Magnetically steered cell therapy for reduction of intraocular pressure as a treatment strategy for open-angle glaucoma

We delivered and magnetically steered either hAMSCs or iPSC-TMs to the TM of eyes of MYOC^Y437H mice (Figure 1; mice described above), measuring IOPs and outflow facilities at short-, mid-, and long-term time points, corresponding to ~1 month, 3–4 months, and 9 months after cell delivery (Figure 1). Our high-level goals were to: (i) elucidate the impact of hAMSC or iPSC-TM delivery on IOP; and (ii) quantify the portion of IOP change due to changes in outflow facility, a key functional metric of the TM. Outflow facility is the numerical inverse of the hydraulic resistance to AH drainage through the conventional outflow pathway.

We expected transgenic MYOC^Y437H mice to show elevated IOP by 6–7 months of age, when baseline IOP measurements were taken (Zhu et al., 2016; Zhu et al., 2017; Zode et al., 2011). Surprisingly, we saw no meaningful IOP difference between Tg-MYOCY437H mice (Tg group) and wild-type (WT) littermates (Figure 2; Table 1 and Table 2). Despite this lack of IOP elevation in the transgenic model, magnetically steered delivery of hAMSCs led to a marked IOP decrease in Tg animals as compared to sham injection of saline at short-, mid-, and long-term time points. The IOP reduction was sustained in hAMSC-treated eyes over all three time points, with no statistically significant difference between any combination of these time points. iPSC-TM treatment also led to a reduction in IOP compared to sham (phosphate-buffered saline [PBS]) injection controls at both the short- and mid-term time points, although this difference did not reach statistical significance at the latter time. The IOP reduction due to iPSC-TM cells was approximately half that due to hAMSC treatment at both short- and medium-term time points (short term: ${\displaystyle -4.3\left[-5.6,-2.9\right]\mathrm{m}\mathrm{m}\mathrm{H}\mathrm{g}}$ for hAMSC vs. ${\displaystyle -2.3\left[-3.6,-1.0\right]\mathrm{m}\mathrm{m}\mathrm{H}\mathrm{g}}$ for iPSC-TM, $p=0.021$; mid-term: ${\displaystyle -4.5\left[-5.8,-3.1\right]\mathrm{m}\mathrm{m}\mathrm{H}\mathrm{g}}$ for hAMSC vs. ${\displaystyle -1.9\left[-3.3,-0.4\right]\mathrm{m}\mathrm{m}\mathrm{H}\mathrm{g}}$ for iPSC-TM, $p=0.005$; all data reported as means and 95% confidence intervals).

Figure 2

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We observed increases in outflow facility for eyes receiving stem cells which were consistent with observed changes in IOP (Figure 3A and B; Table 1 and Table 2). Specifically, no significant difference in facility was found between the naïve WT and transgenic groups, while hAMSC treatment led to a marked increase in outflow facility vs. injection (sham) controls at short-, mid-, and long-term time points. Further, the percentage increases in facility due to hAMSC delivery vs. sham injection controls were similar at all time points. Groups receiving iPSC-TMs also showed an increase in facility, but these differences did not reach statistical significance. Specifically, hAMSC delivery led to a significantly higher percentage increase in facility compared to iPSC-TM delivery: short-term: ${\displaystyle 170\left[70,310\right]\mathrm{\%}}$ for hAMSC vs. ${\displaystyle 40\left[-10,110\right]\mathrm{\%}}$ for iPSC-TM, $p=0.011$ ; mid-term: ${\displaystyle 180\left[110,280\right]\mathrm{\%}}$ for hAMSC vs. ${\displaystyle 40\left[0,110\right]\mathrm{\%}}$ for iPSC-TM, $p=0.003;$ data reported as percent increase in treatment group compared to relevant (sham) injection control.

Figure 3

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We then asked whether the measured decreases in IOP were quantitatively consistent with the experimentally measured increases in outflow facility. To answer this question, we used the modified Goldmann equation (Brubaker, 2004), which relates IOP to facility and other variables, computing an ‘expected’ IOP from the facility measurements for each cohort of mice. Comparison of this expected IOP with the actual (measured) IOP showed a close correlation (Figure 3Ci), determined by linear regression (slope of fitted line was not statistically different from one, $p=0.22$, $R^2=0.99$). Still, the outflow facility measurements overestimated the actual IOP by a small amount (${\displaystyle 1.2\left[1.1,1.3\right]\mathrm{m}\mathrm{m}\mathrm{H}\mathrm{g}}$, ${\displaystyle p<{10}^{-6}}$, null hypothesis: average difference between experimental and expected IOPs equals zero, Figure 3Cii). Despite this ‘shift’ between the experimentally measured and expected IOP, the horizontal error bars in Figure 3Ci, derived by a propagation of error analysis, include the unity line for all groups, suggesting that the small discrepancy between the two experimental and expected values falls within the measurement errors (see Discussion).

The observed reductions in IOP and increases in outflow facility after delivery of both cell types suggested functional changes in the conventional outflow pathway. We therefore asked whether these changes were associated with alteration of the cellular density in the TM by evaluating cell counts in histological sections of the iridocorneal angle from all of our experimental groups (Figure 4; Table 1 and Table 2). We observed more nuclei in eyes receiving cell transplantation, with a striking 2.2-fold increase in TM cellularity (normalized to the anterior-posterior length of the outflow tissues) after hAMSC treatment at the short-term time point vs. the corresponding (sham) injection control (Figure 4C). Interestingly, this spike in TM cell density was followed by a decline over time, reaching a 1.6-fold increase at the mid-term time point and apparently plateauing at 1.6-fold at the long-term time point. Despite this modest decline, hAMSC-treated eyes showed significantly higher cellular density vs. their injection controls at both mid-term and long-term time points.

