- Research article
- Open Access
Optimization of human corneal endothelial cell culture: density dependency of successful cultures in vitro
- Gary SL Peh†1,
- Kah-Peng Toh†1,
- Heng-Pei Ang1,
- Xin-Yi Seah1,
- Benjamin L George1 and
- Jodhbir S Mehta1, 2, 3Email author
© Peh et al.; licensee BioMed Central Ltd. 2013
- Received: 15 January 2013
- Accepted: 28 April 2013
- Published: 3 May 2013
Global shortage of donor corneas greatly restricts the numbers of corneal transplantations performed yearly. Limited ex vivo expansion of primary human corneal endothelial cells is possible, and a considerable clinical interest exists for development of tissue-engineered constructs using cultivated corneal endothelial cells. The objective of this study was to investigate the density-dependent growth of human corneal endothelial cells isolated from paired donor corneas and to elucidate an optimal seeding density for their extended expansion in vitro whilst maintaining their unique cellular morphology.
Established primary human corneal endothelial cells were propagated to the second passage (P2) before they were utilized for this study. Confluent P2 cells were dissociated and seeded at four seeding densities: 2,500 cells per cm2 (‘LOW’); 5,000 cells per cm2 (‘MID’); 10,000 cells per cm2 (‘HIGH’); and 20,000 cells per cm2 (‘HIGH×2’), and subsequently analyzed for their propensity to proliferate. They were also subjected to morphometric analyses comparing cell sizes, coefficient of variance, as well as cell circularity when each culture became confluent. At the two lower densities, proliferation rates were higher than cells seeded at higher densities, though not statistically significant. However, corneal endothelial cells seeded at lower densities were significantly larger in size, heterogeneous in shape and less circular (fibroblastic-like), and remained hypertrophic after one month in culture. Comparatively, cells seeded at higher densities were significantly homogeneous, compact and circular at confluence. Potentially, at an optimal seeding density of 10,000 cells per cm2, it is possible to obtain between 10 million to 25 million cells at the third passage. More importantly, these expanded human corneal endothelial cells retained their unique cellular morphology.
Our results demonstrated a density dependency in the culture of primary human corneal endothelial cells. Sub-optimal seeding density results in a decrease in cell saturation density, as well as a loss in their proliferative potential. As such, we propose a seeding density of not less than 10,000 cells per cm2 for regular passage of primary human corneal endothelial cells.
- Human corneal endothelium
- Human corneal endothelial cells
- Primary cell culture
- Cell density
The human cornea is a transparent dome-like disc found on the anterior segment of the eye, and is responsible for the refraction of light to the retina in the posterior eye for visual detection. This clear tissue consists of three cellular layers: the epithelium, stroma, and endothelium, and are separated by two acellular membranes (Bowman’s and Descemet’s) . The role of the mono-layered corneal endothelium is to regulate corneal hydration, and dysfunction of this critical cellular layer will gradually result in corneal opacification and eventually results in loss of vision and corneal blindness [2–4]. Corneal transplantation is the only option available to restore vision. However, global shortage of available donor graft material and an ageing population requiring transplants, restricts the numbers of corneal transplants performed yearly . This necessitates development of suitable graft alternatives through tissue engineering or a potential corneal endothelial cell replacement therapy through the injection of cultivated corneal endothelial cells (CECs) [5, 6]. In order to facilitate the research and development of the above-mentioned studies, a robust approach that enables consistent propagation of isolated primary human corneal endothelial cells (HCECs) in vitro, to obtain sufficient numbers, is required.
