Login processing...

Trial ends in Request Full Access Tell Your Colleague About Jove

Genetics

Optimized High Quality DNA Extraction from Formalin-Fixed Paraffin-Embedded Human Atherosclerotic Lesions

doi: 10.3791/61452 Published: February 12, 2021
Sabine Bauer1,2,4, Jessica Pauli1,2, Jaroslav Pelisek1,3

Abstract

Formalin-fixed paraffin-embedded (FFPE) tissues represent a valuable source for molecular analyses and clinical genomic studies. These tissues are often poor in cells or difficult to process. Therefore, nucleic acids need to be carefully isolated. In recent years, various methods for DNA isolation have been established for tissues from many diseases, mostly cancer. Unfortunately, genomic DNA extracted from FFPE tissues is highly degraded due to the cross-linking between nucleic acid strands and proteins, as well as random breakings in sequence. Therefore, DNA quality from these samples is markedly reduced, making it a challenge for further molecular downstream analyses. Other problems with difficult tissues are, for example, the lack of cells in calcified human atherosclerotic lesions and fatty tissue, small skin biopsies, and consequently low availability of the desired nucleic acids as it is also the case in old or fixed tissues.

In our laboratories, we have established a method for DNA extraction from formalin-fixed atherosclerotic lesions, using a semi-automated isolation system. We compared this method to other commercially available extraction protocols and focused on further downstream analyses. Purity and concentration of the DNA were measured by spectrometry and fluorometry. The degree of fragmentation and overall quality were assessed.

The highest DNA quantity and quality was obtained with the modified blood DNA protocol for the automated extraction system, instead of the commercial FFPE protocol. With this step-by-step protocol, DNA yields from FFPE samples were in average four times higher and fewer specimens failed the extraction process, which is critical when dealing with small-vessel biopsies. Amplicon sizes from 200–800 bp could be detected by PCR. This study shows that although DNA obtained from our FFPE tissue is highly fragmented, it can still be used for successful amplification and sequencing of shorter products. In conclusion, in our hands, the automated technology appears to be the best system for DNA extraction, especially for small FFPE tissue specimen.

Introduction

Formalin fixation followed by paraffin embedding (FFPE) is a standard procedure for long-term preservation of pathological specimen in biobanking1. These samples provide a valuable source for histological studies as well as molecular analyses, especially genetic studies2. Further advantages of FFPE tissues are better long-term storage, lower costs, and easier storage conditions. Our intention here is to provide a reliable and easy-to-use protocol for reproducible nucleic acid isolation from small amounts of FFPE sections, since high quality DNA extraction is the first crucial step in a wide range of molecular techniques and FFPE tissues are the most available source of samples.

New scientific approaches, such as next-generation sequencing (NGS) and “omics” research approaches, require high quality of nucleic acids3,4,5. Extracting DNA from FFPE tissue samples remains a challenging endeavor. DNA from FFPE samples can vary widely in quality and quantity depending upon its age and fixation conditions. Formalin, the most frequently used compound, leads to DNA-protein crosslinking6,7,8 and causes unspecific random breakage in the nucleotide sequence9. This may significantly impact downstream genomic analyses, since crosslinking can disable polymerase chain reaction (PCR) amplification6,10. Due to contaminants during the fixation process, purity of the DNA isolated from FFPE samples is often limited. In recent years, various methods for DNA isolation were established, mostly from cancer tissue specimens2,11,12,13.

In general, protocols for the extraction of nucleic acids from FFPE tissue can be differentiated into three main groups. The first, most commonly used group of methods includes commercially available silica-based column systems14. The second group involves manual organic phase extraction methods with phenol and chloroform, first described by Joseph Sambrook and David W. Russell15. As a third group, automated systems were established over the last years such as liquid handling systems as well as paramagnetic particle-based systems16. Each of the three named systems holds different advantages and disadvantages such as hazardous chemicals (i.e., xylene, phenol, chloroform), high costs17, manpower18, and time consumption19. Especially, for the difficult tissue specimen as well as high throughput analyses standardization, reproducibility, relatively low time-consumption, manpower, and costs are the most relevant features in finding a suitable method for nucleic acid isolation20. Automated extraction methods are known to show better reproducible results and are more sensitive for small biopsies. Moreover, less amount of tissue or blood is needed and the risk of clogging of the system due to high amounts of paraffin is reduced. Although machines for automated nucleic acid extraction and the needed kits are more expensive compared to manual methods, they are still convincing due to less problematic extraction processes. Literature search provides a lot of publications that illustrate a direct comparison between manual, column-based, and automated DNA and RNA extraction methods from different tissues and organisms, such as plants, animals, and humans as well as cells in culture20,21,22. There are also evidences present in literature to show that DNA and RNA isolated from 10-year old snap frozen tissue can be used for downstream analyses such as PCR, quantitative PCR, NGS, methylation analyses, and cloning9,23,24,25,26.

The major problem with, for example, aged human vascular tissue, as well as small tissue biopsies, especially concerning FFPE samples, is the lack of cells in the highly calcified atherosclerotic lesions, which consequently leads to low concentrations of nucleic acids1. Although several methods for DNA extraction from FFPE tissue have already been established and are widely used, the manual sample preparation methods require long hands-on time27 and toxic reagents such as xylene or phenol are necessary for deparaffinization2. As described, the deparaffinization process is a crucial time-consuming step (e.g., around 30 min) that markedly affects the quality and quantity of the extracted DNA (e.g., toxic effects on DNA, such as fragmentation and degradation of deparaffinization solution and high temperatures)28. Recently developed new DNA extraction protocols focus on using other non-toxic deparaffinization solutions, repair strategies and automated bead technologies. In particular, automated and semi-automated methods have been shown to be successful in DNA extraction with efficient recovery, lack of cross contamination, and easy performance29. We have established a protocol that overcomes these limitations. As a result, our technique allows a reduction of processing and hands-on time at highest quantitative and qualitative standards.

