http://orcid.org/0000-0001-9045-0133
Figures
Abstract
Limited success achieved in translating basic science discoveries into clinical applications for chronic airway diseases is attributed to differences in respiratory anatomy and physiology, poor approximation of pathologic processes, and lack of correlative clinical endpoints between humans and laboratory animal models. Here, we discuss advantages of using ferrets (Mustela putorus furo) as a model for improved understanding of human airway physiology and demonstrate assays for quantifying airway epithelial ion transport in vivo and ex vivo, and establish air-liquid interface cultures of ferret airway epithelial cells as a complementary in vitro model for mechanistic studies. We present data here that establishes the feasibility of measuring these human disease endpoints in ferrets. Briefly, potential difference across the nasal and the lower airway epithelium in ferrets could be consistently assessed, were highly reproducible, and responsive to experimental interventions. Additionally, ferret airway epithelial cells were amenable to primary cell culture methods for in vitro experiments as was the use of ferret tracheal explants as an ex vivo system for assessing ion transport. The feasibility of conducting multiple assessments of disease outcomes supports the adoption of ferrets as a highly relevant model for research in obstructive airway diseases.
Citation: Kaza N, Raju SV, Cadillac JM, Trombley JA, Rasmussen L, Tang L, et al. (2017) Use of ferrets for electrophysiologic monitoring of ion transport. PLoS ONE 12(10): e0186984. https://doi.org/10.1371/journal.pone.0186984
Editor: Diego Alvarez de la Rosa, Universidad de la Laguna, SPAIN
Received: May 5, 2017; Accepted: October 11, 2017; Published: October 27, 2017
Copyright: © 2017 Kaza et al. This is an open access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Data Availability: All relevant data are within the paper and its supporting information files.
Funding: This work was supported by the National Institute of Diabetes and Digestive and Kidney Diseases, Grant P30 DK072482 (SMR), the National Heart, Lung, and Blood Institute grant 1R01 HL105487 (SMR),CFF R262 (SMR), American Lung Associationm, Grant RG-305752 (SVR), Flight Attendants Medical Research Association Grant, Grant YFA130008 (SVR). The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The laboratory is funded by Astra Zeneca, on projects unrelated to the present work. This does not alter our adherence to PloS One policies on sharing data and materials.
Introduction
Obstructive lung diseases such as cystic fibrosis (CF), chronic obstructive pulmonary disease (COPD), and asthma are characterized by a pronounced involvement of the airway epithelium [1]. These disorders collectively constitute a major cause of morbidity, mortality, and healthcare utilization [2], yet development of novel therapies to lessen disease burden is impeded by lack of animal models and techniques that are informative for elucidating disease biology, identifying new drug targets, and predicting the effect of drug candidates.
The search for better preclinical tools for obstructive lung disease has encouraged the development of higher-order mammals that have greater resemblance to humans than lower mammalian orders such as mice. Features important to model include the complex airway anatomy and prominent distribution of mucus-producing airway glands and goblet cells, which clearly impact epithelial function [3–5]. Indeed, while murine models of obstructive lung diseases have been useful for the identification of mechanisms related to inflammation, emphysema, fibrosis, and repair [6, 7], mice do not recapitulate some crucial features of airway diseases, like the development of spontaneous lung disease, which is a major limitation. Ion transport across the tracheal epithelium is an integral part of animal model characterization of airway diseases. One of the possible reasons murine models do not develop spontaneous chronic lung disease is the high expression of alternative cAMP-inducible chloride channels in the tracheal epithelium, unlike in higher order mammals like the ferret where CFTR is the primary cAMP-inducible chloride channel [8–10].
