducted according to the guidelines of the Declaration of Helsinki, and approved by the Institutional Review Board (or Ethics Committee) of UZA/ University of Antwerp (B300201525585, 15 April 2019).

Informed Consent Statement

Informed consent was obtained from all subjects involved in the study.

Data Availability Statement

The data presented in this study are available from the corresponding author, L.T., upon reasonable request.

Acknowledgments

We would like to express our gratitude to all women who volunteered to participate in this study.

Conflicts of Interest

Novosanis, which produces and provided the Colli-Pee® device, was founded as a spin-off company of the University of Antwerp, Belgium and is now a subsidiary of OraSure Technologies Inc., US. A.V., V.V., and P.V.D. were co-founders of Novosanis. C.J.L.M.M. is minority shareholder and part-time CEO of Self-screen B.V., a spin-off company of VU University Medical Center Am, which develops, manufactures, and licenses the high-risk HPV assay and methylation marker assays for cervical cancer screening and holds patents on these tests. C.J.L.M.M. has a very small number of shares of QIAGEN and MDXHealth, has received speakers’ fees from GSK, QIAGEN, and SPMSD/Merck, and served occasionally on the scientific advisory boards (expert meeting) of these companies. R.D.M.S. has a minority stake in Self-screen B.V. (The Netherlands), a spin-off company of VU University Medical Center Amsterdam, which owns patents related to this work. A.F. and R.M. are employed by Self-screen B.V. Other authors declare that they have no conflict of interest.

Sample Availability

Not available.

Appendix A

Molecules 26 01989 g0a1 550
Figure A1. Results for GAPDH (upper figures) and PhHV-1 (lower figures) on 4 FV urine samples. Each ID has a unique color mating its Cq values. Samples were processed directly (Direct) and after 12 days of storage at room temperature. Presence of UCM in the samples is referred to as either “With_UCM” or “Without_UCM”. The use DNA Extraction method is referred to as well; AM_EM or EM. No PhHV-1 result was obtained for ID3 at time point 0 for category With_UCM_AM_EM due to pipetting error. UCM; Urine Conservation Medium, EM; EasyMag, AM; Amicon filtration.
Figure A1. Results for GAPDH (upper figures) and PhHV-1 (lower figures) on 4 FV urine samples. Each ID has a unique color mating its Cq values. Samples were processed directly (Direct) and after 12 days of storage at room temperature. Presence of UCM in the samples is referred to as either “With_UCM” or “Without_UCM”. The use DNA Extraction method is referred to as well; AM_EM or EM. No PhHV-1 result was obtained for ID3 at time point 0 for category With_UCM_AM_EM due to pipetting error. UCM; Urine Conservation Medium, EM; EasyMag, AM; Amicon filtration.
Molecules 26 01989 g0a1
Molecules 26 01989 g0a2 550
Figure A2. Spreading and correlation curve of PhHV-1 Cq values of DNA extracted with EM over timespan between collection of the urine sample and storage at −80 °C. A linear model was used to evaluate this effect. For each extra day between FV urine collection and storage at −80 °C, the Cq value increased with 0.19. This effect was significant. No such significant effect was seen for all other human endpoints.
Figure A2. Spreading and correlation curve of PhHV-1 Cq values of DNA extracted with EM over timespan between collection of the urine sample and storage at −80 °C. A linear model was used to evaluate this effect. For each extra day between FV urine collection and storage at −80 °C, the Cq value increased with 0.19. This effect was significant. No such significant effect was seen for all other human endpoints.
Molecules 26 01989 g0a2
Molecules 26 01989 g0a3 550
Figure A3. Correlation curves for all human endpoint combinations on DNA extracted using EM for 4, 10, and 20 mL FV urine collection volumes. High risk (HR)-HPV positive samples are marked grey. All correlations are highly significant. R² values are highest for 20 mL and lowest for 10 mL samples.
Figure A3. Correlation curves for all human endpoint combinations on DNA extracted using EM for 4, 10, and 20 mL FV urine collection volumes. High risk (HR)-HPV positive samples are marked grey. All correlations are highly significant. R² values are highest for 20 mL and lowest for 10 mL samples.
Molecules 26 01989 g0a3
Molecules 26 01989 g0a4 550
Figure A4. Correlation curves for all human endpoint combinations on DNA extracted using CF800_EM for 10 and 20 mL FV urine collection volumes. HR-HPV positive samples are marked grey. All correlations are highly significant, and R² values are similar for both volumes.
Figure A4. Correlation curves for all human endpoint combinations on DNA extracted using CF800_EM for 10 and 20 mL FV urine collection volumes. HR-HPV positive samples are marked grey. All correlations are highly significant, and R² values are similar for both volumes.
Molecules 26 01989 g0a4
Molecules 26 01989 g0a5 550
Figure A5. Correlation curves for all human endpoint combinations on 20 mL FV urine samples extracted with AM_EM, EM, CF800_EM, and CF800_QIA. HR-HPV positive samples are marked grey. All correlations are highly significant.
Figure A5. Correlation curves for all human endpoint combinations on 20 mL FV urine samples extracted with AM_EM, EM, CF800_EM, and CF800_QIA. HR-HPV positive samples are marked grey. All correlations are highly significant.
Molecules 26 01989 g0a5
Molecules 26 01989 g0a6 550
Figure A6. Correlation curves for all human endpoint combination on 10 mL FV urine samples extracted with EM, CF800_EM, and CF3000_EM. HR-HPV positive samples are marked grey. All correlations are highly significant. Using the method EM, R² values are lower than CF800_EM, and CF3000_EM.
Figure A6. Correlation curves for all human endpoint combination on 10 mL FV urine samples extracted with EM, CF800_EM, and CF3000_EM. HR-HPV positive samples are marked grey. All correlations are highly significant. Using the method EM, R² values are lower than CF800_EM, and CF3000_EM.
Molecules 26 01989 g0a6