Especially for reproducible high-throughput analyses such as genotyping, epigenomic studies, and RNA sequencing the handling of FFPE specimen with column-based purification systems is often difficult and time consuming (e.g., long deparaffinization steps, column clogging, and long hands-on times). Clogging of the silica membranes due to high amount of paraffin is the major issue. Other circumstances that can worsen the isolation of high-quality nucleic acids are small amounts of tissue such as micro-biopsies of skin, small mouse tissue, very fatty or calcified tissue as plaques, ossified tissue, and aged samples. Especially in diagnosis and forensics, automated and semi-automated systems such as liquid handling or paramagnetic particle-based extraction methods became more and more essential over the last few years30,31, mainly due to relatively low hands-on times and the possibility of standardization. Most of the already published protocols work perfectly for smooth tissues with high or medium amounts of cells such as tumor biopsies or plant tissue13,22,32. Literature about methods for semi-automated particle-based methods used for isolating DNA from relatively hard-to-handle tissue such as fixed single cells, calcified vessels, collagen rich tissue, and fatty tissue with low cell numbers are only poorly described33.

In this study, an optimized semi-automated method for DNA isolation from vascular paraffin embedded sections is described, comparing it to two manual column-based protocols. DNA quantity, purity, and the extent of fragmentation were used for validation. The commercially available blood DNA protocol, was used as a starting point and the manual steps of the semi-automated system were subsequently optimized for the use of FFPE as well as fresh frozen tissue samples from human and animal tissue, combining steps from the FFPE and the tissue protocol. The automated step of this protocol is pre-installed on the instrument and depends on the used kit (here, the blood DNA kit). With the described semi-automated cartridge-based system it is possible to isolate DNA from blood, fresh-frozen tissue, formalin-fixed tissue and even single cells with the same protocol, machine, kit and consumables, instead of using different protocols and kits for the instrument, as it is recommended by the company. There are only minor differences in the protocols, such as one buffer and some incubation times for the different applications, which makes this protocol very useful for extracting DNA from all kinds of tissues. Our protocol is primarily optimized for calcified, poor in cells and fibrous human vascular tissue, but can of course be used and further optimized for all kinds of difficult tissues mentioned above.

Summarized, for researchers in the cardiovascular field working on atherosclerosis (e.g., aorta, carotid arteries, coronary arteries) we provide an easy-to-use, point-by-point protocol for semi-automated DNA extraction from vascular FFPE samples.

Subscription Required. Please recommend JoVE to your librarian.

Protocol

The permission to collect human carotid atherosclerotic specimens in our biobank was approved by the local Hospital Ethics Committee (2799/10, Ethikkommission der Fakultät für Medizin der Technischen Universität München, Munich, Germany). Written informed consent was obtained from all patients. Experiments were performed in accordance with the principles of the Declaration of Helsinki.

1. Tissue preparation

  1. Prepare 5–8 tissue sections of 10 µm from the FFPE sample with the microtome and transfer it in a 1.5 mL tube. It is not necessary to reduce the excess of paraffin from the block.
    NOTE: Thinner single sections instead of one large section accelerate the buffer reaction. Discard the first sections due to O2 exposure. For bigger samples, it is also possible to use fewer sections.
  2. Centrifuge these tubes in a bench top centrifuge, set to 5,000 x g for 1 min at room temperature to collect each sample on the bottom of the tube.
    CAUTION: Too long centrifugation leads to clotting of the sample and complicates the lysis.

2. Lipid dissolution and deparaffinization

NOTE:This step is needed for deparaffinization and lipid digestion. The buffer used is less toxic than commercial deparaffinization solutions.

  1. Add 300 µL of the commercially available incubation buffer and 6 µL of 1-thioglycerol to each tube.
    NOTE: Do not use more than 300 µL as this is the maximum volume of the automation system cartridge.
  2. Vortex for 10 s and incubate the sample for 10 min at 80 °C and 500 rpm in a heating block to solubilize paraffin.
    CAUTION: The tissue should be completely dissolved in the end. If necessary, vortex several times during incubation.

3. Sample and protein digestion

NOTE:Native digestion with protease K is crucial to have clean DNA extracts without proteins. It also reduces any contaminating proteins present. Furthermore, nucleases are also destroyed to save the DNA34. This overnight step is also needed for complete sample digestion.

  1. Let the sample cool down to 60 °C and then add 30 µL of the provided Proteinase K solution.
  2. Vortex again and incubate the mixture at 65 °C and 500 rpm overnight (4–20 h) in a heating block. Vortex the samples during incubation from time to time for complete sample digestion.
    NOTE: Overnight incubation leads to better results. Mixing steps are recommended every 30–60 min. In the end, there should not be any visual tissue piece inside the tube.

4. Cell lysis

  1. Add 400 µL of the lysis buffer, provided in the blood kit and vortex shortly.
  2. Incubate the sample again at 65 °C for 30 min with 500 rpm.
  3. Let the sample cool down to room temperature. The paraffin will harden on top.
    CAUTION: Do not vortex again, to keep the paraffin separated from the sample. Otherwise, the paraffin is mixed with the tissue, which destroys the sample. The sample will be collected in step 6.1.

5. Preparation of the pre-dispensed cartridges

  1. Turn on the machine, as well as the associated tablet computer.
  2. Start the software app and click on the Door button to open the instrument.
  3. Remove the rack from the instrument and insert the pre-filled cartridge into the probe rack. Ensure that the cartridge clicks twice when into place and remove the sealing foil.
  4. Add the plunger in the last (8) well of the cartridge. It serves as pipette tip in the instrument.
  5. Fill the provided 0.5 mL elution tubes with 65 µL of elution buffer, provided with the kit. Leave the tubes open and insert them into the dedicated position in the front part of the rack, after the cartridge.
    NOTE: The minimum volume for elution is 60 µL. The system will lose 5–10 µL of the added elution volume.

6. Automated DNA extraction

  1. Carefully puncture the paraffin on top of the 1.5 mL tube from step 4.3 to reach to the clean sample at the bottom of the tube without mixing it with paraffin again.
  2. Transfer the whole mixture (730 µL) of the prepared sample in the first well of the cartridge.
  3. Insert the rack into the automated DNA extraction machine. Ensure that the rack locks in the back of the machine first and in the front afterwards.
  4. Start the run by clicking the upper left orange Start button in the software. A window with different pre-installed protocols will open. Select Blood DNA protocol on the instrument. Confirm that plunger, elution tube, and sample were added by clicking yes in the software. The door of the instrument will close automatically, and the run starts (the light will turn green). The run will take approximately 38 min. No further calibration is needed.
    NOTE: Watch until the system has picked up the plungers for all samples in the rack. If this is not happening the system stops automatically and the machine protocol must be restarted.
  5. Ensure that the system performs the automated lysis step in the first well of the cartridge, followed by washing steps in wells 3 to 7. There is no further programming step needed. The complete program is pre-installed by the company.
  6. Once done, ensure that the system elutes the DNA in the prepared elution tubes via the added plunger. The magnetic particles stay in the plunger. The plunger in the end goes back to the last well of the cartridge.