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A potential concern with superparamagnetic iron oxide nanoparticle (SPION) loading of stem cells to enable magnetic steering is that SPIONs could cause stem cell cytotoxicity or could leak from stem cells after delivery to the TM, and thus cause cytotoxicity in TM cells. We therefore searched for SPIONs in eyes after stem cell delivery (Appendix 1). Unfortunately, SPIONs were somewhat difficult to visualize, but we did not see notable SPION accumulation in the TM, a finding that is consistent with the significant increase in TM cellularity after MSC delivery.

Delivery of iPSC-TMs also led to an increase in TM cellular density vs. (sham) injection controls at both short-term and mid-term time points, although these differences were more modest than seen in hAMSC-injected eyes and did not reach statistical significance. Interestingly, the TM cellular densities in iPSC-TM-treated eyes at both time points were comparable to those at the mid-term and long-term time points in hAMSC-treated eyes but were significantly different than hAMSC-treated eyes at the short-term time point.

Cross-plotting normalized TM cellularity vs. IOP for pooled data from all the experimental groups (Figure 4D) showed a strong negative correlation between these two parameters, indicating an association between greater TM cellularity and lower IOP.

An increased deposition of extracellular matrix (ECM), and, in particular, basement membrane material (BMM), in the TM immediately adjacent to the inner wall (IW) of Schlemm’s canal has been associated with ocular hypertension (Li et al., 2021; Overby et al., 2014). Since this region within the TM accounts for the majority of AH outflow resistance (Ethier et al., 1986), we asked whether the amount of BMM was altered by stem cell treatment. To address this question, we compared the mid-term hAMSC transplanted group vs. its corresponding injection control (Figure 5), selecting the mid-term time point for this analysis since this was the longest time point previously studied (Zhu et al., 2017), and we were interested in persistent ECM changes within the TM.

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Reduced amounts of BMM adjacent to the IW of Schlemm’s canal were evident in transmission electron micrographs from eyes receiving hAMSCs compared to sham-injected controls at the mid-term time point (Figure 5A). Quantification showed that stem cell treatment significantly decreased the amount of BMM, as determined by the ratio of BMM length adjacent to Schlemm’s canal IW to total IW length; specifically, this ratio was 0.52 [0.34, 0.70] in sham-treated eyes vs. 0.34 [0.22, 0.47] in hAMSC-treated eyes (${\displaystyle p<0.0001}$). The BMM length ratio was measured by two independent annotators (MRB, CRE), and differences between the annotators were not significant (annotator considered as a random effect, $p\approx 1$, likelihood ratio test).

Manuguerra-Gagné et al. previously reported a surprisingly low retention duration of hAMSCs in the TM of rat eyes, with virtually no fluorescently labeled exogenous cells being present in histological sections 4 days after injection (Manuguerra-Gagné et al., 2013). We therefore pre-labeled injected cells with PKH26 fluorescent dye, which allowed us to track cells for up to 3 weeks after injection. En face images showed a relatively uniform distribution of cells over the entire circumference of the eye (Figure 6A), similar to previous results with magnetically steered cells (Bahrani Fard et al., 2023). Sagittal sections (Figure 6B) showed an accumulation of exogenous cells deep within the iridocorneal angle. Interestingly, strong fluorescent signals were observed within the TM in iPSC-TM-injected eyes, indicating cell integration with the target tissue; in contrast, most hAMSCs accumulated close to the TM (within 50 µm), but did not enter the TM. Note that fluorescent signals observed in the posterior part of the eye and outside the eye near the limbus were caused by autofluorescence (Figure 6—figure supplement 1).

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Unfortunately, there was a very high rate of tumorigenicity in eyes receiving iPSC-TMs, with more than 60% of eyes showing large intraocular masses within a month of cell injection, typically on the iris (Figure 6B). In most cases, these tumors left the eyes unusable for IOP or outflow facility measurements. Examination of select iPSC-TM-transplanted sections by a board-certified pathologist (HEG) confirmed the presence of tumors (Figure 7), based on observation of rosettes and neuroectodermal phenotype, characteristics also found in various tumor types, including retinoblastoma (Wippold and Perry, 2006). Additionally, a high nuclear-cytoplasmic ratio, a hallmark of tumor malignancy (Moore et al., 2019), and rarefaction due to tissue necrosis were noted. No signs of tumor growth were observed in the eyes injected with hAMSCs at the long-term time point (Figure 7).

Figure 7

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Our major finding was that magnetically steered delivery of hAMSCs led to a significant and sustained lowering of IOP, which could be almost entirely explained by improved function of the conventional outflow pathway. Specifically, we saw an ~27% (4.5 mmHg) IOP reduction in eyes receiving hAMSCs vs. saline (sham) injection control eyes, which was sustained for 9 months after cell delivery. This lowering of IOP was closely related to a stable ~2.8-fold increase in outflow facility in the hAMSC treatment group vs. saline injection controls.

Eyes subjected to saline injection exhibited marginally higher IOPs and lower outflow facilities on average, in comparison to the transgenic animals at baseline. However, due to the lack of statistical significance in these differences and the inherent age difference between the saline-injected animals and the non-injected controls at baseline, no conclusive inference can be drawn regarding the effect of saline injection. To investigate this phenomenon further, we also analyzed IOPs in uninjected contralateral eyes at the mid-term time point (Appendix 2). The uninjected contralateral transgenic eyes (10 months of age) showed an IOP of 16.5 [15.9, 17.1] mmHg, which was intermediate between the IOP levels of the 6- to 7-month-old Tg group (15.4 [14.7, 16.1] mmHg) and the sham-injected group (16.9 [15.5, 18.2] mmHg). However, none of these differences reached statistical significance. Of note, contralateral hypertension has been previously reported after subconjunctival and periocular injection of dexamethasone-loaded nanoparticles (Li et al., 2019), and we similarly cannot definitively rule out potential contralateral effects induced by our stem cell injections. Thus, we cannot draw any definite conclusions from these additional IOP comparisons at this time.

