In this study, we describe the process of T lymphocyte isolation from fresh samples of calcified aortic valves and the analytical steps of T cell-cloning for the characterization of the adaptive leukocyte subsets by using flow cytometry analysis.
Calcific aortic valve disease (CAVD), an active disease process ranging from mild thickening of the valve to severe calcification, is associated with high mortality, despite new therapeutic options such as transcatheter aortic valve replacement (TAVR).
The complete pathways that start with valve calcification and lead to severe aortic stenosis remain only partly understood. By providing a close representation of the aortic valve cells in vivo, the assaying of T lymphocytes from stenotic valve tissue could be an efficient way to clarify their role in the development of calcification. After surgical excision, the fresh aortic valve sample is dissected in small pieces and the T lymphocytes are cultured, cloned then analyzed using fluorescence activated cell sorting (FACS).
The staining procedure is simple and the stained tubes can also be fixed using 0.5% of paraformaldehyde and analyzed up to 15 days later. The results generated from the staining panel can be used to track changes in T cell concentrations over time in relation to intervention and could easily be further developed to assess activation states of specific T cell subtypes of interest. In this study, we show the isolation of T cells, performed on fresh calcified aortic valve samples and the steps of analyzing T cell clones using flow cytometry to further understand the role of adaptive immunity in CAVD pathophysiology.
Calcific aortic valve disease (CAVD) is one of the most common heart valve disorders, with a heavy impact on healthcare. The frequency of aortic valve replacement in the last years has increased dramatically and is expected to increase further, due to the growing elderly population1.
The underlying pathophysiology of CAVD is only partially known and the current therapeutic strategies are limited to conservative measures or aortic valve replacement, either through surgical or percutaneous procedures. To date, no effective medical treatment can hinder or reverse CAVD progression and high mortality is associated with early symptom-onset, unless aortic valve replacement (AVR) is performed2. In patients with severe symptomatic aortic stenosis, the 3-year symptom-free survival was reported as low as 20%3. Transcatheter aortic valve replacement (TAVR) represents a new option, revolutionizing treatment for high-risk patients, especially among the elderly and has dramatically reduced the mortality, which was intrinsically high in this population4,5,6. Despite the promising results of TAVR, further research is necessary to understand CAVD pathophysiology to identify novel early therapeutic targets7,8,9.
Previously thought to be a passive, degenerative process, CAVD is now recognized as an active progressive disease, characterized by an osteoblastic phenotype switch of the aortic valve interstitial cells10. This disease involves progressive mineralization, fibrocalcific changes and reduced motility of the aortic valve leaflets (sclerosis), which ultimately obstruct blood flow leading to narrowing (stenosis) of the aortic valve opening11.
Inflammation is considered a key process in CAVD pathophysiology, similar to the process of vascular atherosclerosis. Endothelial injury enables the deposition and accumulation of lipid species, especially oxidized lipoproteins in the aortic valve12. These oxidized lipoproteins provoke an inflammatory response, as they are cytotoxic, with the inflammatory activity leading to mineralization. The role of innate and adaptive immunity in CAVD development and disease progression has been recently highlighted13. The activation and clonal expansion of specific subsets of memory T cells have been documented in patients with CAVD and mineralized aortic valve leaflets, so that inflammatory processes are assumed to be involved at least in the development of CAVD and presumably in disease progression as well14. In fact, although antigen-presenting cells and macrophages are present in both the healthy and diseased valve, the presence of T lymphocytes is indicative of an aged and diseased aortic valve. This lymphocytic infiltrate along with an increase in neovascularization and metaplasia are characteristic histological signs of CAVD15.
We hypothesize the existence of an interaction between the aortic valve interstitial cells and the activation of the immune system, which potentially triggers the initiation of a chronic inflammatory process in the aortic valve. The assaying of T cells from stenotic aortic valve tissue could be an efficient way to clarify their role in calcification development, as it can provide a close representation of the aortic valve cells in vivo. In the present work, using aortic valve tissue, we isolate T-lymphocytes, culture and clone them, and subsequently characterize them using fluorescence-activated cell sorting (FACS). Fresh aortic valve samples were excised from CAVD patients who received surgical valve replacement for severe aortic stenosis. After the surgical excision, the fresh valve sample was dissected in small pieces and the T cells were cultured, cloned then analyzed using flow cytometry. The staining procedure is simple and the stained tubes can be fixed using 0.5% of paraformaldehyde and analyzed up to 15 days later. The data generated from the staining panel can be used to track changes in T lymphocyte distribution over time in relation to intervention and could easily be further developed to assess activation states of specific T cell subsets of interest.