7. Finish the run

  1. When the run is completed (the machine shows green blinking light), open the instrument by clicking the button for opening (door-sign) and remove the rack from the system.
  2. Discard the cartridges.
  3. Reinsert the empty rack to the instrument and close the door via the door button in the upper-right corner. Close the software app and turn off the machine, as well as the tablet computer.
  4. Store eluates at -20 °C for long-term storage or at 4 °C for short-term storage or use it directly for downstream analysis or concentration measurements.

Subscription Required. Please recommend JoVE to your librarian.

Representative Results

For the establishment of the protocol, 5 FFPE tissue blocks from patients with atherosclerosis of the carotid artery were used. DNA was isolated with an optimized semi-automated protocol (kit C) as well as with two commercially available manual column-based protocols (kit A and kit B, see Table of Materials). DNA extraction with kit A and B was performed according to the manufacturer´s protocol. The only change that was made in the protocol of the two commercially available kits (kit A and kit B): deparaffinization in the beginning was performed twice due to high amounts of paraffin surrounding the sections. After deparaffinization with xylene, DNA was bound to the column-membrane and washed three times. After drying the membrane by centrifugation, DNA was eluted with 60 µL of the provided elution buffer.

To determine the optimal quantity of samples needed for reproducible results from every patient, different amounts of material were taken. Consecutive tissue sections of 2 x 10 µm (20 µm in total), 5 x 10 µm (50 µm in total), and 8 x 10 µm (80 µm in total) were used (Figure 1). The quality and quantity of total genomic DNA isolated with the automated system and the two-manual column-based systems were assessed both with spectrometry, a microplate reader spectrometric system as well as fluorometry. Fragmentation analysis was performed using automated screen-tape technology and polymerase chain reaction (PCR). Statistical analysis was done using commercially available software (see Table of Materials).

The semi-automated protocol leads to higher quantity of the extracted DNA
Using micro-volume spectrometry and plate reader spectrometry as well as fluorometry as shown in Figure 2, the total amount of genomic DNA was compared for the different amounts of tissue sections (20 µm, 50 µm, 80 µm in total). A linear increase of DNA concentration was obtained with the cartridge-based semi-automated kit C, with all three quantification methods. For the manual kits A and B, no significant differences were observed between 20 µm, 50 µm, and 80 µm sections. The mean concentration of all five tissue samples measured with micro-volume spectrometry and microplate reader technology for DNA extracted with the semi-automated protocol (Figure 2A,B, Table 1) showed a significant, four times higher, concentration (45 ng/µL) compared to the column-based protocols A and B (p = 0.016). Kit A attained mean concentrations of 12.5 ng/µL, while Kit B attained only 8.5 ng/µL. Figure 3 shows the quality of the extracted DNA with the three named methods. Summing up that there is no big difference in quality. The semi-automated kit shows more stable quality, the measured quantities are comparable. Similar results were found by using fluorimetric measurements of the DNA concentration (Figure 2C). Mean concentrations of DNA using kit A were further reduced to 3 ng/µL compared to the spectrometric analysis. Summarizing the quantity of DNA, the automated protocol turned out to be the most efficient method for low cells-tissue samples.

Automated extraction protocol leads to a better quality of the extracted DNA
Furthermore, the quality of DNA isolated with the three different protocols was assessed spectrophotometrically, both using spectrophotometer and microplate reader, calculating the A260/280 ratio (Figure 3A,B and Table 2). Nucleic acids have their absorbance maximum at 260 nm. Purity of high quality DNA is generally in the range from A260/280 values of 1.6–1.8, as evidenced by the two dashed lines in Figure 3A,B35. The mean ratio of the manual column-based kit A was 1.92 ± 0.6 in spectrometry and 2.58 ± 1.2 measured with microplate-reader technology. Kit B showed smaller ratios (1.45 ± 0.3 and 1.85 ± 0.7). DNA isolated with the semi-automated kit C showed purity ratios of 1.4 ± 0.07 in spectrometry and 1.68 ± 0.05 calculated with the microplate reader. In both the measurements, the automated isolation method showed less variation in purity ratio than the manual kits but only kit A showed significant differences in paired t-test analysis because of the huge scattering (p = 0.0025 and p < 0.001). Regarding the microplate measurement, all samples isolated with the automate system passed the purity criteria (ratios between 1.6 and 1.8), whereas kit A and kit B in many cases failed these criteria (p < 0.001). Spectrometry (Figure 3A) evidenced that not all samples isolated with the optimized cartridge system (minimum ratio = 1.36) reached the defined purity threshold (dashed lines, indicating the A260/280 ratio of 1.6 and 1.8), indicating buffer contamination. In addition, huge variation of the calculated ratio for kits A and B was observed. Consequently, semi-automated DNA isolation provides samples with comparable and reproducible quality, whereas the DNA quality is widely fluctuating with column-based isolation methods. Another quality check was performed using DV200 calculation (Figure 3A, Table 2). Here, the manual column-based extraction system A showed a value of 90% ± 3.8 for fragments bigger than 200 bp, whereas kit B only showed 85% ± 7.1 (p = 0.01). Also, in this analysis, DNA extracted with the semi-automated protocol showed the highest percentage of fragments bigger than 200 bp (92% ± 3.6).

Summing it up, quality of the DNA extracted with the semi-automated system was more stable and reproducible, whereas DNA isolated with the column-based systems showed more variation in quality ratios. DV200 indicated similar quality for kits A and C, whereas kit B had less fragments bigger than 200 bp.