References

  1. Vorsters, A.; Van den Bergh, J.; Micalessi, I.; Biesmans, S.; Bogers, J.; Hens, A.; De Coster, I.; Ieven, M.; Van Damme, P. Optimization of HPV DNA detection in urine by improving collection, storage, and extraction. Eur. J. Clin. Microbiol. Infect. Dis. 2014, 33, 2005–2014. [Google Scholar] [CrossRef]
  2. Vorsters, A.; Micalessi, I.; Bilcke, J.; Ieven, M.; Bogers, J.; Van Damme, P. Detection of human papillomavirus DNA in urine. A review of the literature. Eur. J. Clin. Microbiol. Infect. Dis. 2012, 31, 627–640. [Google Scholar] [CrossRef] [PubMed]
  3. Snoek, B.C.; Splunter, A.P.; Bleeker, M.C.G.; Ruiten, M.C.; Heideman, D.A.M.; Rurup, W.F.; Verlaat, W.; Schotman, H.; van Gent, M.; Trommel, N.E.; et al. Cervical cancer detection by DNA methylation analysis in urine. Sci. Rep. 2019, 9. [Google Scholar] [CrossRef] [PubMed]
  4. Pattyn, J.; Van Keer, S.; Téblick, L.; Van Damme, P.; Vorsters, A. HPV DNA detection in urine samples of women: ‘An efficacious and accurate alternative to cervical samples?’. Expert Rev. Anti. Infect. Ther. 2019, 17, 755–757. [Google Scholar] [CrossRef] [PubMed]
  5. Van Keer, S.; Pattyn, J.; Tjalma, W.A.A.; Van Ostade, X.; Ieven, M.; Van Damme, P.; Vorsters, A. First-void urine: A potential biomarker source for triage of high-risk human papillomavirus infected women. Eur. J. Obstet. Gynecol. Reprod. Biol. 2017, 216, 1–11. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  6. Luttmer, R.; De Strooper, L.M.A.; Steenbergen, R.D.M.; Berkhof, J.; Snijders, P.J.F.; Heideman, D.A.M.; Meijer, C.J.L.M. Management of high-risk HPV-positive women for detection of cervical (pre)cancer. Expert Rev. Mol. Diagn. 2016, 16, 961–974. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  7. Ebisch, R.M.F.; Siebers, A.G.; Bosgraaf, R.P.; Massuger, L.F.A.G.; Bekkers, R.L.M.; Melchers, W.J.G. Triage of high-risk HPV positive women in cervical cancer screening. Expert Rev. Anticancer Ther. 2016, 16, 1073–1085. [Google Scholar] [CrossRef] [PubMed]
  8. Cho, H.W.; Ouh, Y.T.; Hong, J.H.; Min, K.J.; So, K.A.; Kim, T.J.; Paik, E.S.; Lee, J.W.; Moon, J.H.; Lee, J.K. Comparison of urine, self-collected vaginal swab, and cervical swab samples for detecting human papillomavirus (HPV) with Roche Cobas HPV, Anyplex II HPV, and RealTime HR-S HPV assay. J. Virol. Methods 2019, 269, 77–82. [Google Scholar] [CrossRef] [PubMed]
  9. Burroni, E.; Bonanni, P.; Sani, C.; Lastrucci, V.; Carozzi, F. Human papillomavirus prevalence in paired urine and cervical samples in women invited for cervical cancer screening. J. Med. Virol. 2015, 87, 508–515. [Google Scholar] [CrossRef] [PubMed]
  10. Cómbita, A.L.; Gheit, T.; González, P.; Puerto, D.; Murillo, R.H.; Montoya, L.; Vorsters, A.; Van Keer, S.; Van Damme, P.; Tommasino, M.; et al. Comparison between Urine and Cervical Samples for HPV DNA Detection and Typing in Young Women in Colombia. Cancer Prev. Res. (Phila.) 2016, 9, 766–771. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  11. Ducancelle, A.; Legrand, M.C.; Pivert, A.; Veillon, P.; Le Guillou-Guillemette, H.; De Brux, M.A.; Beby-Defaux, A.; Agius, G.; Hantz, S.; Alain, S.; et al. Interest of human papillomavirus DNA quantification and genotyping in paired cervical and urine samples to detect cervical lesions. Arch. Gynecol. Obstet. 2014, 290, 299–308. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  12. Pathak, N.; Dodds, J.; Zamora, J.; Khan, K. Accuracy of urinary human papillomavirus testing for presence of cervical HPV: Systematic review and meta-analysis. BMJ 2014, 349. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  13. Vorsters, A.; Van Keer, S.; Biesmans, S.; Hens, A.; De Coster, I.; Goossens, H.; Ieven, M.; Van Damme, P. Long-term follow-up of HPV infection using urine and cervical quantitative HPV DNA testing. Int. J. Mol. Sci. 2016, 17, 750. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  14. Van Keer, S.; Willhauck-Fleckenstein, M.; Pattyn, J.; Butt, J.; Tjalma, W.A.A.; Van Ostade, X.; Hens, N.; Van Damme, P.; Waterboer, T.; Vorsters, A. First-void urine as a non-invasive liquid biopsy source to detect vaccine-induced human papillomavirus antibodies originating from cervicovaginal secretions. J. Clin. Virol. 2019, 117, 11–18. [Google Scholar] [CrossRef] [PubMed]
  15. Pattyn, J.; Panicker, G.; Willhauck-Fleckenstein, M.; Van Keer, S.; Téblick, L.; Pieters, Z.; Tjalma, W.A.A.; Matheeussen, V.; Van Damme, P.; Waterboer, T.; et al. Comparison of a VLP-based and GST-L1-based multiplex immunoassay to detect vaccine-induced HPV-specific antibodies in first-void urine. J. Med. Virol. 2020. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  16. Pattyn, J.; Van Keer, S.; Tjalma, W.; Matheeussen, V.; Van Damme, P.; Vorsters, A. Infection and vaccine-induced HPV-specific antibodies in cervicovaginal secretions. A review of the literature. Papillomavirus Res. 2019, 8, 100185. [Google Scholar] [CrossRef] [PubMed]
  17. Franceschi, S.; Chantal Umulisa, M.; Tshomo, U.; Gheit, T.; Baussano, I.; Tenet, V.; Tshokey, T.; Gatera, M.; Ngabo, F.; Van Damme, P.; et al. Urine testing to monitor the impact of HPV vaccination in Bhutan and Rwanda. Int. J. Cancer 2016, 139, 518–526. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  18. Senkomago, V.; Des Marais, A.C.; Rahangdale, L.; Vibat, C.R.T.; Erlander, M.G.; Smith, J.S. Comparison of urine specimen collection times and testing fractions for the detection of high-risk human papillomavirus and high-grade cervical precancer. J. Clin. Virol. 2016, 74, 26–31. [Google Scholar] [CrossRef] [PubMed]
  19. Rohner, E.; McGuire, F.H.; Liu, Y.; Li, Q.; Miele, K.; Desai, S.A.; Schmitt, J.W.; Knittel, A.; Nelson, J.A.E.; Edelman, C.; et al. Racial and Ethnic Differences in Acceptability of Urine and Cervico-Vaginal Sample Self-Collection for HPV-Based Cervical Cancer Screening. J. Women’s Health 2020, 29, 971–979. [Google Scholar] [CrossRef] [PubMed]
  20. Sellors, J.W.; Lorincz, A.T.; Mahony, J.B.; Mielzynska, I.; Lytwyn, A.; Roth, P.; Howard, M.; Chong, S.; Daya, D.; Chapman, W.; et al. Comparison of self-collected vaginal, vulvar and urine samples with physician-collected cervical samples for human papillomavirus testing to detect high-grade squamous intraepithelial lesions. CMAJ 2000, 163, 513–518. [Google Scholar] [PubMed]
  21. Tamalet, C.; Le Retraite, L.; Leandri, F.X.; Heid, P.; Sancho Garnier, H.; Piana, L. Vaginal self-sampling is an adequate means of screening HR-HPV types in women not participating in regular cervical cancer screening. Clin. Microbiol. Infect. 2013, 19. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  22. Racey, C.S.; Withrow, D.R.; Gesink, D. Self-collected HPV testing improves participation in cervical cancer screening: A systematic review and meta-analysis. Can. J. Public Health 2013, 104, e159–e166. [Google Scholar] [CrossRef] [PubMed]