Cells of the human corneal endothelial layer are not known to actively proliferate within the eye, and have been found to be arrested in the G1-phase of the cell cycle . Contact-dependent inhibition, together with factors found within the aqueous humor, keep the corneal endothelium in a non-proliferative state [8, 9]. However, ex vivo mechanical wounding studies and treatment of HCECs using EDTA to disrupt cell-to-cell contact have shown that these cells retain the capacity to proliferate [10, 11]. The isolation and cultivation of HCECs in vitro have been reported by many groups, some with more apparent success than others . Varying factors from isolation techniques, differing basal media, diverse range of supplements (including different types of growth factors and the concentration of bovine serum used), to individual donor cornea variability accounts for much of the mixed results . In our previous study designed to negate potential donor cornea variability, we showed that the growth of CECs isolated from a single donor behaves differently when placed in culture medium of different formulations . In that study, we identified two culture media, coded in that study as M2  and M4 , to be able to support the active proliferation of isolated HCECs. Interestingly, some of the established primary HCEC-cultures showed differential growth preference for the two proliferative culture media. While most isolated HCECs grew relatively well in either of the medium, some samples displayed a marked preference for one medium over the other . With such complexity involved, a systematic approach is required to be able to further improve the cultivation of HCECs in vitro. For example, it has been postulated that HCECs can be propagated on non-coated cell culture ware , but the use of culture ware pre-coated with extracellular matrices, such as a commercially available serum-free coating solution containing fibronectin, collagen and albumin (FNC coating mixture), greatly improved the attachment and subsequent expansion of the isolated HCECs [12, 16]. More recently, it has been reported that the addition of a selective ROCK inhibitor Y-27632 enhanced cell adhesion and proliferation of CECs isolated from cynomolgus monkeys, which translated to improved cell survival and enhanced cell engraftment for CEC-based regenerative therapy [17, 18].
Previously, it has been reported that the growth pattern of CECs isolated from macaque monkeys is affected by initial cell seeding density, suggesting that successful CEC-culture may be density dependent . To our knowledge, the density dependent growth of HCECs and its effect on in vitro expansion has not been described. The aim of this study was to investigate the density dependency of the growth of primary HCECs isolated from pairs of donor corneas and its implication for a robust cell expansion strategy in order to obtain sufficient numbers of bona fide primary cells for downstream development of a tissue-engineered graft alternative or cell injection therapy.
Ham’s F12, Medium 199, Human Endothelial-SFM, fetal bovine serum (FBS), Dulbecco’s Phosphate-Buffered Saline (PBS), TrypLE Express (TE), 100× anti-biotic/anti-mycotic solution were purchased from Invitrogen (Carlsbad, CA, USA). Insulin, transferrin, selenium (ITS), ascorbic acid, trypan blue (0.4%) were purchased from Sigma (St. Louis, MO, USA). FNC coating mix was purchased from United States Biologicals (Swampscott, MA, USA). Collagenase A was obtained from Roche (Mannhein, Germany).
The following protocols conformed to the tenets of the Declaration of Helsinki, and written consent was acquired from the next of kin of all deceased donors regarding eye donation for research. This study was approved by the institutional review board of the Singapore Eye Research Institute/Singapore National Eye Centre.
Research-grade human corneoscleral tissues
Days to culture
Cell count (OS/OD)
Acute Cardiac Crisis
Isolation and growth of human corneal endothelial cells
Primary cultures were isolated from human corneoscleral tissues as described previously  with some modifications in the way the isolated HCECs were cultured for expansion. Briefly, corneas were washed three times in a 1× anti-biotic/anti-mycotic solution in PBS (wash buffer) for 15 minutes. Cells of the corneal endothelium were isolated using a two-step “peel-and-digest” approach. A disposable vacuum donor punch (Ripon, England) was used to hold the corneoscleral rims in place, endothelial cell-side up. A short 30 seconds treatment with 0.1% trypan blue solution (diluted in PBS), on the corneal endothelial cell surface was used to outline the Schwalbe’s line. Using sterile surgical forceps, the sheet of Descemet’s membrane with intact endothelium, approximately 0.5 to 1mm posterior to the Schwalbe’s line was carefully removed and incubated in collagenase A (2 mg/ml) at 37°C for at least 4 hours (up to 6 hours) to dislodge the corneal endothelial cells from the Descemet’s membrane. Dislodged corneal endothelial cell-clusters were rinsed once in PBS and further dissociated with a brief treatment of TE for 5 minutes to obtain smaller cell-clumps. The cell clumps were washed and collected after centrifugation at 0.8 g for 5 minutes and plated on FNC-coated tissue culture dishes for attachment. Isolated cells were left to adhere overnight in a stabilization medium made up of Human Endothelial-SFM supplemented with 5% FBS and 1× anti-biotic/anti-mycotic. Adhered HCECs were then cultured in F99 medium containing Ham’s F12 and M199, mixed in a 1:1 ratio, supplemented with 5% FBS, 20 μg/ml ascorbic acid, 1× ITS, 1× anti-biotic/anti-mycotic and 10 ng/ml bFGF. When the cultured cells reached 80-90% confluence, they were exposed to the stabilization medium for at least one week before passage. The inclusion of this step enhanced the morphology of the expanded HCECs (unpublished observation; manuscript in preparation). Cultured HCECs were passaged using TE, and sub-cultured at a seeding density of 10,000 cells per cm2 for each passage and were used at the third passage for this study. At the second passage, cultured HCECs were dissociated and plated at the following seeding densities: 2,500 cells per cm2 (‘LOW’), 5,000 cells per cm2 (‘MID’), 10,000 cells per cm2 (‘HIGH’), and 20,000 cells per cm2 (‘HIGH×2’). Cells were then cultured for at least 10 days before morphometric analysis. All incubation and cultures of HCECs were carried out in a humidified incubator at 37°C with 5% CO2 and fresh medium was replenished every two days.