Our measured IOPs were close to ‘expected IOPs’ calculated from facility measurements, strongly suggesting that the majority of the IOP-lowering effect after hAMSC delivery was due to an improvement in the function of the conventional outflow pathway.

Despite the very close correlation between measured and expected IOPs noted above, there was a small but consistent offset between these two quantities, which may be due to several factors. First, cell delivery could theoretically cause a decrease in the rate of AH formation or an increase in the rate of uveoscleral outflow, which would lower experimentally measured IOP. However, according to Equation 2, a change in the pressure-independent flow rate ($Q$) would disproportionately affect the IOP in groups with lower facility. For example, if we conservatively assume that the 1.2 mmHg average residual (experimental IOP – expected IOP) was caused by a difference in inflow rate for transgenic animals vs. WT animals, which we used as the reference for calculating inflow rate (see Materials and methods), the 95% confidence interval on the mean of the residuals would have been ~5 times larger than what we actually calculated. The second possible explanation is that the mismatch was caused by an error in rebound tonometry, e.g., due to tonometer miscalibration or an anesthesia-induced drop in IOP (Qiu et al., 2014). However, if we assume that all groups, including WT animals, had an experimentally measured IOP that was artifactually lower than true IOP, the pressure-independent flow rate ($Q$) calculated for WT animals would incorporate this effect. Thus, when this $Q$ is used to calculate expected IOPs for groups other than WT animals, there should not be an offset between the experimental and expected IOPs, at least for groups with facilities similar to WT animals. We therefore suggest that the most plausible explanation is an inherent difference between the transgenic and WT animals, such as in the biomechanical properties of the cornea (leading to an error in the IOP read by the tonometer), in the episcleral venous pressure, or in the amount of IOP reduction due to anesthesia.

Despite some uncertainty about the minor offset between the expected and measured IOPs, the data strongly suggests that the IOP lowering caused by stem cell therapy is largely due to a restoration of function to the conventional outflow pathway.

One of the hallmarks of POAG is loss of TM cells (Alvarado et al., 1984), which was an early motivation for TM cell therapy as a potential treatment for this disease. We found that hAMSC delivery led to a striking 2.2-fold increase in TM cellularity 3–4 weeks after treatment vs. saline-injected controls, which showed cellularities similar to eyes from WT mice. This increased cellularity declined somewhat by 3–4 months after cell injection but then stabilized for up to 9 months after injection. Additionally, the increase in cellularity was strongly correlated with a decrease in IOP for pooled data from all the experimental groups. This correlation more directly highlights the potential of TM cell therapy in treating ocular hypertension, where TM cellularity is reduced and IOP is elevated (Alvarado et al., 1984). Interestingly, Alvarado et al., 1984 showed that humans at birth have ~2.3-fold higher TM cellularity compared to a 40-year-old individual, and that this cellularity reduces sharply within the first 5 years of life. This trend in human eye cellularity resembles, both qualitatively and quantitatively, our observations after hAMSC treatment when the ~27 months’ average lifespan (Graber et al., 2013) of the mouse is taken into account. Further studies of factors controlling TM cellularity after hAMSC delivery are indicated but lie beyond the scope of the current study.

Another feature of POAG is an accumulation of ECM within the juxtacanalicular tissue (Fuchshofer et al., 2003). The mechanism(s) underlying this ECM accumulation are not entirely understood. Nevertheless, increased levels of transforming growth factor-β2 (TGF-β2) in the AH of POAG patients (Tripathi et al., 1994) and its role in decreasing the activity of matrix metalloproteinases (MMPs) suggest that the abnormal ECM deposits may be due to decreased ECM turnover (Fuchshofer et al., 2003; Tamm and Fuchshofer, 2007). Thus, after detecting the significant increase in TM cellularity and reduction in IOP using hAMSCs, we wondered whether transplanted cells would also affect ECM levels in the TM. Our quantification showed that this was indeed the case: hAMSC-transplanted eyes at the mid-term time point had 35% less BMM under the IW of Schlemm’s canal than in saline-injected control eyes. This finding is consistent with the general theme of TM functional restoration seen throughout this study. A future study to analyze the levels of TGF-β2 in the AH, as well as the ratio of active to pro-form levels of MMPs in hAMSC-transplanted eyes, would be of interest to better understand the mechanism through which exogenous cells modulate ECM turnover.

Unfortunately, it is not feasible to directly compare the results of this study with those of previous studies that have successfully demonstrated the efficacy of nonmagnetic cell therapy in MYOC^Y437H mice (Zhu et al., 2016; Zhu et al., 2017). This is due to the unexpected lack of a POAG phenotype in our transgenic mice (discussed in detail below). Yet in our study, we found a stable IOP lowering and increase in outflow facility over 9 months (corresponding to one-third of the animals’ lifespan), which for the first time attests to the possible longevity of IOP lowering due to TM cell therapy. In addition, because of the targeted nature of our delivery technique, we could achieve these reported therapeutic outcomes by injecting a total of only ~1500 cells, which is significantly lower, i.e., more efficient, than the 50,000 cells used in previous studies (Zhu et al., 2016; Zhu et al., 2017).