  23. Verdoodt, F.; Jentschke, M.; Hillemanns, P.; Racey, C.S.; Snijders, P.J.F.; Arbyn, M. Reaching women who do not participate in the regular cervical cancer screening programme by offering self-sampling kits: A systematic review and meta-analysis of randomised trials. Eur. J. Cancer 2015, 51, 2375–2385. [Google Scholar] [CrossRef] [PubMed]
  24. Ducancelle, A.; Reiser, J.; Pivert, A.; Guillou-Guillemette, H.L.; Le Duc-Banaszuk, A.S.; Lunel-Fabiani, F. Home-based urinary HPV DNA testing in women who do not attend cervical cancer screening clinics. J. Infect. 2015, 71, 377–384. [Google Scholar] [CrossRef] [PubMed]
  25. Vorsters, A.; Van Damme, P.; Clifford, G. Urine testing for HPV: Rationale for using first void. BMJ 2014, 349, 6252. [Google Scholar] [CrossRef] [PubMed]
  26. Gakidou, E.; Nordhagen, S.; Obermeyer, Z. Coverage of Cervical Cancer Screening in 57 Countries: Low Average Levels and Large Inequalities. PLoS Med. 2008, 5, e132. [Google Scholar] [CrossRef]
  27. Van Doornum, G.J.J.; Guldemeester, J.; Osterhaus, A.D.M.E.; Niesters, H.G.M. Diagnosing herpesvirus infections by real-time amplification and rapid culture. J. Clin. Microbiol. 2003, 41, 576–580. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  28. Niesters, H.G.M. Molecular and diagnostic clinical virology in real time. Clin. Microbiol. Infect. 2004, 10, 5–11. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  29. Luttmer, R.; De Strooper, L.M.A.; Dijkstra, M.G.; Berkhof, J.; Snijders, P.J.F.; Steenbergen, R.D.M.; Van Kemenade, F.J.; Rozendaal, L.; Helmerhorst, T.J.M.; Verheijen, R.H.M.; et al. FAM19A4 methylation analysis in self-samples compared with cervical scrapes for detecting cervical (pre)cancer in HPV-positive women. Br. J. Cancer 2016, 115, 579–587. [Google Scholar] [CrossRef] [PubMed]
  30. Van Den Helder, R.; Van Trommel, N.E.; Van Splunter, A.P.; Lissenberg-Witte, B.I.; Bleeker, M.C.G.; Steenbergen, R.D.M. Methylation analysis in urine fractions for optimal CIN3 and cervical cancer detection. Papillomavirus Res. 2020, 9, 100193. [Google Scholar] [CrossRef] [PubMed]
  31. Bosschieter, J.; Bach, S.; Bijnsdorp, I.V.; Segerink, L.I.; Rurup, W.F.; Van Splunter, A.P.; Bahce, I.; Novianti, P.W.; Kazemier, G.; Van Moorselaar, R.J.A.; et al. A protocol for urine collection and storage prior to DNA methylation analysis. PLoS ONE 2018, 13. [Google Scholar] [CrossRef] [PubMed]
  32. Pattyn, J.; Van Keer, S.; Biesmans, S.; Ieven, M.; Vanderborght, C.; Beyers, K.; Vankerckhoven, V.; Bruyndonckx, R.; Van Damme, P.; Vorsters, A. Human papillomavirus detection in urine: Effect of a first-void urine collection device and timing of collection. J. Virol. Methods 2019, 264, 23–30. [Google Scholar] [CrossRef]
  33. Van Keer, S.; Tjalma, W.A.A.; Pattyn, J.; Biesmans, S.; Pieters, Z.; Van Ostade, X.; Ieven, M.; Van Damme, P.; Vorsters, A. Human papillomavirus genotype and viral load agreement between paired first-void urine and clinician-collected cervical samples. Eur. J. Clin. Microbiol. Infect. Dis. 2018, 37, 859–869. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  34. Tshomo, U.; Franceschi, S.; Tshokey, T.; Tobgay, T.; Baussano, I.; Tenet, V.; Snijders, P.J.F.; Gheit, T.; Tommasino, M.; Vorsters, A.; et al. Evaluation of the performance of Human Papillomavirus testing in paired urine and clinician-collected cervical samples among women aged over 30 years in Bhutan. Virol. J. 2017, 14, 74. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  35. Wardak, S. Human Papillomavirus (HPV) and Cervical Cancer. Available online: https://www.who.int/en/news-room/fact-sheets/detail/human-papillomavirus-(hpv)-and-cervical-cancer (accessed on 5 October 2020).