DNA fragmentation is independent of the used protocol
Fragmentation of the DNA was assessed with semi-automated screen tape technology. In Figure 4A, representative gels are shown to display the extent of fragmentation of all samples used in this study. Dark color indicates a higher density whereas grey shaded images indicate lower densities. Here, similar patterns were observed for all samples and in all three kits. The first three samples show the darkest region (which equals the highest accumulation of the fragmented DNA), in the lower part of the gel representing the smaller DNA fragments, samples from patient 4 and 5 show more (denser) fragments in the upper part of the gel, indicating less fragmented DNA. In Figure 4B, the difference in DNA fragmentation using various amounts of material (20 µm, 50 µm, and 80 µm) is shown for one representative sample using all three isolation strategies. Electropherograms show the corresponding fragment distribution. The data is summarized in Table 3. Here, the only visual difference between the three kits was found in the graphs of the 20 µm sections, with the automate kit showing a clearer electropherogram with more DNA detected. For 50 µm and 80 µm sections, no visible difference in the electropherogram was found between the different kits used in the study.

Figure 5A shows the mean distribution of the fragment sizes for the semi-automated cartridge system kit C as well as for the two manual kits A and B. Mean distribution of the fragment sizes for the automated system shows the following results: 5% of the DNA fragments were smaller than 200 bp, 62% sized between 200 bp and 1500 bp and 29% of the DNA fragments were longer than 1,500 bp. Higher percentage of augmented DNA fragmentation was measured with Kit B (12%) and Kit A (8%). Medium size fragments were similar for kit A (62%) and kit B (57%). Regarding the longer DNA fragments, no significant difference (kit A 26%, kit B 27%) were observed. This leads to the conclusion that DNA isolated with the optimized semi-automated kit (kit C) seems to be less fragmented than DNA isolated with column-based kits.

The fragmentation peak (highest amount of DNA for a certain fragment size) in all three kits was analyzed for each of the five tissue samples (Figure 5B). No differences between the three isolation methods could be detected concerning the overall DNA fragmentation. Of note, regardless of the kit utilized, samples 1 to 3 show an average maximum peak between 280 bp and 620 bp whereas samples 4 and 5 are less fragmented with an average fragmentation peak between 1,200 bp and 1,800 bp. These results indicate that DNA fragmentation is affected by the quality of the specimens itself.

DNA extracted with the semi-automated kit is suitable for PCR analysis
Ultimately, eight DNA samples isolated with the optimized protocol were used for downstream analysis performing PCR of different fragment lengths. Appropriate primers for the beta-actin housekeeping gene were chosen. A primary smooth muscle cell line served as a control (Figure 6). By displaying the detectable fragments in agarose gel electrophoresis, both samples with large maximum fragments (500 bp–800 bp for samples 1, 2, and 8) as well as samples with only 200 bp of maximum fragments were detected (samples 6 and 7), independent of the extraction method used.

Figure 1
Figure 1: Experimental workflow. The main steps of sample preparation and semi-automated DNA extraction are shown in the context of the used specimens and in comparison, with the manual DNA extraction kits A and B. Please click here to view a larger version of this figure.

Figure 2
Figure 2: Concentration measurement. The upper part (A-C) shows the DNA concentrations measured with spectrometry, microplate reader technology and fluorometry using 20 µm, 50 µm, and 80 µm sections (each, n = 5) for all three different kits applied. The lower part shows the distribution of the DNA concentrations of five samples (80 µm) measured with spectrometry (D), microplate reader technology (E) and fluorometry (F). p-values are calculated with the paired t-test, p < 0.05 was considered significant. Please click here to view a larger version of this figure.

Figure 3
Figure 3: Purity of the isolated DNA. The purity of DNA was assessed by calculating the A260/280 ratio in two different spectrometers (A,B) for all three different kits (n = 15). Dashed lines demonstrate the optimal ratio (1.6–1.8). (C) shows the DV200 (fragments >200 bp) in % calculated via fragmentation analysis. P-values are calculated with Mann-Whitney test and shown in the graph accordingly, p < 0.05 was considered significant. Please click here to view a larger version of this figure.

Figure 4
Figure 4: Representative images from the fragmentation analysis. The fragmentation of each individual sample 1–15 is shown in the screen-tape traces. For every sample (n = 5) different amount of DNA from 20 µm, 50 µm, and 80 µm sections were analyzed separately (n = 3 for each sample) (A). (B) shows the DNA fragmentation of one representative specimen for 20 µm, 50 µm, and 80 µm sections for all three kits. Please click here to view a larger version of this figure.

Figure 5
Figure 5: Fragment distribution by screen-tape analysis. (A) shows the distribution of short, medium, and long fragments within the samples isolated with different kits. (B) shows the maximum fragmentation peak of the DNA isolated from samples 1–5 plotted for the individual kits. For every kit, the 20 µm, 50 µm and 80 µm sections of each samples are pooled. p-values are calculated with paired multiple t-test and shown in the graph, p < 0.05 was considered significant. Please click here to view a larger version of this figure.

Figure 6
Figure 6: Fragmentation analysis with PCR. This gel electrophoresis shows the PCR products with different amplicon lengths of the beta-actin housekeeping gene for eight different samples and one control cell line. Lanes are named as follows: 1 = 100 bp, 2 = 200 bp, 3 = 300 bp, 4 = 400 bp, 5 = 500 bp, 6 = 600 bp, 7 = 700 bp, 8 = 800 bp, 9 = 1,000 bp, and 10 = 1,300 bp. Please click here to view a larger version of this figure.

Kit A Kit B Kit C
Spectrometer max concentration [ng/µl] 26.2 13.25 72.35
min concentration [ng/µl] 8.45 7.75 23.55
mean concentration [ng/µl] 15.96 10.89 47.72
Microplate reader max concentration [ng/µl] 24 13.9 56.2
min concentration [ng/µl] 5.2 0 18.6
mean concentration [ng/µl] 12.5 7.4 41.5
Fluorometer max concentration [ng/µl] 10.3 23.4 47.6
min concentration [ng/µl] 0.211 0.842 12.5
mean concentration [ng/µl] 3.369 14.64 33.1

Table 1: Results of quantitative analysis. This table shows the minimum, maximum, and mean concentration, of the DNA isolated from the five patients with the three different kits. Concentrations were measured spectrometrically using micro spectrometer and microplate reader, as well as fluorometrically.