Immunocytochemistry and antibodies
Confluent cultures of primary HCECs grown on glass coverslips at the second passage were fixed in 100% ice-cold ethanol for 5 minutes. The staining procedure involved immersion of the fixed sample in a block solution of PBS containing 10% normal goat serum for 30 minutes. Samples were subsequently incubated with the primary antibody for an hour, followed by a secondary antibody in the dark for 30 minutes at room temperature. Between incubations, samples were rinse twice within PBS. Labeled samples were mounted onto glass slides in Vectashield containing DAPI (Vector Laboratories, Burlingame, CA, USA) to counter-stain cell nuclei. Fluorescence images were captured using a Zeiss Axioplan 2 fluorescence microscope (Carl Zeiss, Germany). The primary antibodies used in this study were: mouse IgG1 anti-Na+K+/ATPase α1 (5 μg/mL; Santa Cruz Biotechnology) and mouse IgG1 anti-ZO-1 (5 μg/mL; BD Biosciences Pharmingen). Secondary antibody used was Alexa Fluor 488 goat anti-mouse IgG (2 μg/mL; Life Technologies). Negative controls were cells incubated with an anti-mouse IgG1 isotype control (5 μg/mL; BioLegends) in place of the primary antibody.
Morphometric analysis and time-lapse imaging
Cellular morphology of cultured HCECs was captured using a Nikon TS1000 phase contrast microscope with a Nikon DS-Fil digital camera (Nikon, Japan). Morphometric data of the area and perimeter of randomly selected cells from phase contrast images of each seeding density was manually outlined by point-to-point tracing of the cell borders using ImageJ software . Cell circularity was then determined using the formula: , where a value approaching 1.0 indicates a circular profile. Hence, hexagonal HCECs will have a profile closer to 1.0 compared to long and spindly fibroblast-like HCECs. At least 100 HCECs from each condition (n = 3) were analyzed. For time-lapse imaging, HCECs were seeded onto FNC-coated 35 mm dishes and transferred into a time-lapse imaging system: Biostation IM-Q (Nikon, Japan). The incubator chamber within was maintained at 37°C and 5% CO2. Viewing area was selected manually and the system was setup to take images automatically every 30 minutes for 24 hours under both 10× and 20× objective lenses. Images were exported from the Biostation IM-Q format and compiled into video using Avidemux software (http://fixounet.free.fr/avidemux/).
Cell proliferation assay
The proliferation of HCECs grown at 4 different seeding densities at the third passage was assessed using Click-iT™ EdU Alexa Fluor 488 Imaging kit (Invitrogen). This assay measures the incorporation of EdU (5-ethynyl-2’-deoxyuridine) into DNA during active DNA synthesis. Cultured HCECs were sub-cultured onto FNC-coated glass slides at the four seeding densities of 2,500 cells per cm2, 5,000 cells per cm2, 10,000 cells per cm2, and 20,000 cells per cm2 overnight to allow cell attachment. Adhered HCECs were then treated with 10 uM EdU solution for 24 hours. After treatment, cells were fixed in 4% paraformaldehyde (PFA) for 15 minutes at room temperature, rinsed twice with 3% BSA in PBS, and permeabilized with 0.1% Triton X-100 in PBS for 20 minutes at room temperature. Click-iT™ reaction cocktail used to detect the incorporated EdU was made by combining 1× Click-iT™, CuSO4, Alexa Fluor azide and the reaction buffer additive provided in the kit. Samples were incubated in the reaction cocktail for 30 minutes at room temperature in the dark. After two rinses with 3% BSA in PBS, samples were mounted on glass slides with Vectashield containing DAPI. Fluorescence images were captured using a Zeiss Axioplan 2 fluorescence microscope. At least 100 nuclei were analyzed randomly for each donor set (n = 3).