  36. Verlaat, W.; Van Leeuwen, R.W.; Novianti, P.W.; Schuuring, E.; Meijer, C.J.L.M.; Van Der Zee, A.G.J.; Snijders, P.J.F.; Heideman, D.A.M.; Steenbergen, R.D.M.; Wisman, G.B.A. Host-cell DNA methylation patterns during high-risk HPV-induced carcinogenesis reveal a heterogeneous nature of cervical pre-cancer. Epigenetics 2018, 13, 769–778. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  37. De Strooper, L.M.A.; Berkhof, J.; Steenbergen, R.D.M.; Lissenberg-Witte, B.I.; Snijders, P.J.F.; Meijer, C.J.L.M.; Heideman, D.A.M. Cervical cancer risk in HPV-positive women after a negative FAM19A4/mir124-2 methylation test: A post hoc analysis in the POBASCAM trial with 14 year follow-up. Int. J. Cancer 2018, 143, 1541–1548. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  38. Wentzensen, N.; Schiffman, M.; Palmer, T.; Arbyn, M. Triage of HPV positive women in cervical cancer screening. J. Clin. Virol. 2016, 76, S49–S55. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  39. Leeman, A.; del Pino, M.; Molijn, A.; Rodriguez, A.; Torné, A.; de Koning, M.; Ordi, J.; van Kemenade, F.; Jenkins, D.; Quint, W. HPV testing in first-void urine provides sensitivity for CIN2+ detection comparable with a smear taken by a clinician or a brush-based self-sample: Cross-sectional data from a triage population. BJOG Int. J. Obstet. Gynaecol. 2017, 124, 1356–1363. [Google Scholar] [CrossRef] [PubMed]
  40. BE 71030031000; Biobank Antwerpen, BBMR-ERIC; No. Access: (25), [BIORESOURCE].
  41. Payan, C.; Ducancelle, A.; Aboubaker, M.H.; Caer, J.; Tapia, M.; Chauvin, A.; Peyronnet, D.; Le Hen, E.; Arab, Z.; Legrand, M.C.; et al. Human papillomavirus quantification in urine and cervical samples by using the Mx4000 and LightCycler general real-time PCR systems. J. Clin. Microbiol. 2007, 45, 897–901. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  42. Hesselink, A.T.; Berkhof, J.; Van Der Salm, M.L.; Van Splunter, A.P.; Geelen, T.H.; Van Kemenade, F.J.; Bleeker, M.G.B.; Heideman, D.A.M. Clinical validation of the HPV-Risk assay, a novel real-time PCR assay for detection of high-risk human papillomavirus DNA by targeting the E7 region. J. Clin. Microbiol. 2014, 52, 890–896. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  43. Verlaat, W.; Snijders, P.J.F.; Novianti, P.W.; Wilting, S.M.; De Strooper, L.M.A.; Trooskens, G.; Vandersmissen, J.; Van Criekinge, W.; Wisman, G.B.A.; Meijer, C.J.L.M.; et al. Genome-wide DNA methylation profiling reveals methylation markers associated with 3q gain for detection of cervical precancer and cancer. Clin. Cancer Res. 2017, 23, 3813–3822. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  44. Verlaat, W.; Snoek, B.C.; Heideman, D.A.M.; Wilting, S.M.; Snijders, P.J.F.; Novianti, P.W.; Van Splunter, A.P.; Peeters, C.F.W.; Van Trommel, N.E.; Massuger, L.F.A.G.; et al. Identification and validation of a 3-gene methylation classifier for hpv-based cervical screening on self-samples. Clin. Cancer Res. 2018, 24, 3456–3464. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  45. Snellenberg, S.; Strooper, L.M.A.D.; Hesselink, A.T.; Meijer, C.J.L.M.; Snijders, P.J.F.; Heideman, D.A.M.; Steenbergen, R.D.M. Development of a multiplex methylation-specific PCR as candidate triage test for women with an HPV-positive cervical scrape. BMC Cancer 2012, 12, 551. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  46. Overmeer, R.; Henken, F.; Snijders, P.; Claassen-Kramer, D.; Berkhof, J.; Helmerhorst, T.; Heideman, D.; Wilting, S.; Murakami, Y.; Ito, A.; et al. Association between dense CADM1 promoter methylation and reduced protein expression in high-grade CIN and cervical SCC. J. Pathol. 2008, 215, 388–397. [Google Scholar] [CrossRef] [PubMed]