To improve translational utility, ferrets are proving advantageous. Recently, a CF ferret model was developed that exhibits features highly reminiscent of human lung disease and, if GI obstruction can be resolved by genetic or pharmacologic manipulation, could be highly informative due its size and utility for interventional studies [10, 11]. Ferrets are also commonly used to model viral infections of the respiratory system, which clearly impact epithelial function [12–14], and are amenable to complex research maneuvers to induce lung disease (i.e. cigarette smoke or other environmental exposures). For instance, ferrets have recently been demonstrated to generate chronic bronchitis, in addition to emphysema, upon cigarette smoke exposure, providing notable opportunities to examine the biology of COPD [15].
Despite the emerging strengths of ferrets in modeling airway disease, techniques to interrogate the epithelial biology of ferret airways have not yet been fully developed. As such, we have developed novel assays of airway electrophysiology in ferrets to investigate disease mechanisms relevant to obstructive airway disease research. In this manuscript, we demonstrate reliable conduct of transepithelial potential difference (PD) across the nasal and lower airway ferret epithelium as well as within-subject reproducibility of these measures, thus supporting further investigations using ferrets, including interventional studies. In addition, we describe and implement tissue culture methods for conducting air-liquid interface cultures (ALI) of ferret bronchial epithelial cells, which have potential utility for in vitro validation of physiologic mechanisms and for identifying pharmacologic and molecular agents, as have been successfully implemented in other species such as swine [16–18].
Methods
Animal welfare and approvals
This study was carried out in strict accordance with the recommendations in the Guide for the Care and Use of Laboratory Animals of the National Institutes of Health. The protocol was approved by the Institutional Animal Care and Use Committee (IACUC) of the University of Alabama at Birmingham (APN: 09681). All in vivo procedures were performed under anesthesia, and all efforts were made to minimize suffering. Ferrets were euthanized by exsanguination from cardiac puncture following an injection of ketamine and dexmedetomide at the end of the study to assure appropriate analgesia and anxiolysis.
Transepithelial nasal potential difference (NPD) measurement
Transepithelial NPD in ferrets was measured using an apparatus previously used in human studies (Fig 1) and following the standard operating procedure of the CF Therapeutics Development Network and the European Clinical Trial Network [19]. Hardware included a 4/30 PowerLab Analog-Digital Converter (AD Instruments, Colorado Springs, CO), BMA-200 AC/DC Bioamplifier (CWE, Ardmore, PA), ISO-Z isolation headstage for BMA-200 (CWE, Ardmore, PA), and a PC operating LabChart 7.0 software. PD was measured with Accumet miniature KCl calomel reference electrodes (Fisher Scientific, Cat. No:13-620-79) coupled with agar bridges to the nasal and subcutaneous compartments and to perfusion pumps to perfuse reagents into the nasal cavity (five in total, one for each drug infusion; WPI, Sarasota, FL). Other equipment included PE50 tubing and connectors (Braintree Scientific, Boston, Ma), an illuminating rhinoscope, heating pads, and disposables.
Cartoon representing hardware and electrical connections representing PD apparatus modified from the human instrument recommended by the standard operating procedure of the CF Therapeutics Development Network and the European Clinical Trial Network [19]. Ground Lead: Connects electrical apparatus to ground for reference from which voltage is measured. Headstage: Connects electrode inputs to bioamplifier and safely isolates from wall AC current. Bioamplifier: Serves as voltmeter to measure PD. Analog-Digital Converter: Converts analog signals to digital form. K/Cl Calomel Electrodes: Measure PD. Agar Bridge: Connects positively charged (+) calomel electrodes to ferret nasal epithelium or lower airway epithelium through Airway Catheter and negatively charged (-) calomel electrodes to subcutaneous tissue through Butterfly Needle. Syringe Pumps: Deliver test solutions perfused sequentially from pump 1 to 5 with a flow rate of 4ml/hr (see S1 Table). The PD changes are observed and recorded on the computer using LabChart 7.0 software. Following the procedure, the nasal cannula and subcutaneous needle were removed, and anesthesia reversed with atipamezole (5 mg/kg body weight, IM) delivered at an equal volume as dexmedetomidine. All ferrets recovered within 10–15 min, and remained on a warming pad until aroused and moving. Supplemental oxygen was not required during the NPD procedures in our experience, however supplemental oxygen was delivered during recovery from anesthesia.