All numeric data obtained are expressed as mean ± standard deviation. Comparisons of HCECs sizes, cell circularity and cell proliferation were statistically analyzed using two-way ANOVA followed by post-hoc Bonferroni test for multiple comparisons (SPSS Statistics 17.0, IBM, Chicago, IL, USA). Comparison of Day 10 and Day 30 sizes of HCECs were performed using an independent sample t-test. Results with a p-value of less than 0.05 were deemed to be statistically significant.
Isolation and cultivation of primary HCECs
Morphometric assessment of P3 HCECs (Day 10) cultured at four plating densities
Cell size and CV of cultured P3 HCECs at Day 10
Cell size ± SD (μm2)
Coefficient of variation (CV)
8117.83 ± 4396.84*
5997.57 ± 2571.47*
5010.97 ± 2003.53*
3440.30 ± 1236.58*
When cultured HCECs from the same series of donors were plated at the two higher seeding densities, at Day 10, they were found to be smaller in size, with a relatively homogenous compact cellular morphology. Specifically, HCECs seeded at the ‘HIGH’ density had an average cellular size of 5010.97 ± 2003.53 μm2, a CV of 0.40 and a cell circular index of 0.78 ± 0.11 (Figure 3). HCECs seeded at the highest plating density (‘HIGH2×’) were distinctly the most compact (3440.30 ± 1236.58 μm2), and were the most homogeneous (CV: 0.36) and hexagonal in shape as suggested by their cellular circularity index of 0.82 ± 0.08 (Figure 3).
Morphometric assessment of P3 HCECs (Day 30) cultured at lower plating densities
Cell size, CV and cellular circularity of cultured P3 HCECs at Day 30
Cell size ± SD (μm2)
Coefficient of variation (CV)
9470.16 ± 3825.78*
0.79 ± 0.12
8299.53 ± 3408.87*
0.78 ± 0.08
Cell proliferation assay
Additional file 1: Movie S1: Time-lapse images of HCECs from the same donor (P2) seeded at a high density (left) and at a low density (right), taken at an interval of 30 minutes for 24 hours. Images from the two densities were complied and stitched together using Avidemux software into a movie. (MOV 3 MB)
Projected cell numbers of cultured HCECs up to the third passage
Projection of the range of HCECs obtainable each passage at confluent
Projected HCECs at each passage
8.0 × 105 to 1.0 × 106 cells
2.1 × 106 to 3.2 × 106 cells
4.5 × 106 to 7.5 × 106 cells
1.0 × 107 to 2.5 × 107 cells
The vision of patients affected by debilitating corneal blindness as a result corneal endothelial dysfunction can be restored by the replacement of the diseased or damaged corneal endothelium with a healthy donor cornea tissue through a corneal transplant. However, there is a global shortage of donor corneas available for transplants and many more are rejected due to low endothelial cell count, as well as potential cultural, logistical and technical difficulties [4, 21]. To overcome the shortage of donor corneas, development of potential graft alternatives through a tissue bioengineering approach is currently of great clinical interest. However, the ability to consistently cultivate sizable numbers of HCECs in vitro is critical in stimulating further research in the development of such a bioengineered graft replacements.
Whilst a consensus has yet been established for the culture of HCECs, studies contributing to the improvements of their cultivation are ongoing. For example, recent studies using CECs isolated from non-human primates (cynomolgus monkey), conducted to investigate the applicability of Rho kinase inhibitor Y-27632 in promoting the cultivation of primate CECs, showed that Y-27632, at a concentration of 10 μM, promoted adhesion, inhibited apoptosis and increased the proliferation of these primate CECs . The authors have since postulated the use of Y-27632 together with a “cell-injection therapy”, as a potential new therapy for patients with dysfunction of the corneal endothelium . In a more recent study, Okumura and colleagues were able to reverse corneal opacification by an injection of 2 × 105 cultivated rabbit CECs or 2 × 105 cultivated monkey CECs into the anterior chambers of respective rabbit or monkey models of corneal endothelial dysfunction . This translates to a seeding density of approximately 3,150 cells per mm2 within a circular area with a 9 mm diameter. As projected in this current study, using the culture strategy described, HCECs isolated from a pair of donor cornea can be expanded to between 4.5 × 106 to 7.5 × 106 cells at confluence by the second passage. Hypothetically, adopting the cell numbers used in the cell injection therapy (2 × 105 cells per eye) reported by Okumura and colleagues , cultivated confluent human CECs obtainable at the second passage can potentially treat 22 to 37 cases of corneal endothelial dysfunction via cell-injection therapy. Alternatively, similar numbers of tissue-engineered HCEC-constructs can be potentially generated on either synthetic or biological carriers (reviewed in ) as alternative graft materials.