One literature comparison that can be made is for the BMM normalized length. Li et al., 2021 reported values of 0.40 [0.23, 0.57] for this quantity in naïve eyes and 0.50 [0.38, 0.60] for sham-injected (PBS containing nonconjugated polymeric nanoparticles) eyes in 2- to 3-month-old C57BL/6 mice. Overby et al., 2014 measured a BMM normalized length of 0.29 [0.16, 0.42] in 6- to 7-month-old mice from the same strain. Despite our sham mid-term group being 9–11 months of age and being on a transgenic background, with no phenotypic manifestation, the 0.52 [0.34, 0.70] BMM normalized length we measured for this group is consistent with those previously reported values. The fact that we observed reduced BMM length in cell-treated eyes vs. control values may suggest that a homeostatic balance in cell-treated eyes was tipped toward the presence of less BMM, consistent with hypotensive IOP measurements and greater outflow facility.

This study for the first time compared the IOP-lowering performance of hAMSCs vs. iPSC-TMs – two of the most clinically relevant cell types for future TM cell therapy (Coulon et al., 2022). Surprisingly, we found that the performance of iPSC-TMs was significantly inferior to that of hAMSCs, as quantified by several outcome measures; most notably, the IOP reduction after iPSC-TM cell delivery was only half that seen after hAMSC delivery. The beneficial effect of iPSC-TM treatment on TM cellularity was also significantly lower than hAMSC at the short-term time point (1.4-fold vs. 2.2-fold increase), although this difference declined at the mid-term time point (1.4-fold vs. 1.6-fold increase). In addition to their IOP-reducing efficacy, another major drawback of the iPSC-TMs was the high incidence of ocular tumorigenicity. More than 60% of the eyes injected with iPSC-TM cells developed tumors, requiring termination of the experiment. A body of previous literature, including a systematic review of 1000 clinical trials involving mesenchymal stem cell transplantation, finds no incidence of tumorigenicity in tissues receiving mesenchymal stem cells, suggesting an intrinsic resistance to tumor formation once positioned in the correct niche (Lalu et al., 2012; Rodríguez-Fuentes et al., 2021). On the other hand, tumorigenicity remains a concern for iPSC derivatives due to transfection with oncogenic factors, genetic aberrations during in vitro cultures, and contamination of transplants with undifferentiated cells (Neri, 2019; Lamm et al., 2016; Yamanaka, 2020). Despite following a protocol to isolate differentiated iPSC-TM cells, including using a non-integrating viral vector for transfection of reprogramming factors and a commonly used magnetic activated cell sorting approach (Yamanaka, 2020), there unfortunately remains a chance for contamination and reprogramming of these cells posttransplantation. Interestingly, the iris is reported to be a favorable location for organ culture and tumor formation, with fivefold faster growth compared to subcutaneous injection, and thus has previously been considered for tumorigenicity safety studies, emphasizing the importance of rigorous iPSC processing in any future treatments involving iPSC-TM cell injection into the anterior chamber (Olson and Seiger, 1972; Inagaki et al., 2022; Boone and DuPree, 1968).

Both cell types were detectable in the anterior chamber 3 weeks after injection (Figure 6B), with iPSC-TM cells tending to better integrate with the TM tissue, whereas the hAMSCs mostly accumulated close to, but not within, the TM. This phenomenon, which was consistently observed, may be due to the widely reported aggregation of mesenchymal stem cells immediately posttransplantation (Burand et al., 2020), which consequently prevented them from entering the deeper aspects of the TM, characterized by narrow flow channels. Note that the exogenous iPSC-TMs more directly contributed to increasing TM cellularity than did the hAMSCs due to the better integration of iPSC-TM cells into the TM. This finding complicates the interpretation of the relationship between increased TM cellularity and IOP reduction. In addition, loss of signal in long-term in vivo fluorescent cell tracking is inevitable (Progatzky et al., 2013), so the fluorescent signal in Figure 6 may not be marking all the exogenous cells retained in the anterior eye.

The lack of specific hAMSC homing into the TM also provides important insight about the putative mechanism(s) by which these cells lowered IOP and improved AH dynamics. Several hypotheses address how injected cells may affect TM functional restoration: exogenous cells can either integrate with the TM and differentiate into TM-like cells, or can promote endogenous TM cell proliferation through direct contact or through their secretome. Du and colleagues, in two studies using mice, showed that TMSCs that reach the TM co-express AQP1 and CHI3L1, indicative of their differentiation into TM cells, although quantification was not performed (Yun et al., 2018; Xiong et al., 2021). Zhu et al., 2016 reported a 114% increase in TM cellularity after iPSC-TM injection in MYOC^Y437H mice compared to saline-injected controls, yet TM-residing exogenous cells accounted for only 23% of this increase. This finding is consistent with several studies that report the proliferative effect of exogenous cells on the TM in terms of higher Ki-67 expression and BrdU signal, as well as an increased prevalence of Nestin+ progenitor cells (Manuguerra-Gagné et al., 2013; Zhu et al., 2016; Zhu et al., 2020). How this proliferation is mediated, however, is a matter of controversy. In two studies, Zhu et al. showed that iPSC-TMs induce significant proliferation of both cells from the TM5 cell line (an immortalized TM cell line) or primary TM cells carrying Ad5RSV-myocilinY437H when in co-culture, yet did not when they were co-cultured in the presence of a physical (membrane) separation between iPSC-TMs and TM cells (Zhu et al., 2016; Zhu et al., 2020). Interestingly, Xiong et al., 2021 conducted similar experiments with TMSCs and MyocY437H primary TM cells and observed no proliferative effect with or without contact between the cells. On the contrary, two studies have reported the beneficial effect of injecting conditioned media from bone marrow MSCs in hypertensive rat eyes, including a significant reduction in IOP, neuroprotection, and elevated proliferation markers in the TM (Manuguerra-Gagné et al., 2013; Roubeix et al., 2015). In our study, the significant lowering of IOP seen after the delivery of hAMSCs and their accumulation near, but not within, the TM supports the notion that injected cells act upon the TM through their secretome. Thus, a proteomic comparison of the secretome of hAMSCs and iPSC-TMs may provide significant insight into their paracrine effect on TM functional restoration.