Adult male and female ferrets weighing between 0.6–1.8 kg were anesthetized with a drug combination of dexmedetomidine (0.08–0.2 mg/kg, IM) and ketamine (2.5–5 mg/kg, IM), and then placed on a heated operating table until a deep state of anesthesia was reached. Once sedation was achieved, ophthalmic petroleum jelly was applied to the eyes to minimize drying. For NPD measurements, topical 2% lidocaine gel was applied to the outlet of the left nare to inhibit sneeze response, which is particularly prominent in ferrets even under deep sedation. With the injectable anesthetic combination, ferret respirations are not substantially depressed and do not require assisted ventilation, although supplemental oxygen via blow-by can be provided, if required.
Five minutes following lidocaine application, ferrets were sufficiently somnolent and the nasal outlet anesthetized to permit cannulation with a PE-90 cannula pulled to a tip diameter of 0.2 mm and inserted 6–9 mm into the left nostril, just lateral to the nasal septum (S1 Fig). The nasal cannula was connected to cathode electrode in 3 M KCl via an agarose bridge. An IV needle (30G) filled with 1% agarose in 150 mM NaCl solution was placed under the skin and connected to anode electrode in 3 M KCl solution to close the measuring circuit (Fig 1). Following acquisition of a viable baseline potential with Ringer’s USP, test solutions were perfused serially to measure the change in PD attributable to sodium transport through epithelial sodium channel (ENaC) and chloride transport through cystic fibrosis transmembrane conductance regulator (CFTR). Details of each solution and its composition are described in S1 Table. The perfusion pumps were set up in the same sequence as listed in S1 Table and were operated in numerical order. The solutions were dispensed from a 1 mL Becton Dickson syringe and each drug was perfused at a steady flow rate of 4 ml/hr for at least five minutes or until a stable signal was achieved.
Lower airway potential difference (LAPD) measurement
Ferrets were sedated as described above. Following the application of the eye ointment, ferrets were intubated using a laryngoscope and a 4.3mm O.D Mallinckrodt oral/nasal uncuffed endotracheal tube (Covidien, Mansfield, MA). After confirming the position of the endotracheal tube by using a Nellcor pediatric colorimetric CO2 detector (Covidien, MA), a PE-60 cannula was inserted into the tube lumen until it passed through the tube end and contacted the epithelial lining of the lower airway. Like for NPD, the measuring circuit was assessed with a subcutaneous anode. Changes in PD were measured using the NPD protocol. Like the NPD protocol, LAPD procedures did not pose serious safety threats even with repeated conduct. All animals that underwent the procedure survived, with 100% recovery from the anesthetic regimen.