The extraction of calcified tissue, the isolation of leukocytes from calcified tissue and particularly the use of flow cytometry on this type of tissue can be challenging, due to issues such as autofluorescence. Few publications exist with protocols for this specific purpose16,17,18. Herein we present a protocol designed specifically for the direct isolation and culture of T lymphocyte from human aortic valve samples. Clonal expansion of lymphocytes is a hallmark of adaptive immunity. Studying this process in vitro provides insightful information on the level of lymphocyte heterogeneity19. After a three-week incubation period, the T cell clones are ready to be explanted, as an adequate amount of T cells from each clone was obtained, so as to allow the phenotypic and functional study. Subsequently the phenotype of T clones is studied by cytofluorometry.
This immunological protocol is an adaptation of a method previously developed by Amedei et al. for T cell isolation and characterization from human tissue, especially designed for calcified human tissue, such as in CAVD20,21,22. The protocol here for the isolation of PBMCs (peripheral blood mononuclear cells) using irradiated buffy coat describes an effective way to obtain feeder cells (FC), specifically adjusted for the cloning phase of T lymphocytes isolated from valve interstitial cells. The feeder layer consists of in growth arrested cells, which are still viable and bioactive. The role of feeder cells is important to support in vitro survival and growth of T lymphocytes isolated from valve interstitial cells23. In order to avoid feeder cell proliferation in culture, these cells must undergo a growth arrest. This can be achieved in two ways: through physical methods such as irradiation, or through treatment with cytotoxic chemicals, such as mitomycin C (MMC), an antitumoral antibiotic that can be applied directly to the culture surface24. Here we show feeder cell growth arrest achieved through cell irradiation.
This method presents an efficient, cost-effective way to isolate and characterize T cells from aortic valve tissue, contributing to broadening the spectrum of immunological methods for exploring CAVD pathophysiology.
The study was conducted according to the Statute of the Charité for Ensuring Good Scientific Practice and the legal guidelines and provisions on privacy and ethics were respected. The Ethics Committee approved all human experiments and the privacy and anonymity of the patients were maintained in accordance with the rules reported on the Ethic Form.
NOTE: For the protocol described below fresh human stenotic valve samples were used.
1. Reagent preparation
2. Human T lymphocyte isolation and culture into T-25 flasks
3. Cloning phase
NOTE: For the cloning phase of T cells, it is necessary to start with the isolation of feeder cells from an irradiated buffy coat (BC), following the PBMCs protocol.
4. T Lymphocytes culture in multiwell plates
5. First refeeding phase
6. Second refeeding phase
7. First splitting phase from 1 well/sample to 2 wells/sample
8. Second splitting phase from 2 wells/sample to 4 wells/sample
9. Third splitting phase from 4 wells/sample to 8 wells/sample:
10. Cytofluorimetric analysis
11. Antibody Staining Panel Preparation for cytofluorimetric analysis
Marker | Fluorophore |
CD3 | PE/Cy7 |
CD4 | Alexa Fluor 488 |
CD8 | Brilliant violet 510 |
CD14 | Brilliant violet 421 |
CD25 | PE |
CD45 | Brilliant violet 711 |
Table 1. Antibody staining panel to detect the T lymphocytes population in calcification aortic valve disease.
We used a simple and cost-effective method to characterize the leukocyte population of fresh aortic valve samples derived from human patients with severe aortic valve stenosis (refer to protocol). The method for isolating PBMCs is a vital step in obtaining feeder cells, which are used in every step of the experiment (cloning, refeeding and splitting phases) and enable the detection and characterization of infiltrating leukocytes in aortic valve samples. The key steps of this method are shown in Figure 1.
Figure 1. FCs isolation from buffy coat. (A) Blood layered over density gradient medium (B) White blood cells ring obtained after centrifugation (C) White blood cells collected and resuspended in PBS solution (D) White cells observed under light microscopy Please click here to view a larger version of this figure.
After two weeks of incubation, we successfully cloned and grew a T cell population, as shown in Figure 2.
Figure 2. T cell clone after two weeks of incubation observed using light microscopy. Please click here to view a larger version of this figure.