The main limitation of this study was the lack of a POAG phenotype in our transgenic mouse colony. Even though MYOC^Y437H mice have previously been shown to exhibit an elevation in IOP and a decrease in both outflow facility and TM cellularity, our colony did not show any difference in those parameters compared to WT animals. While we are not certain of the cause, one possibility is that our IOP measurements were inaccurate. However, this is unlikely because of the correlation between measured IOP and outflow facility in cohorts (Figure 3C) and the fact that IOPs in our WT animals lay within previously reported ranges (Zhu et al., 2016; Zhu et al., 2017; Overby et al., 2014; Yun et al., 2014). It should be noted that reported IOPs for anesthetized WT C57BL/6 mice vary depending on the measurement method used, with a lower bound of ~12.5 mmHg under deep levels of injection-induced anesthesia (John et al., 1997) and an upper bound of ~20 mmHg under gas-induced extra light anesthesia (Li et al., 2021), with values close to our measurements being frequent in the literature. An alternative, and perhaps more likely, possibility is that the transgene was silenced in the original breeders of this colony. Unfortunately, this only became evident after the 6–7 months’ wait time required for the expected onset of the phenotype. Despite the strong effectiveness of our novel TM cell therapy technique (even in the absence of ocular hypertension), the main concern is whether cell therapy would work as effectively in a glaucomatous eye. Raghunathan et al., 2018 showed that when healthy TM cells are cultured on the ECM derived from glaucomatous TM cells, the healthy cells experience differential stiffening and altered expression profiles similar to the glaucomatous phenotype. Therefore, a glaucomatous ECM may negatively impact the exogenous cells and curtail their therapeutic potential. Fortunately, since in our study, hAMSCs did not seem to need to integrate into the TM to lower IOP, they may also not be affected by glaucomatous changes in the TM. Additionally, Goldmann’s equation (Equation 2) shows that the same percentage increase in outflow facility produces a greater magnitude of IOP lowering in a hypertensive eye vs. in a normotensive eye. Therefore, evaluation of magnetically steered hAMSC cell therapy in an alternative preclinical glaucoma model is indicated.

An additional limitation is that, since histology was only performed on a subset of the eyes after outflow facility measurements, it is possible that there may also have been undetected tumors in the iPSC-injected eyes reported in the IOP and outflow facility plots. This could affect the reported efficacy of the iPSC-TM cells, and further experiments comparing hADMSCs to more carefully processed iPSC-TM cells may be worthwhile.

In summary, this work shows the effectiveness of our novel magnetic TM cell therapy approach for long-term IOP reduction through functional changes in the conventional outflow pathway. The comparison between hAMSCs and iPSC-TM cells strongly suggested the inferiority of the latter cell type in this treatment paradigm, as judged by tumorigenicity and less effective IOP lowering. The localization of injected hAMSCs deep in the iridocorneal angle, but not full integration into the TM, supports the hypothesis that exogenous cells promote TM functional restoration through paracrine signaling. Therefore, even though the mouse model used in this study did not show a POAG phenotype, this treatment approach merits further study with the eventual goal of clinical translation.

We conducted experiments in several cohorts of mice, as follows:

• WT: wild-type hybrid mice (naïve controls)

• Tg: Tg-MYOCY437H mice, a model of POAG (see details below)

• Sham: Tg mice receiving PBS (injection controls)

• hAMSC: Tg mice receiving magnetically steered hAMSCs

• iPSC-TM: Tg mice receiving magnetically steered iPSC-TMs

Our key outcome measures were IOP, outflow facility, TM cellularity, cell retention in the anterior segment, and ultrastructural analysis of TM ECM, with timelines as indicated in Figure 1B. All measurements were made in ex vivo eyes, except for IOP, which was measured longitudinally in living mice.

After breeding and genotyping, mice, regardless of sex, were maintained to age 6–7 months, when transgenic animals were expected to have developed a POAG phenotype. We then made baseline measurements and performed stem cell (or sham) injections and followed animals for various durations:

• Short-term: 3–4 weeks after cell injection

• Mid-term: 3–4 months after cell injection, and

• Long-term: 9 months after cell injection.

Exogenous cell retention in the anterior chamber was measured at only the short-term time point. This is because, in our experience (data not shown), the tracer’s signal was only faintly present 2 months after injection in vivo, while signal was maintained for a longer period in vitro, as advertised by the manufacturer. We are unsure whether this loss of signal was caused by a loss of cell integrity or by fluorescence fading in vivo. Further, due to the high incidence of tumorigenicity and inferior overall effectiveness in animals receiving iPSC-TM cells, long-term measurements, as well as ultrastructural analysis, were not pursued for this group. We chose to perform ultrastructural analysis for the hAMSC group at the mid-term time point, as this is the longest time point previously studied (Zhu et al., 2017) and enables comparison with previous work.

hAMSCs were purchased commercially (Lonza Bioscience, Walkersville, MD, USA) and were prepared for injection as described previously (Bahrani Fard et al., 2023). The cells were maintained at 37°C and 5% CO₂ in α-MEM supplemented by 10% FBS and 1% penicillin and streptomycin and 2 mM L-glutamine. Cells were passaged using 0.05% trypsin (25-053 CI, Corning Inc, Corning, NY, USA) to detach cells, followed by resuspension and seeding at 5000 cells/cm² in T-25 cell culture flasks. hAMSCs at 80% confluence (passage 5 or 6) were magnetically labeled by overnight incubation with 150 nm amine-coated SPIONs (SA0150, Ocean NanoTech, San Diego, CA, USA) at 25 µg/ml, followed by inspection under light microscopy to verify sufficient SPION endocytosis. Cells were then trypsinized, resuspended by the addition of cell culture media, and placed in a 1.5 ml microtube. To remove insufficiently magnetized cells, a 0.25” cubic N52 neodymium magnet was placed on the side of the tube, resulting in rapid formation of a cell pellet close to the magnet. Supernatant and nonmagnetic cells were then removed.