Primary culture of ferret airway epithelial cells
Ferret airway epithelial cells were grown as primary cultures following techniques used in primary culture of human airway epithelial cells [20, 21]. Airway epithelial cells were dissociated from the trachea, grown at ALI, and used in short-circuit current (Isc) experiments after terminal differentiation. Briefly, trachea was excised from a euthanized ferret and debrided immediately following excision. Trachea were then washed twice in Minimum Essential Media (MEM) containing 0.5 mg/ml DTT (Sigma-Aldrich, St. Louis, MO) and 25 U/ml DNAse I (Roche, Basel, Switzerland). Following the washes, trachea was placed in dissociation media containing MEM, 2.5 U/ml DNAse I, 100 μg/ml ceftazidime, 80 μg/ml tobramycin, 1.25 μg/ml amphotericin B, and 4.4 U/ml pronase (Sigma-Aldrich) for 24–36 h at 4°C. Loosened airway epithelial cells were then expanded in growth media containing BEGM (LONZA, Basel, Switzerland) supplemented with an additional 10 nM all trans-retinoic acid (Sigma-Aldrich) every 24 h. Once cells were 80–90% confluent, they were seeded on Snapwell 1.13 cm2 permeable supports (1×106cells/filter; Bayer, Pittsburgh, PN) or Costar 0.4 μm permeable supports (5×105 cells/filter; Bethesda, MD) after coating with NIH 3T3 fibroblast-conditioned media, and grown in differentiating media containing DMEM/F12 (Invitrogen, Carlsbad, California), 2% Ultroser-G (Pall, New York, NY), 2% Fetal Clone II (Hyclone, Logan, UT), 2.5 μg/ml Insulin (Sigma-Aldrich), 0.25% bovine brain extract (LONZA), 20 nM hydrocortisone (Sigma-Aldrich), 500 nM Triodothyronine (Sigma-Aldrich), 2.5 μg/ml transferrin (Invitrogen), 250 nM ethanolamine (Sigma-Aldrich), 1.5 μM epinephrine (Sigma-Aldrich), 250 nM phosphoetheanolamine (Sigma-Aldrich), and 10 nM all trans-retinoic acid until terminally differentiated. Only first and second passage cell cultures with transepithelial electrical resistance (TEER) of more than 100 ohms/cm2 were considered for electrophysiological studies. Cells were fixed with standard histologic techniques for microscopy [12].
Short-circuit current measurements on cultured primary ferret bronchial epithelial cells and ex vivo ferret trachea
Short-circuit current (Isc) was measured under voltage clamp conditions using MC8 clamps and P2300 Ussing chambers (Physiologic Instruments, San Diego, CA). ALI monolayers were initially bathed on both sides with identical Ringer’s solutions containing (in mM) 115 NaCl, 25 NaHCO3, 2.4 KH2PO4, 1.24 K2HPO4, 1.2 CaCl2, 1.2 MgCl2, and 10 D-glucose (pH 7.4). Bath solutions were vigorously stirred and gassed with 95%O2∶5% CO2. Isc was obtained using an epithelial voltage clamp (Physiologic Instruments). A one-second three-mV pulse was imposed every 10 seconds to monitor resistance calculated using Ohm’s law. Where indicated, the mucosal bathing solution was changed to a low Cl− solution containing 1.2 NaCl and 115 Na+ gluconate, and all other components as above. This was followed by the CFTR agonist forskolin as indicated with minimum five-min observation at each concentration. GlyH101 (20 μM final concentration) was added to the mucosal bathing solution at the end of experiments to block CFTR-dependent Isc. All chambers were maintained at 37°C.
Tracheal Isc studies to assess ion transport across the epithelium were conducted on freshly harvested trachea from euthanized ferrets. Isc measurements in ferret airway explants were conducted following dissection of the mucosal layer and were performed as in ALI monolayers, except for use of P2307 tissue mounts. Amiloride (100 μM) was added to block residual Na+ current and was followed by a low Cl− solution containing 1.2 NaCl and 115 Na+ gluconate. The CFTR agonist forskolin and antagonist GlyH101 were added to the mucosal bathing solution, where indicated, to respectively activate and thereafter block CFTR-dependent Isc.
Statistics
Descriptive statistics (mean, SD, and SEM) were compared using 2-sided Student’s ttest or 2-way ANOVA, as appropriate. Post-hoc tests for multiple comparisons following ANOVA were calculated using Fisher’s least significant difference only if ANOVA was significant. All statistical tests were 2-sided and were performed at a 5% significance level (i.e., α = 0.05) using GraphPad Prism software. Error bars designate SEM unless indicated otherwise.