Sample µm Kit Microplate 260/280 Spectrometer 260/280 DV200 [%]
Patient 1 20 Kit A 6 1.65 90.72
Patient 1 50 Kit A 1.8 1.71 90
Patient 1 80 Kit A 2.09 1.345 88.98
Patient 2 20 Kit A 1.88 1.53 87.14
Patient 2 50 Kit A 2.29 1.465 92.46
Patient 2 80 Kit A 4.36 2.68 84.78
Patient 3 20 Kit A 1.91 1.85 89.24
Patient 3 50 Kit A 2.21 1.92 90.86
Patient 3 80 Kit A 2.06 1.675 94.59
Patient 4 20 Kit A 2.27 1.86 95.72
Patient 4 50 Kit A not detectable 3.385 87.13
Patient 4 80 Kit A 2.33 1.905 95.64
Patient 5 20 Kit A 1.6 1.51 82.87
Patient 5 50 Kit A 1.79 1.525 91.76
Patient 5 80 Kit A 3.47 2.765 not detectable
Patient 1 20 Kit B 1.88 not detectable 80.23
Patient 1 50 Kit B 0.73 1.43 75.72
Patient 1 80 Kit B 1.44 1.585 75.64
Patient 2 20 Kit B 2.63 1.45 79.75
Patient 2 50 Kit B 1.92 1.765 87.14
Patient 2 80 Kit B 1.56 1.52 91.01
Patient 3 20 Kit B not detectable 1.335 78.00
Patient 3 50 Kit B 2.28 1.63 83.21
Patient 3 80 Kit B 2 1.67 78.61
Patient 4 20 Kit B 0.59 0.625 94.37
Patient 4 50 Kit B 2.29 1.78 92.97
Patient 4 80 Kit B not detectable not detectable not detectable
Patient 5 20 Kit B 2.63 1.41 83.15
Patient 5 50 Kit B not detectable 1.005 92.06
Patient 5 80 Kit B 2.21 1.69 94.51
Patient 1 20 Kit C 1.69 1.495 90.73
Patient 1 50 Kit C 1.72 1.555 94.43
Patient 1 80 Kit C 1.72 1.565 88.71
Patient 2 20 Kit C 1.64 1.4 92.75
Patient 2 50 Kit C 1.63 1.455 93.26
Patient 2 80 Kit C 1.72 1.51 94.34
Patient 3 20 Kit C 1.63 1.4 91.78
Patient 3 50 Kit C 1.7 1.505 93.61
Patient 3 80 Kit C 1.74 1.595 94.61
Patient 4 20 Kit C 1.62 1.36 92.89
Patient 4 50 Kit C 1.71 1.495 94.2
Patient 4 80 Kit C 1.76 1.575 95.17
Patient 5 20 Kit C 1.57 1.36 80.55
Patient 5 50 Kit C 1.66 1.455 92.65
Patient 5 80 Ki t C 1.69 1.45 90.29

Table 2: Results of qualitative analysis. A260/280 ratios calculated with micro-spectrometer as well as microplate-reader are shown for every sample (n = 15) and the three different extraction methods. DV200 (fragments bigger than 200 bp) calculated via fragmentation analysis is also shown for kits A, B, and C.

Sample µm Kit Fragments % <200bp Fragments % 200-1500 bp Fragments % >1500bp Fragments max peak (bp)
Patient 1 20 Kit A 9.04 77.08 13.64 484
Patient 1 50 Kit A 10.14 77.03 12.97 378
Patient 1 80 Kit A 10.91 76.56 12.42 393
Patient 2 20 Kit A 11.01 67.04 20.1 589
Patient 2 50 Kit A 6.09 68.67 23.79 628
Patient 2 80 Kit A 11.54 66.07 18.71 560
Patient 3 20 Kit A 10.22 77.29 11.95 412
Patient 3 50 Kit A 8.52 76.93 13.93 465
Patient 3 80 Kit A 4.79 77.5 17.09 580
Patient 4 20 Kit A 2.7 55.77 39.95 1331
Patient 4 50 Kit A 7.6 54.3 32.83 1183
Patient 4 80 Kit A 2.5 61.06 34.58 1185
Patient 5 20 Kit A 12.32 36.52 46.35 1895
Patient 5 50 Kit A 5.34 36.37 55.39 1856
Patient 5 80 Kit A not detectable not detectable not detectable not detectable
Patient 1 20 Kit B 18.51 69.28 10.95 283
Patient 1 50 Kit B 23.58 65.24 10.48 254
Patient 1 80 Kit B 22.42 67.14 8.5 257
Patient 2 20 Kit B 16.21 59.88 19.87 523
Patient 2 50 Kit B 9.39 63.7 23.44 678
Patient 2 80 Kit B 7.45 67.62 23.39 666
Patient 3 20 Kit B 18.53 65.15 12.85 370
Patient 3 50 Kit B 15.96 72.12 11.09 316
Patient 3 80 Kit B 20.7 71.49 7.12 266
Patient 4 20 Kit B 3.09 57.44 36.93 1296
Patient 4 50 Kit B 3.69 52.2 40.77 1373
Patient 4 80 Kit B not detectable not detectable not detectable not detectable
Patient 5 20 Kit B 9.86 34.96 48.19 1831
Patient 5 50 Kit B 3.76 31.42 60.64 2002
Patient 5 80 Kit B 1.93 33.24 61.27 2015
Patient 1 20 Kit C 8.88 81.47 9.26 358
Patient 1 50 Kit C 5.92 83.95 10.48 374
Patient 1 80 Kit C 11.02 80.18 8.53 334
Patient 2 20 Kit C 5.18 74.75 18 492
Patient 2 50 Kit C 4.96 75.67 17.59 458
Patient 2 80 Kit C 3.14 72.46 21.88 441
Patient 3 20 Kit C 7.15 79.05 12.73 393
Patient 3 50 Kit C 5.85 78.02 15.59 365
Patient 3 80 Kit C 2.59 68.54 26.07 458
Patient 4 20 Kit C 3.94 54.49 38.4 1433
Patient 4 50 Kit C 1.42 45.24 48.96 1634
Patient 4 80 Kit C 0.76 37.03 58.14 1849
Patient 5 20 Kit C 13.02 40.78 39.77 not detectable
Patient 5 50 Kit C 2.72 39.08 53.57 1813
Patient 5 80 Ki t C 5.25 31.87 58.42 2024

Table 3: Results of fragmentation analysis. Here, the percentage of the fragments smaller than 200 bp, bigger than 1,500 bp and between 200 bp and 1,500 bp is shown for all five patients, the different amounts of starting material (20 µm, 50 µm, and 80 µm) and the three different isolation methods. Percentages smaller than 2% were named as not detectable.

Subscription Required. Please recommend JoVE to your librarian.