In exogenous cell retention studies, the cells remaining in the microtube were labeled using the PKH26 lipophilic dye kit (Sigma-Aldrich, St. Louis, MO, USA) according to the manufacturer’s instructions. In brief, a cell solution was prepared in the diluent component of the kit and was vigorously mixed with an equal volume of the 4 µM dye solution. After 3 min at room temperature, an equal volume of FBS was added to the cell solution to stop the reaction, and cells were washed three times with the cell culture media to remove any unbound dye. For all the experiments where animals received hAMSC, cell count and >90% viability were verified using a Countess II Automated Cell Counter (Thermo Fisher Scientific, Waltham, MA, USA). The cells were then resuspended in sterile PBS (1X, Thermo Fisher Scientific, Waltham, MA) to a final concentration of 1k cells/µl.

Mouse iPSC-TMs have previously been developed and characterized (Zhu et al., 2016). In brief, mouse dermal fibroblasts are reprogrammed through Sendai virus-mediated reprogramming with the transcription factors OCT4, SOX2, KLF4, and c-MYC. The pluripotency of reprogrammed iPSCs was confirmed using RT-PCR, immunocytochemistry, immunoblotting, and teratoma formation. iPSCs were then differentiated by culturing in conditioned media from primary human TM (phTM) cells. To prepare this conditioned media, phTM cells were extracted from donor eyes and cultured in α-MEM supplemented by 10% inactivated FBS and 2% primocin. Conditioned media was then collected from the cells and sterilized by passing through a 0.2 µm membrane filter. The iPSCs were maintained in conditioned media for 8 weeks to induce differentiation. It is important to remove any undifferentiated iPSCs from the iPSC-TM populations due to the risk of tumorigenicity associated with pluripotent stem cells. Therefore, the iPSC-TMs were incubated with CD15 antibodies (Miltneyi Biotec, Bergisch Gladbach, Germany) conjugated with magnetic microbeads to label the undifferentiated iPSCs. Then, the cells were washed, loaded into a MACS LD column, and were placed in a magnetic separator (Miltenyi Biotec, Germany).

All animal procedures were approved by the Georgia Tech Institutional Animal Care and Use Committee (approved IACUC protocol number A100282) and performed in conformance with the ARVO Statement for the Use of Animals in Ophthalmic and Vision Research. Breeder pairs of C57BL/6 Tg-MYOCY437H mice were shipped from Iowa to a quarantining facility (Charles River, Wilmington, MA, USA), underwent IVF rederivation, and were shipped to Georgia Tech after ~4 months. Breeders carrying one copy of the transgene on a C57BL/6 background were crossed with SJL mice (Charles River) of similar age, with half of the hybrid offspring carrying the transgene. Pups were genotyped using human MYOC primers (forward: CGTGCCTAATGGGAGGTCTAT; reverse: CTGGTCCAAGGTCAATTGGT). Only F1 animals were used in studies.

Cell injection needles were fabricated as described previously (Bahrani Fard et al., 2023). In brief, glass micropipettes were pulled using a pipette puller (P-97, Sutter Instruments, Novato, CA, USA), and the tips were broken and beveled at a 30° on a microelectrode beveler (BV-10, Sutter Instruments, Novato, CA, USA), followed by rotating to both sides for enhanced sharpness (tri-beveling). The resulting needle had a pointed tip and an outer diameter of approximately 100 µm. Cell adhesion to the needle walls in the lumen can cause inconsistent cell delivery to the eye; thus, we plasma-cleaned the needles, coated them with trichlorosilane, and loaded them with 0.02% Pluronic F-127 (P2443, Sigma-Aldrich) for 1 hr at room temperature, followed by vigorously rinsing with PBS. Needles were sterilized with 70% ethanol prior to injections.

Each animal was prepared for unilateral injection of cells by applying a tropicamide eyedrop (Bausch & Lomb, Bridgewater, NJ, USA) to start pupil dilation before inducing anesthesia using an induction chamber receiving 2.5% isoflurane at 600 ml/min. Once the toe-pinch reflex was lost, the animal was transferred to a heated bed, and the head was immobilized with Velcro straps while anesthesia was maintained through a nose cone. A drop of tetracaine (Bausch & Lomb) was applied to the eye being injected while the contralateral eye received ophthalmic lubricant (Systane Ultra, Alcon, Geneva, Switzerland) to prevent drying. The needle, mounted on an injector assembly (MMP-KIT, WPI, Sarasota, FL, USA), was attached to a micromanipulator and connected to a microsyringe pump (PHD Ultra, Harvard Apparatus, Holliston, MA, USA). The needle was filled with 3 µl of the injection solution (either cells or PBS for control [sham] injections), aligned at a 30° angle with the eye, and advanced into the AC in a swift motion until the tip was located approximately in the center of the AC while the eye was held in a proptosed position using a pair of nonmagnetic forceps (Figure 1A). A total of 1.5 µl of the solution was injected at 2.4 µl/min and if the solution contained cells, a point magnet (a thin stainless steel rod attached to a permanent magnet) was used to magnetically steer the cells toward the TM in a continuous motion for the duration of cell ejection from the needle, as previously described in detail (Bahrani Fard et al., 2023). Injected eyes received ophthalmic antibiotic combination ointment (neomycin, polymyxin, bacitracin) and were kept on a heated bed until recovery from anesthesia.