Molecules 26 01989 g001 550
Figure 1. Flow diagram of the study; 32 women subscribed online, whereof 28 eligible women were included. Each woman received a study package at home as described. From those 28 women, three women were excluded (reasons for exclusion listed in the figure). All 25 included women collected three consecutive samples using three different Colli-Pee® urine devices with collector tubes that differ in size. On the same day of collection (or at the latest, one day after collection), the urine samples were sent back to the lab via postal mail where they were aliquoted and stored at −80 °C prior to further analysis. On each sample, DNA was extracted using the EM. On the samples collected with Colli-Pee® 20 mL and 10 mL, three and two other DNA extraction methods were performed, respectively. All DNA extracts were analyzed for GAPDH and phocine herpesvirus 1 (PhHV-1) using an in-house qPCR. In addition, samples were analyzed using the human papillomavirus (HPV)-Risk Assay and methylation-specific qPCR at Self-Screen B.V. n; number, EM; extraction method, SN; supernatant.
Figure 1. Flow diagram of the study; 32 women subscribed online, whereof 28 eligible women were included. Each woman received a study package at home as described. From those 28 women, three women were excluded (reasons for exclusion listed in the figure). All 25 included women collected three consecutive samples using three different Colli-Pee® urine devices with collector tubes that differ in size. On the same day of collection (or at the latest, one day after collection), the urine samples were sent back to the lab via postal mail where they were aliquoted and stored at −80 °C prior to further analysis. On each sample, DNA was extracted using the EM. On the samples collected with Colli-Pee® 20 mL and 10 mL, three and two other DNA extraction methods were performed, respectively. All DNA extracts were analyzed for GAPDH and phocine herpesvirus 1 (PhHV-1) using an in-house qPCR. In addition, samples were analyzed using the human papillomavirus (HPV)-Risk Assay and methylation-specific qPCR at Self-Screen B.V. n; number, EM; extraction method, SN; supernatant.
Molecules 26 01989 g001
Molecules 26 01989 g002 550
Figure 2. Violin plot of qPCR Cq values for PhHV-1 for all 25 included samples. EM was used for all extraction volumes, CF800_EM for both 10 mL and 20 mL, AM_EM, CF800_QIA only for 20 mL, and CF3000_EM only for 10 mL. Calculated cut-offs for each extraction method are; AM_EM: 36.26, EM: 35.83, CF800_EM: 36.40, CF800_QIA: 40.00, CF3000_EM: 3 5.81. Significance levels are represented in the figure by an asterisk (** p < 0.01; *** p < 0.001).
Figure 2. Violin plot of qPCR Cq values for PhHV-1 for all 25 included samples. EM was used for all extraction volumes, CF800_EM for both 10 mL and 20 mL, AM_EM, CF800_QIA only for 20 mL, and CF3000_EM only for 10 mL. Calculated cut-offs for each extraction method are; AM_EM: 36.26, EM: 35.83, CF800_EM: 36.40, CF800_QIA: 40.00, CF3000_EM: 3 5.81. Significance levels are represented in the figure by an asterisk (** p < 0.01; *** p < 0.001).