Discussion

DNA extraction methods for FFPE tissue vary in quality and quantity of isolated DNA, which inevitably affects the performance of further downstream analyses. Thus, automation is becoming imperative to improve workflow and standardization, as well as quality management. Therefore, in the present study, a semi-automated method for DNA extraction from FFPE samples was evaluated demonstrating better results than the other tested manual column-based protocols.

To optimize the described semi-automated method, our aim was to have one general protocol for every kind of tissue and body liquid, as well as fixed specimen. Hence, we used the commercially available DNA Blood kit from the company (Table of Materials) for optimization. First of all, we included an incubation step for deparaffinization, using the commercially available incubation buffer and 1-thioglycerol of the same manufacturer. In different tests regarding the incubation time and optimum melting temperature of the paraffin, we chose a 10 min incubation step at 80 °C as intended in other commercially available FFPE kits. Concerning the amount of FFPE slices, most companies recommend 2 µm x 10 µm slices for DNA extraction. As known in this magnitude, it is extremely difficult to isolate DNA from specimen containing little cell amount. Hence, we tried different amounts of fixed tissue slices and found that using 50 µm of tissue in total (best in single sections of 5 µm–10 µm) showed the best results. This is at any rate suitable for tissue with low cell amounts, but tissue with higher amounts of cells can also be treated like this. Especially column-based systems here show a high limitation with clogging of the silica membrane. The Proteinase K digestion was suggested to last between 4–20 h. Here, we found out that an incubation time of 4–6 h is indeed fine, but overnight incubation leads to more sufficient quality and quantity of DNA. For better cell lysis, it also appeared helpful to add another 10 µL of Proteinase K on the next day and incubate again for 1 h. As a shaking/mixing speed we chose more than the suggested 300 rpm since we saw that stronger mixing (500 rpm–600 rpm) leads to better proteinase K digestion, and therefore, higher amounts of DNA. Also, additional mixing steps (such as vortexing or full speed shaking) during the incubation leads to better DNA extraction. Contrary to the original FFPE protocol, we chose further incubation time after the addition of lysis buffer to the sample, with the lysis being more sufficient at 65°C. The last optimization step of the protocol was the addition of another incubation buffer. The system requires at least 60 µL of elution buffer. With the automated system being known to loose 5 µL –10 µL, we choose to have an elution volume of 65 µL.

This protocol has some crucial steps to note. The first one is to set the right temperature to solubilize the paraffin. 80 °C seems to be the best temperature for optimal melting. It is also crucial to cool the sample to 60 °C before adding proteinase K to prevent this enzyme from degradation. Next, it is important to not vortex the sample again after the 30 min incubation time with lysis buffer since the paraffin has to harden on top. Otherwise, the sample will be contaminated with paraffin. As a last step, it is also important to add some extra elution buffer volume since the system loses 5 µL–10 µL. We think that 65 µL of elution buffer is a good amount. If higher amounts of DNA are expected, the volume can of course be increased.

The optimized semi-automated isolation method provided the highest concentrations of total genomic DNA in all FFPE samples. Using the same amount of elution volume, also the total yield of DNA was four times higher. Additionally, the column-based kits showed no increase in DNA yield using thicker tissue sections, whereas the automate system demonstrated a linear increase of the DNA concentration associated with the augmented amount of tissue used. These differences can be explained mainly due to the paraffin clogging in the columns and the consequent lowering of the DNA binding capacity. Our data also suggests that larger amount of FFPE tissue, in our case 80 µm sections, are not necessary when isolating DNA with the semi-automated system. We could show that already a smaller amount (20 µm sections) leads to a sufficient yield of DNA. Thus, valuable tissue material can be saved. Moreover, DNA extracted with the semi-automated protocol, fulfilled, in most cases, the required purity criterion for high quality DNA (A260/280 ratio between 1.6 and 1.8). In contrast, DNA obtained from column-based isolation systems showed wide variation in a DNA purity and fewer samples fit the mentioned optimum ratio.

Sarnecka et al. described recently that a magnetic particle-based system is more sufficient than column-based systems12. Khokhar and colleagues could demonstrate that the automated system based on another protocols is more sufficient for smaller amplicons and widely robust in terms of quantity and purity of the extracts compared with other methods36. Our samples confirmed these findings showing a high distribution in the A260/280 ratio of the DNA isolated by the other kits.

Regarding the fragmentation analysis, eight DNA extracts obtained from these three commercial methods were used for PCR amplification. Different fragment lengths of one housekeeping gene (beta actin) were amplified and visualized using gel electrophoresis. There was only mild variation between the individual samples that may be attributed to the fact that all tissues have similar stage of atherosclerosis. This assumption was confirmed by histology (data not shown). Furthermore, this data shows that all samples were treated with formalin in the same standard manner. No significant differences were observed with regards to the fragment length obtained from the different samples independent of the method used for DNA extraction. Hence, fragmentation of FFPE tissue does not depend on the method used for DNA isolation but is rather affected by the variability of the human specimens and formalin treatment.

Since the used semi-automated system is described as a magnetic particle mover, not a liquid handler, it also offers some advantages over other semi-automated systems. The main advantage is the minimal risk of cross-contamination, since no liquid handling or splashing happens during sample processing. Another point we want to mention is the high amount of samples, which can be processed in one run of the system, without having much more hands-on time. Using a semi-automated system also leads to a lower probability of user mistakes than with the column-based or phase-separation methods. Especially for biobanking analyses and diagnostic work as well as for handling difficult tissues the semi-automated method described above is highly recommended. In these areas, it is very important that different workers and sometimes even unexperienced people all come to fast, easy, and reproducible results. Other advantages of the system are the generally applicable protocol, which can be used for every kind of tissue as well as blood, other body liquids, and also cells with only one minor change in the first step of the protocol, where no incubation buffer is needed.

Even if our results clearly demonstrated the superiority of the automated system for DNA extraction from FFPE over the manual protocols, it is to mention that we have compared only three commercially available kits. Consequently, our conclusion concerns only the methods tested in our study. In addition, the number of samples was low, and we used only atherosclerotic plaques for comparison. In order to generalize the results of our study, other tissue samples in a greater number would be necessary.