We measured the IOPs between 1 and 3 pm (to minimize diurnal variations) by first placing the mouse in an induction chamber until the righting reflex was lost and breathing slowed. The animal was then transferred to a heated platform, secured with straps, and a tonometer (TonoLab, iCare, Vantaa, Finland) mounted on a micromanipulator (M3301, WPI, Sarasota, FL, USA) was aligned perpendicular to the corneal surface at the center of the cornea. Eight IOP measurements were taken from each eye, and the reported IOP was the average of all eight measurements. Even though some labs exclude the highest and lowest of the eight measurements from the IOP average (McDowell et al., 2022), we did not observe significant intra-measurement variability and thus included all the eight replicates when determining the IOP. The entire duration of IOP measurement was typically 3 min or less, which is less than has been reported for the start of significant anesthesia-induced IOP reduction (Qiu et al., 2014; Tsuchiya et al., 2021).

Outflow facility, which quantifies the ease of fluid drainage from the eye, is defined as the ratio of steady-state outflow rate over IOP in an enucleated eye. We measured facility in enucleated eyes using the previously established iPerfusion system (Sherwood et al., 2016). The system’s sensors were calibrated before each measurement session to ensure reliability and the absence of bubbles or leaks, which can cause large errors in the measurements. Animals were euthanized by intraperitoneal injection of sodium pentobarbital, and eyes were enucleated by sliding a pair of fine-angled forceps behind the eye through the nasal side of the eye socket and pulling the eye out by grabbing onto the optic nerve and the surrounding retrobulbar tissues. The posterior of the eye was secured to a mounting post using a very small drop of cyanoacrylate adhesive (Superglue) inside a heated water bath (35°C) filled with DPBS supplemented with 5.5 mM glucose. A beveled micropipette, mounted on a micromanipulator, was then used to cannulate the eye at a 30° angle. The eyes were stabilized at an IOP of 8 mmHg for 30 min and then perfused at eight evenly distributed pressure steps starting from 4.5 mmHg and finishing at 16.5 mmHg while flow rate and pressure data were acquired (Figure 3Ai–iii). The resulting flow-pressure data were fit with an empirical power-law relationship (Sherwood et al., 2016)

where $C$ is the steady-state outflow facility calculated for each pressure step, $P$ is the steady-state pressure for that step, and the subscript $r$ refers to the parameter evaluated at the reference pressure of 8 mmHg which corresponds to the physiologic pressure difference across the conventional outflow pathway (Sherwood et al., 2016). $\beta$ is a nonlinearity parameter that is determined by data fitting along with $C_r$. A total of 114 eyes were randomly chosen for outflow facility measurements, of which 9 were excluded due to failed perfusion (e.g. poor cannulation).

Steady-state AH dynamics can be described by the modified Goldmann equation (Brubaker, 2004):

where ${\displaystyle Q_{in}}$ is the rate of AH humor formation, $Q_0$ is the uveoscleral (unconventional) outflow rate, and $P_e$ is the episcleral venous pressure. Since the left-hand side of Equation 2 is essentially pressure-independent, $Q$ was assumed to be the same across all the experimental groups.

To cross-validate the IOP and outflow facility measurements, we calculated $Q$ in WT animals by inserting the mean measured outflow facility and mean measured IOP from WT animals into Equation 2, assuming $P_e$ to be 7 mmHg (Sherwood et al., 2016). Average outflow facilities for all the groups were then adjusted using Equation 1 to account for the pressure dependence of facility. Using these adjusted facilities and assuming $Q$ to be the same for all groups, we calculated an ‘expected IOP’ for each experimental group, which can be interpreted as the IOP that is consistent with the measured outflow facility.

Similar to the procedure used previously (Bahrani Fard et al., 2023), all experimental eyes were immersion fixed in 10% formalin (Fisher Healthcare, Waltham, MA, USA) overnight at 4°C after the corresponding in vivo and ex vivo measurements (no measurements were performed on the eyes used for exogenous cell retention study). Of these eyes, a total of 59 were randomly selected from various groups for TM cellularity quantifications. Eyes were then dissected under a surgical microscope, and isolated anterior segments were cut into four leaflets. This anterior segment whole mount was placed on a glass slide with the cornea facing up and mounted with PBS. A Leica DMB6 epifluorescent microscope (Leica Microsystems, Wetzlar, Germany) was used to create fluorescent en face tilescan images. Two quadrants of each whole mount were then prepared for cryosectioning. These quadrants received sequential 15 min treatments in 15% sucrose (Sigma-Aldrich, St. Louis, MO, USA), 30% sucrose, and a 1:1 solution of 30% sucrose and optimal cutting temperature (OCT) media. After embedding in OCT, samples were floated in a 100% ethanol bath cooled by dry ice to flash-freeze. 10-µm-thick sagittal sections were cut using a CryoStar NX70 cryostat (Thermo Fisher Scientific, Waltham, MA, USA) and placed on Superfrost Plus gold slides (Thermo Fisher Scientific, Waltham, MA, USA). In an additional step, specific to TM cellularity quantification, the samples were permeabilized with 0.2% Triton X-100 for 10 min and stained with DAPI (NucBlue Fixed Cell DAPI, Invitrogen, Waltham, MA, USA) for 15 min followed by coverslipping with antifade media (ProLong Gold Antifade medium, Invitrogen, Waltham, MA, USA). Sagittal sections were then imaged as tilescans.

To quantify TM cellularity, ideally all the cells in the TM should be counted. However, due to the partial or complete collapse of Schlemm’s canal and the small separation between the TM and the iris in the murine iridocorneal angle (Li et al., 2019), identifying the boundaries of the TM can be challenging. Thus, to minimize error, we instead counted the DAPI-stained nuclei in the region that we could identify as the TM with a high confidence and normalized this count by the length of the IW of Schlemm’s canal adjacent to this segment (Figure 4A and Figure 4—figure supplement 1). Note that morphological characteristics such as the autofluorescence in the corneoscleral shell, high degree of pigmentation in the iris, as well as the change in the density and orientation of the cells transitioning from the TM to iris helped with locating the TM cell nuclei.