To improve the growth of CECs, it was reported in an earlier study that there is a significant relationship between cell density and the growth of primate CECs isolated from non-human primate (macaque monkey) . To our knowledge, there is no published data showing cell density dependent growth for extended cultivation of primary HCECs. In this present study, the growth dynamics of cultivated HCECs was examined when expanded HCECs, from each donor at the second passage were plated out at 4 seeding densities in an attempt to delineate an optimal seeding density for their continual in vitro expansion. Based on cellular morphology, our results showed that there is a density dependency in the growth of primary HCECs. Lower seeding densities tend to encourage greater cell proliferation for the first few days, although this observation was not significant. As assessed by cell morphometric measurements at Day 10 in culture, HCECs seeded at lower densities were significantly larger in size, became heterogeneously variable in terms of their cellular shape, and contained mixtures of hexagonal HCECs, as well as enlarged or elongated fibroblast-like cells (Figure 2). Comparatively, HCECs from the same series of donors that were passaged at higher plating densities retained relatively compact cellular morphology, characteristic of the naïve corneal endothelium. This result is consistent with the findings reported for primate CEC-cultures . Interestingly, HCECs plated at the low or medium densities were unable to form a compact monolayer even after extended culture for 1 month. Some form of cellular reorganization occurred as the cultures became more homogeneous and rounder when analyzed at Day 30. Such cellular reorganization and cellular spreading phenomena have has been reported in vivo where existing cells of the corneal endothelium spread out to maintain the functional integrity of the corneal endothelial layer to sustain corneal deturgescence and maintain corneal transparency as a way to replace dead or damaged CECs [22, 23]. However, HCECs seeded at lower densities remained significantly larger compared to cells plated at higher densities (Table 3). This result can be inferred as an overall loss of proliferative potential . The decrease in saturation density, together with an increase in cell size, as well as the loss of further division capability are also hallmarks of cellular senescence (review in ). However, it should be noted that cultivated HCECs are mediated in part by contact-induced inhibition . Hence it is unclear if the loss of proliferative potential is due to premature cellular senescence or contact inhibition. Hence further studies to delineate the mechanisms that may be in play should focus on the gene signatures, protein expression or enzyme activity such as senescence-associated beta galactosidase, as well as the activity of p27kip1 in cultured HCECs that are plated at a lower seeding density.
Our results demonstrated that the successful outcome of extended culture of primary HCECs is negatively impacted by lower, sub-optimal plating density, and can significantly affect their proliferative potential. Even though HCECs may be viable when seeded at lower densities, the quality of those cells was not comparable to cells that were sub-cultured at higher densities. From a pair of donor corneas, using the isolation methodologies and culture approach for the propagation of isolated primary HCECs described in this study, and following a seeding density of not less than 1 × 104 cells per cm2, it is possible to obtain up to 2.5 × 107 cells with preserved polygonal/hexagonal cellular morphology that resembled cells of the corneal endothelium at the end of the third passage. Whether cultivated HCECs should be utilized at the second or third passage is the subject of further functional characterization using both in vitro (cellular physiology) and in vivo (corneal dysfunction animal model) approach. Nevertheless, a robust culture strategy that can consistently produce a sizeable number cultivated bone fide primary HCECs is essential to facilitate the validation of cell-injection therapy, or downstream development of an alternative corneal endothelium construct through cell-tissue engineering.
We thank SBIC-Nikon Imaging Centre (Singapore) for their assistance and for the use of the Biostation IM-Q live cell recorder. We also thank Lion Eye Institute for Transplant and Research (Tampa, FL, USA) for their assistance with procurement of the research-grade donor corneas used in this study. This work was supported by grants from the National Research Foundation Translational and Clinical Research (TCR) Programme Grant (R621/42/2008) and from the Biomedical Research Council Translation Clinical Research Partnership (TCRP) Grant (TCR0101673). The funding bodies had no role in study design, data collection, analysis, decision to publish, or preparation of the manuscript.
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