Figure 3 illustrates the gating scheme utilized for the analysis of T cell subpopulations in patients with CAVD. As shown from the result of the FACS analysis, there are more CD4+ T-cells (43.032%) than CD8+ T-cells (1.079%).
Figure 3. Gating scheme utilized for T cell-subpopulation analysis. (A) A gate has been applied to identify the specific T cell population in a stenotic valve. (B) CD14 negative lymphocytes and CD3 positive lymphocytes. (C) CD3 lymphocytes are gated to distinguish CD4+ T cells from CD8+ T cells. Please click here to view a larger version of this figure.
To show that the same T cell markers are present in both native valve samples and cloned samples, we performed FACS analysis without the cloning phase, as illustrated in Figure 4.
Figure 4. FACS analysis results of two valve samples. We compared the T cells obtained from a native valve sample and a cloned sample, validating that the T cells found in the native valve share specific markers of the T cells in the final cloned product. (A) FACS results of a native valve sample, without the cloning phase. (B) FACS results of the valve sample analysed after the cloning phase. Please click here to view a larger version of this figure.
The entire workflow is summarized in Figure 5, starting from the dissection of the human aortic valve and leading up to the FACS analysis. All steps are required for the analysis of one aortic valve sample. Phase 1 shows the lymphocyte isolation from stenotic aortic valve tissue. The valve samples need to be cut and placed in a Petri dish filled with wash buffer. The valve pieces can be placed inside a T25 flask filled with CCM and stored in a CO2 incubator for one week. Phase 2 shows the Cloning phase, which consists of two parts: 1) FCs isolation from irradiated buffy coat bag and 2) T cells cloning phase and culminates with the cell culture in a 96-wells multiwell plate, which is stored in a CO2 incubator for one week. Phases 3 and 4 consist of the refeeding phase using FCs from irradiated buffy coat; this phase must be repeated for two consecutive weeks. Phases 4, 5 and 6 show the splitting phase of T cell clones; the first splitting phase is from 1 well/sample to two wells for each sample in a new multiwell plate; the second splitting is from 2 wells /sample to 4 wells for each in the same multiwell plate; the third and last splitting phase is from 4 wells/sample to 8 in a new multiwell plate. Phase 7 is the final phase, where the samples are analyzed using FACS analysis.
Figure 5. CAVD Experimental workflow. Please click here to view a larger version of this figure.
From the preliminary results (Figure 2) we can conclude that lymphocytes, along with CD45+ leukocytes are present in calcified aortic valves, thus indicating that calcific aortic valve disease is linked with activation of the immune system and inflammatory activity.
Here we present a method to characterize T lymphocyte subpopulations isolated from stenotic aortic valve samples, using flow cytometry. This method requires the use of irradiated buffy coat to isolate the PBMCs. The radiation frequency to which the buffy coat bags must be subjected is 9000 Rad/90 Gray (Gy) and it represents a crucial step to halt the proliferation of the feeder cells. The role of the cells isolated from the buffy coat bags is to act only as feeder cells and provide nutrients for the T cells isolated from the valves. The use of an unirradiaded buffy coat bag would promote proliferation of PBMCs in culture, as has been noted in the past25. A radiation frequency below 90 Gy showed PBMCs proliferation in culture, so we recommend using exactly 90 Gy of radiation. Of note, it is advisable to use the buffy coat irradiated on the same day or at most the next day, keeping it on a device that keeps it in constant agitation. Another crucial step of this method could be represented by the lymphocyte cloning phase, which could be affected by artifacts; to avoid this event we perform the FACS on fresh aortic valve samples. The cloning phase of T lymphocytes has the advantage of obtaining a larger number of T clones (an average of 15 T cells clones for each valve) to be analyzed phenotypically and functionally, than the number obtained from the analysis of one fresh sample. The cloning technique has been used by this research group for many years and depending on the type of tissue analyzed, the lymphocyte profile was different21,26,27. The first passage of the method concerns the T cell isolation from a stenotic aortic valve. All the steps described must be performed under a laminar flow hood in sterile conditions and it is strongly recommended to disinfect all materials before use. The time required to obtain results was 6 weeks and the average of T lymphocyte cells obtained from the cloning phase was 20 x 106 cells. The monitoring phase of the multiwell plates is very important and must not be overlooked. A change in the color of the medium to yellow could represent bacterial contamination, in which case all the instruments used need to be sterilized and the multiwell plates thrown away.