Nevertheless, the automated system seems to have considerable advantage over the manual kits, particularly for specimens with low amount of expected nucleic acids. Also, the system itself has certain limitations. For example, as mentioned above, it is necessary to use in minimum 60 µl for elution, because the plunger needs this amount to elute the DNA. Also, the loss of elution volume is higher for the semi-automated system than for the column-based systems. The automated method has a loss of around 10 µl of elution volume, whereas the manual methods only have a loss of 5 µl. Also, the higher costs have to be mentioned. But for high throughput analyses, the semi-automated system still offers the best benefits compared to costs. As a last limitation of the system, it is important to note that automated and semi-automated extraction is a self-contained closed system. It is, of course, possible to isolate, for example, DNA and protein, or also RNA and DNA from one sample, but it is not that easy and often used with manual phase separation methods. All buffers are customized to the kit and are not usable for other methods in contrast to Trizol reagents. At the end, it is also important to mention that, in general, DNA from FFPE samples is not suitable for whole genome sequencing because the fragmentation of the nucleic acids is too strong.

In conclusion, in this study, we demonstrate that a fully automated DNA isolation method might be an excellent tool to reduce the hands-on time and the amount of starting material. Also, it seems to be the best choice to reduce the contamination risks between samples. In addition, the flexibility of the automated system allows processing of not only one but up to 48 samples per run, which makes this method a useful tool for future high throughput analyses of samples with low number of cells and thus minor amount of nucleic acids. The quality and quantity of the isolated DNA using the automated system appears superior over other manual kits and also usage in further analyses as Southern blot, single nucleotide genotyping, cloning analyses, methylation assays as well as PCR amplification is possible.

Subscription Required. Please recommend JoVE to your librarian.

Disclosures

The authors declare that there is no conflict of interest.

Acknowledgments

The establishment of the protocol for automated DNA extraction was supported by Dr. Paul Muschler from the Promega company. We thank Paul Muschler for his support and scientific contribution. We also thank our colleague Dr. Moritz von Scheidt (German Heart Center Munich) for providing us with the Maxwell instrument and for supporting the experimental part. All experiments were performed in the laboratories of German Heart Centre (Munich, Germany) and Klinikum rechts der Isar (Munich, Germany). The research was funded by DFG (PE 900/6-1).

Materials

Name Company Catalog Number Comments
1.5 ml tubes for sample incubation Eppendorf, Hamburg, Germany 30120086
1-Thioglycerol Promega, Walldorf, Germany A208
Agilent tape station software 3.2 Agilent, Waldbronn, Germany
dsDNA HS Kit ThermoFisher Scientific, Schwerte, Germany Q32851
FFPE DNA Purification Kits (Kit A) Norgene Biotek, Heidelberg, Germany 47400
FFPE tissue samples n=5 Munich Vascular Biobank,Munich, Germany
GeneRead DNA FFPE Kit (Kit B) Qiagen, Hilden, Germany 180134
Heating blocks, set to 80°C and 65°C VWR,Darmstadt,Germany 460-0250
High Sensitivity D5000 reagents Agilent, Waldbronn, Germany 5067-5593
High Sensitivity D5000 ScreenTape Agilent, Waldbronn, Germany 5067-5592
Incubation Buffer Promega, Walldorf, Germany D920
Maxwell Blood Kit RSC including: Lysis Buffer, Elution Buffer, Proteinase K Promega, Walldorf, Germany AS1400
Maxwell RSC 48 Instrument Promega, Walldorf, Germany AS8500
Microcentrifuge Eppendorf, Hamburg, Germany
NanoDrop 2000c Spectrometer ThermoFisher Scientific, Schwerte, Germany ND-2000C
Optical caps Agilent, Waldbronn, Germany 401425
Optical tube strips Agilent, Waldbronn, Germany 401428
Pipettors and pipette tips Eppendorf, Hamburg, Germany
Prism 6 for statistics, version 6.01 GraphPad Inc., San Diego, California
Qubit 3.0 Fluorometer ThermoFisher Scientific, Schwerte, Germany Q33216
TapeStation 4200 Agilent, Waldbronn, Germany
Tecan Infinite M200 Pro Tecan, Männedorf, Swizerland IN-MNANO