Eyes of animals injected with iPSC-TMs showing anatomical signs of tumor growth were enucleated and immersion fixed in 10% formalin for histopathological studies. Three of these eyes were randomly chosen, dehydrated, and embedded in paraffin. Subsequently, 5-µm-thick sagittal sections were cut using a microtome (Thermo Fisher Scientific, Waltham, MA, USA) and stained with hematoxylin and eosin (H&E). Three additional eyes from the hAMSC long-term group underwent the same procedure for comparison.

The amount of BMM in the hAMSC mid-term experimental group and in corresponding injection control eyes (four eyes in each cohort) was quantified using electron micrographs, using an approach similar to that previously described (Li et al., 2021; Overby et al., 2014). In brief, the two anterior segment quadrants not used for TM cell counting (described above) were immersion fixed overnight at 4°C in universal fixative (2.5% glutaraldehyde, 2.5% paraformaldehyde in Sörensen’s buffer). The specimens were next embedded in Epon resin, and 65 nm sagittal sections were cut through iridocorneal tissues using an ultramicrotome (Leica EM UC6, A-1170; Leica Mikrosysteme GmbH) followed by staining with uranyl acetate/lead citrate. Sagittal sections were examined with a JEM-1400 electron microscope (JEOL USA, Peabody, MA, USA) at ×8000 magnification. At least one section per quadrant was included in the quantification of BMM deposits as described below.

The lengths of BMM segments directly in contact with the IW of Schlemm’s canal and the total length of IW were measured from electron micrographs using ImageJ (Schneider et al., 2012) by two independent annotators in a masked fashion. To enhance BMM identification from micrographs, we first adjusted the contrast for each image, using an ImageJ macro that assigned a brightness level of 255 to a manually selected region of the lumen of SC and a brightness level of zero to a manually selected region of a cell nucleus. The ratio of the length of BMM segments directly underlying the IW to the total length of IW was calculated for each segment, representing the extent of non-fenestrated BMM material underlying the IW. Figure 5—figure supplement 1 exhibits an example of the demarcations. Note that ECM deposits clearly separated from the IW were not considered as BMM deposits.

IOP, outflow facility, and TM cellularity index were tested for normality using the Shapiro-Wilk test for each treatment group. Since the outflow facility is known to be log-normally distributed (Sherwood et al., 2016), facility data was first log-transformed prior to conducting any statistical tests. All outcome measures, except for TM cellularity and normalized BMM length, were analyzed by one-way ANOVA. For TM cellularity and BMM length, we used a linear mixed-effects model, treating the experimental group as the fixed effect while considering the eyes, various sections of each eye, and annotators (for BMM only) as replicates, i.e., as random effects. Following these analyses, we conducted post hoc comparisons with Bonferroni correction. However, we limited our comparisons to those chosen a priori to be relevant to the interpretation of our study to avoid an overly conservative adjustment of critical p-values as required by Bonferroni correction. To compare the impact of different treatments on IOP and outflow facility, we computed the difference between the treatment groups and their respective injection controls. Subsequently, we conducted two-tailed t-tests with Bonferroni correction. Given the log-transformation of facility data, the subtracted values became ratios upon inverse transformation. To check for consistency between IOP and outflow facility measurements, we calculated residuals as the difference between the expected and experimentally measured IOPs. A two-tailed t-test was then performed on these residuals with $H_0:\mu =0$. Pearson’s correlation test was used to measure the relation between TM cellular density and IOP. All analyses were done using MATLAB (v2020, MathWorks, Natick, MA, USA). A significance level of 5% was employed for all tests, unless explicitly stated otherwise.

For reasons described below, it was useful to know where SPIONs had accumulated within the eye. We therefore carried out histological analyses of tissue sections to visualize SPIONs, using a Prussian blue staining process.

SPIONs co-located with exogenous cells posttransplantation

A major concern regarding the use of SPIONs for cell encapsulation is dose-dependent toxicity, which could damage both the transplanted cells and native tissues (Sadeghiani et al., 2005; Stroh et al., 2004). We therefore visualized the SPIONs using Prussian blue staining anterior segment sagittal sections (Appendix 1—figure 1). Unfortunately, this dark blue stain proved barely discernible from pigment. Detectable labeling could mostly be found at comparable locations within the AC as in hAMSC-injected eyes (Figure 6B), where both the cells and SPIONs accumulated in the vicinity of TM, and in iPSC-TM-injected eyes (Figure 6B), with the cells and SPIONs found within the TM. Prussian blue did not stain materials in the saline-injected control eyes.

Appendix 1—figure 1

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The funders had no role in study design, data collection and interpretation, or the decision to submit the work for publication.

National Institutes of Health grant R01 EY030071 (CRE, SYE, MHK); The Georgia Research Alliance (CRE).

This study was performed in strict accordance with the recommendations in the Guide for the Care and Use of Laboratory Animals of the National Institutes of Health. All animal procedures were approved by the Georgia Tech Institutional Animal Care and Use Committee (approved protocol A100282) and performed in conformance with the ARVO Statement for the Use of Animals in Ophthalmic and Vision Research.

1. Preprint posted: May 15, 2024
2. Sent for peer review: October 8, 2024
3. Reviewed Preprint version 1: November 28, 2024
4. Reviewed Preprint version 2: May 7, 2025
5. Version of Record published: July 7, 2025

You can cite all versions using the DOI https://doi.org/10.7554/eLife.103256. This DOI represents all versions, and will always resolve to the latest one.

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