Molecules 26 01989 g002
Molecules 26 01989 g003 550
Figure 3. Boxplots representing the Cq values of GAPDH, HBB, and ACTB for each evaluated collection volume using EM (upper figures) and CF800_EM (lower figures). Individual Cq values are represented as dots. All data were analyzed using the non-parametric Wilcoxon signed-rank testing. Significant differences are represented in the figure by an asterisk (p < 0.05).
Figure 3. Boxplots representing the Cq values of GAPDH, HBB, and ACTB for each evaluated collection volume using EM (upper figures) and CF800_EM (lower figures). Individual Cq values are represented as dots. All data were analyzed using the non-parametric Wilcoxon signed-rank testing. Significant differences are represented in the figure by an asterisk (p < 0.05).
Molecules 26 01989 g003
Molecules 26 01989 g004 550
Figure 4. Boxplots representing the Cq value of GAPDH, HBB, and ACTB for each DNA extraction method on both 20 mL samples (upper figures) and 10 mL sample volume (lower figures). Individual Cq values are represented as dots. All data were analyzed using the non-parametric Wilcoxon signed-rank testing. Significance levels are represented in the figure by an asterisk (* p < 0.05; ** p < 0.01; *** p < 0.001).
Figure 4. Boxplots representing the Cq value of GAPDH, HBB, and ACTB for each DNA extraction method on both 20 mL samples (upper figures) and 10 mL sample volume (lower figures). Individual Cq values are represented as dots. All data were analyzed using the non-parametric Wilcoxon signed-rank testing. Significance levels are represented in the figure by an asterisk (* p < 0.05; ** p < 0.01; *** p < 0.001).
Molecules 26 01989 g004
Table
Table 1. HPV DNA Cq values (either HPV-31, -33, -35, -39, -45, -51, -52, -56, -58, -59, -66, -67, or -68) for all different first-void (FV) urine collection volumes and DNA extraction method combinations. Percentage of positive samples/extract is noted underneath. There were no significant differences between groups (p > 0.05). EM; EasyMag, CF; Centrifugation.
Table 1. HPV DNA Cq values (either HPV-31, -33, -35, -39, -45, -51, -52, -56, -58, -59, -66, -67, or -68) for all different first-void (FV) urine collection volumes and DNA extraction method combinations. Percentage of positive samples/extract is noted underneath. There were no significant differences between groups (p > 0.05). EM; EasyMag, CF; Centrifugation.
HPV Cq Values
AM_EMEMCF800_EMCF800_QIACF3000_EM
20 mL4 mL10 mL20 mL10 mL20 mL20 mL10 mL
ID1----38.78---
ID222.0817.9019.1723.1717.2822.7524.7521.65
ID3--------
ID4--35.46-32.26--32.57
ID5--------
ID636.7134.32-29.11-28.8925.9733.53
ID729.6423.5824.6526.2523.6222.8124.8925.70
ID8--------
ID9----30.83--37.46
ID10--------
ID1222.1625.0924.0423.7320.9421.6622.8021.12
ID1319.8221.9725.6120.8924.1519.4018.9924.57
ID14--------
ID1539.24-37.87-----
ID16--------
ID1734.9230.3433.5234.5535.9438.5933.9635.50
ID1836.19-37.00-31.2536.3938.1631.07
ID1924.6322.9224.5726.1722.5824.4325.2623.38
ID21--------
ID22--------
ID2331.59-35.1135.7332.9838.98-36.29
ID24--------
ID2529.9038.9027.9330.6530.1230.6733.1028.37
ID27--------
ID28--------
Percent positive (%)44.0032.0044.0036.0052.0040.0036.0048.00
Publisher’s Note: MDPI stays neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Share and Cite