DOWNLOAD MATERIALS LIST

References

  1. Pelisek, J., et al. Biobanking: objectives, requirements, and future challenges-experiences from the munich vascular biobank. Journal of Clinical Medicine. 8, (2), 251 (2019).
  2. Goelz, S. E., Hamilton, S. R., Vogelstein, B. Purification of DNA from formaldehyde fixed and paraffin embedded human tissue. Biochemical and Biophysical Research Communications. 130, (1), 118-126 (1985).
  3. Busch, A., Eken, S. M., Maegdefessel, L. Prospective and therapeutic screening value of non-coding RNA as biomarkers in cardiovascular disease. Annals of Translational Medicine. 4, (12), (2016).
  4. Kandpal, R. P., Saviola, B., Felton, J. The era of 'omics unlimited. BioTechniques. 46, (5), 351-355 (2009).
  5. McDonough, S. J., et al. Use of FFPE-derived DNA in next generation sequencing: DNA extraction methods. PloS One. 14, (4), (2019).
  6. Gilbert, M. T. P., et al. The isolation of nucleic acids from fixed, paraffin-embedded tissues-which methods are useful when. PloS One. 2, (6), (2007).
  7. Williams, C., et al. A high frequency of sequence alterations is due to formalin fixation of archival specimens. The American Journal of Pathology. 155, (5), 1467-1471 (1999).
  8. Solomon, M. J., Varshavsky, A. Formaldehyde-mediated DNA-protein crosslinking: a probe for in vivo chromatin structures. Proceedings of the National Academy of Sciences. 82, (19), 6470-6474 (1985).
  9. Gillio-Tos, A., et al. Efficient DNA extraction from 25-year-old paraffin-embedded tissues: study of 365 samples. Pathology. 39, (3), 345-348 (2007).
  10. Srinivasan, M., Sedmak, D., Jewell, S. Effect of fixatives and tissue processing on the content and integrity of nucleic acids. The American Journal of Pathology. 161, (6), 1961-1971 (2002).
  11. van Eijk, R., Stevens, L., Morreau, H., van Wezel, T. Assessment of a fully automated high-throughput DNA extraction method from formalin-fixed, paraffin-embedded tissue for KRAS, and BRAF somatic mutation analysis. Experimental and Molecular Pathology. 94, (1), 121-125 (2013).
  12. Sarnecka, A. K., et al. DNA extraction from FFPE tissue samples–a comparison of three procedures. Contemporary Oncology. 23, (1), 52 (2019).
  13. Kalmár, A., et al. Comparison of automated and manual DNA isolation methods for DNA methylation analysis of biopsy, fresh frozen, and formalin-fixed, paraffin-embedded colorectal cancer samples. Journal of Laboratory Automation. 20, (6), 642-651 (2015).
  14. McCormick, S. F. Multilevel adaptive methods for partial differential equations. (SIAM). (1989).
  15. Sambrook, J., Russell, D. W. Purification of nucleic acids by extraction with phenol: chloroform. Cold Spring Harbor Protocols. 2006, (1), 4455 (2006).
  16. Berensmeier, S. Magnetic particles for the separation and purification of nucleic acids. Applied Microbiology and Biotechnology. 73, (3), 495-504 (2006).
  17. Petrigh, R. S., Fugassa, M. H. DNA extraction and a cost-effective detection method for Echinococcus granulosus protoscoleces. Veterinary Parasitology. 198, (3-4), 410-413 (2013).
  18. Lee, J. H., Park, Y., Choi, J. R., Lee, E. K., Kim, H. S. Comparisons of three automated systems for genomic DNA extraction in a clinical diagnostic laboratory. Yonsei Medical Journal. 51, (1), 104-110 (2010).
  19. Rohland, N., Siedel, H., Hofreiter, M. A rapid column-based ancient DNA extraction method for increased sample throughput. Molecular Ecology Resources. 10, (4), 677-683 (2010).
  20. Gutiérrez-López, R., Martínez-de la Puente, J., Gangoso, L., Soriguer, R. C., Figuerola, J. Comparison of manual and semi-automatic DNA extraction protocols for the barcoding characterization of hematophagous louse flies (Diptera: Hippoboscidae). Journal of Vector Ecology: Journal of the Society for Vector Ecology. 40, (1), 11-15 (2015).
  21. Seiler, C., et al. Nucleic acid extraction from formalin-fixed paraffin-embedded cancer cell line samples: a trade off between quantity and quality. BMC Clinical Pathology. 16, (1), 17 (2016).
  22. Harada, S. Sample Preparation Techniques for Soil, Plant, and Animal Samples. Springer. 125-138 (2016).
  23. Haile, S., et al. Automated high throughput nucleic acid purification from formalin-fixed paraffin-embedded tissue samples for next generation sequence analysis. PloS One. 12, (6), 0178706 (2017).
  24. Fujii, T., et al. Evaluation of DNA and RNA quality from archival formalin-fixed paraffin-embedded tissue for next-generation sequencing-Retrospective study in Japanese single institution. Pathology International. (2020).
  25. Ludyga, N., et al. Nucleic acids from long-term preserved FFPE tissues are suitable for downstream analyses. Virchows Archiv: An International Journal of Pathology. 460, (2), 131-140 (2012).
  26. Niland, E. E., McGuire, A., Cox, M. H., Sandusky, G. E. High quality DNA obtained with an automated DNA extraction method with 70+ year old formalin-fixed celloidin-embedded (FFCE) blocks from the indiana medical history museum. American Journal of Translational Research. 4, (2), 198 (2012).
  27. Riemann, K., et al. Comparison of manual and automated nucleic acid extraction from whole-blood samples. Journal of Clinical Laboratory Analysis. 21, (4), 244-248 (2007).
  28. Steinau, M., Patel, S. S., Unger, E. R. Efficient DNA extraction for HPV genotyping in formalin-fixed, paraffin-embedded tissues. The Journal of Molecular Diagnostics. 13, (4), 377-381 (2011).
  29. Dundas, N., Leos, N. K., Mitui, M., Revell, P., Rogers, B. B. Comparison of automated nucleic acid extraction methods with manual extraction. The Journal of Molecular Diagnostics. 10, (4), 311-316 (2008).
  30. Okello, J. B., et al. Comparison of methods in the recovery of nucleic acids from archival formalin-fixed paraffin-embedded autopsy tissues. Analytical Biochemistry. 400, (1), 110-117 (2010).
  31. Witt, S., Neumann, J., Zierdt, H., Gébel, G., Röscheisen, C. Establishing a novel automated magnetic bead-based method for the extraction of DNA from a variety of forensic samples. Forensic Science International: Genetics. 6, (5), 539-547 (2012).
  32. Ivanova, N. V., Fazekas, A. J., Hebert, P. D. Semi-automated, membrane-based protocol for DNA isolation from plants. Plant Molecular Biology Reporter. 26, (3), 186 (2008).
  33. Sengüven, B., Baris, E., Oygur, T., Berktas, M. Comparison of methods for the extraction of DNA from formalin-fixed, paraffin-embedded archival tissues. International Journal of Medical Sciences. 11, (5), 494 (2014).
  34. Miller, S. A., Dykes, D. D., Polesky, H. F. A simple salting out procedure for extracting DNA from human nucleated cells. Nucleic Acids Research. 16, (3), 1215 (1988).
  35. Wilfinger, W. W., Mackey, K., Chomczynski, P. Effect of pH and ionic strength on the spectrophotometric assessment of nucleic acid purity. BioTechniques. 22, (3), 474-481 (1997).
  36. Khokhar, S. K., Mitui, M., Leos, N. K., Rogers, B. B., Park, J. Y. Evaluation of Maxwell 16 for automated DNA extraction from whole blood and formalin-fixed paraffin embedded (FFPE) tissue. Clinical Chemistry and Laboratory Medicine (CCLM). 50, (2), 267-272 (2012).
This article has been published
Video Coming Soon
PDF DOI DOWNLOAD MATERIALS LIST

Cite this Article

Bauer, S., Pauli, J., Pelisek, J. Optimized High Quality DNA Extraction from Formalin-Fixed Paraffin-Embedded Human Atherosclerotic Lesions. J. Vis. Exp. (168), e61452, doi:10.3791/61452 (2021).More

Bauer, S., Pauli, J., Pelisek, J. Optimized High Quality DNA Extraction from Formalin-Fixed Paraffin-Embedded Human Atherosclerotic Lesions. J. Vis. Exp. (168), e61452, doi:10.3791/61452 (2021).

Less
Copy Citation Download Citation Reprints and Permissions
View Video

Get cutting-edge science videos from JoVE sent straight to your inbox every month.

Waiting X
simple hit counter