Before FACS analysis it is important to establish a suitable gate, to verify that there is no specific overlap between the antibody channels. This enables the optimal separation between positive and negative gates. The use of the same lots of antibodies for all samples involved in the study is recommended to obtain homogeneous result. It is also necessary to protect the fluorophore-conjugated antibodies from light, performing all steps with the light off.
This method is effective in yielding results with high reproducibility and is not expensive. A limitation of this method is the small sample size, due to the limited availability of the human valve samples, as well as the lack of a control group.
The preliminary results support the role of adaptive immunity as a crucial element in the development and progression of calcific aortic valve disease. All the patients enrolled in this study had a diagnosis of severe symptomatic calcific aortic stenosis, with an average age of 70, mostly male. The existence of T cell populations in the aortic valves analyzed provides evidence for the inflammatory activity of the diseased aortic valve as a checkpoint of immune cell activation. A point of future interest could be to analyze the functionality of CAVD-infiltrating T cells and characterize T cell specificity as previously reported in similar diseases, such as in atherosclerosis28,29,30.
The authors have nothing to disclose.
All the buffy coat bags used for this protocol were irradiated thanks to availability of Dr. Peter Rosenthal, Dr. Dirk Böhmer and the whole team of the Radiology Department of Charité Benjamin Franklin. Scholarship Holder/Mary Roxana Christopher, this work is supported by a scholarship from the German Cardiac Society (DGK).
50 mL plastic syringes | Fisherbrand | 9000701 | |
96- well U- bottom Multiwell plates | Greiner Bio-One | 10638441 | |
Bag Spike (needle free) | Sigma | P6148 | Dilute to 4% with PBS |
CD14 Brilliant violet 421 | Biolegend | 560349 | |
CD25 PE | Biolegend | 302621 | |
CD3 PE/Cy7 | Biolegend | 300316 | |
CD4 Alexa Fluor 488 | Biolegend | 317419 | |
CD45 Brilliant violet 711 | Biolegend | 304137 | |
CD8 Brilliant violet 510 | Biolegend | 301047 | |
Eppendorf tube 1.5 mL | Eppendorf | 13094697 | |
Eppendorf tube 0.5 mL | Thermo Scientific | AB0533 | |
Falcon 15 mL conical centrifuge tube | Falcon | 10136120 | |
Falcon 50 mL conical centrifuge tubes | Falcon | 10788561 | |
Falcon Round-Bottom Polystyrene Tubes | BD | 2300E | |
Fast read 102 plastic counting chamber | KOVA INTERNATIONAL | 630-1893 | |
Filters for culture medium 250 mL | NalgeneThermo Fisher Scientific | 168-0045 | |
Filters for culture medium 500 mL | NalgeneThermo Fisher Scientific | 166-0045 | |
HB 101 Lyophilized Supplement | Irvine Scientific | T151 | |
HB Basal Medium | Irvine Scientific | T000 | |
Heat-Inactivated FBS (Fetal Bovine Serum) | Euroclone | ECS0180L | |
HS (Human serum) | Sigma Aldrich | H3667 | |
Human IL-2 IS | Miltenyi Biotec | 130-097-744 | |
L-Glutamine | Gibco | 11140050 | |
Lymphoprep | Falcon | 352057 | |
Non-essential amino acids solution | Sigma | 11082132001 | |
Paraformaldehyde | Thermo Fisher Scientific | 10538931 | |
PBS (Phosphate-buffered saline) | Thermo Fisher Scientific | 10010023 | |
Penicillin/Streptomycin | Gibco | 15070063 | 10000 U/mL |
PHA (phytohemagglutinin) | Stem Cell Technologies | 7811 | |
Plastic Petri dishes | Thermo Scientific | R80115TS | 10 0mm x 15 mm |
RPMI 1640 Media | HyClone | 15-040-CV | |
Sodium pyruvate | Gibco by Life technologies | 11360070 | |
Syringe Filters 0,45µl | Rotilabo-Spritzenfilter | P667.1 | |
T-25 Cell culture flasks | InvitrogenThermo Fisher Scientific | AM9625 | |
T-75 Cell culture flask | Thermo Fisher Scientific | 10232771 | |
β- Mercaptoethanol | Gibco | A2916801 |