MDPI and ACS Style

Téblick, L.; Van Keer, S.; De Smet, A.; Van Damme, P.; Laeremans, M.; Rios Cortes, A.; Beyers, K.; Vankerckhoven, V.; Matheeussen, V.; Mandersloot, R.; et al. Impact of Collection Volume and DNA Extraction Method on the Detection of Biomarkers and HPV DNA in First-Void Urine. Molecules 2021, 26, 1989. https://doi.org/10.3390/molecules26071989

AMA Style

Téblick L, Van Keer S, De Smet A, Van Damme P, Laeremans M, Rios Cortes A, Beyers K, Vankerckhoven V, Matheeussen V, Mandersloot R, et al. Impact of Collection Volume and DNA Extraction Method on the Detection of Biomarkers and HPV DNA in First-Void Urine. Molecules. 2021; 26(7):1989. https://doi.org/10.3390/molecules26071989

Chicago/Turabian Style

Téblick, Laura, Severien Van Keer, Annemie De Smet, Pierre Van Damme, Michelle Laeremans, Alejandra Rios Cortes, Koen Beyers, Vanessa Vankerckhoven, Veerle Matheeussen, Renee Mandersloot, and et al. 2021. "Impact of Collection Volume and DNA Extraction Method on the Detection of Biomarkers and HPV DNA in First-Void Urine" Molecules 26, no. 7: 1989. https://doi.org/10.3390/molecules26071989

Article Metrics

Back to TopTop