Results
Transepithelial NPD tracings in ferrets resemble human tracings
NPD is the voltage across the nasal epithelium, representing the sum of the membrane potentials of the outer epithelial membrane. NPD can be used to evaluate ion transport in vivo, including the contributions of CFTR and ENaC, and thus is a particularly valuable tool for diagnosis and assessment of CF and other airway diseases characterized by chloride and sodium ion transport defects [22]. Notably, previous studies in animals and humans indicate that PD measurements across the nasal epithelium are generally reflective of the PD of the lower airway epithelium [23, 24].
To establish techniques to measure airway electrophysiology in ferrets, we developed and tested a modified method to assess ferret NPD. Fig 2A depicts a representative ferret NPD tracing, which demonstrates all the classical features of tracings observed in humans, including 1) a stable baseline PD that is inhibited by amiloride perfusion; 2) the subsequent hyperpolarization of the membrane upon sequential perfusion with chloride-free Ringers solution and chloride-free Ringers plus forskolin; and 3) partial (i.e. incomplete) blockade of CFTR-dependent hyperpolarization by the CFTR inhibitor GlyH101. These features held when PD measurements were averaged across all ferrets tested (Fig 2B). The average change in epithelial PD (ΔPD) (mean ± SD) with the addition of chloride-free Ringers plus forskolin (Δchloride-free forskolin),representative of the change in CFTR-dependent chloride transport,in ferrets was -13.7 ± 2 mV, while in healthy humans it is in the -29 ±10 mV range (22); other ΔPD measurements from the same ferrets are shown in Fig 2C and Table 1. ΔGlyH101 was 7.0 ± 3.9 mV, and indicated specificity of ΔPD as a metric of CFTR function. The change in PD upon amiloride perfusion, which signifies the change in ENaC-mediated epithelial sodium transport, was 3.5 ± 1.9 mV, and is comparably diminished in magnitude as compared to human values 13 ± 4 mV [22].
A: Representative NPD tracing in ferrets using the apparatus described in Fig 1. Under deep sedation, PD changes following perfusion with Ringer’s solution, Ringer’s solution with amiloride (100 μM), chloride-free solution, chloride-free with forskolin (20 μM), and chloride-free with CFTR-specific inhibitor GlyH101 (10 μM). B: Summary tracing of mean PD measurements (mean ± SEM) in ferrets following infusion of these 5 sequential reagents, N = 7. Ion channel activity of CFTR is quantified by PD changes in response to chloride-free + forskolin or by GlyH101 inhibitor. Similarly, ENaC activity is attributed to PD changes following amiloride treatment. C: Change in NPD (ΔPD) measurements from the same cohort of male and female adult, wild type ferrets plotted as individual measurements. D: Summary tracing of PD measurements (mean ±SEM) in male and female, adult, wild type ferrets acquired at two different times to validate reproducibility, N = 7. No discernable differences in ENaC or CFTR activity were found over 7 weeks. E: PD measurements of each animal subject plotted individually for each perfusate at two time points conducted 7 weeks apart.
Importantly, ion transport measurements were repeatable (Fig 2D and 2E, and Table 2); the within subject repeatability of Δchloride-free froskolin was 0.3 ± 5.3 [mean ± SD], with no serious safety concerns. The anesthetic regimen achieved 100% recovery following multiple sessions of sedation, and multiple ferrets have been successfully evaluated during repeated sessions conducted as few as three days apart, permitting longitudinal analyses over the course of chronic studies. Together, these data indicate that NPD tracings in ferrets are similar to those seen in humans, and can be reliably and safely measured in a repeatable fashion.
Sensitivity of ferret NPD to pharmacological intervention
The ability to repeatedly assess NPD in the same animal enabled the calculation of sample sizes required for evaluating a significant difference in PD measurements in an experimental cohort of animals (Table 3). Sample sizes for detecting within-subject changes in PD are quite feasible for reasonable effect magnitudes.
As a proof of concept for demonstrating a within-ferret change in PD upon an intervention, we tested the sensitivity of NPD as a readout of diminished CFTR function, measuring PD 30 min following intranasal instillation with GlyH101 (10 μM) as compared to intranasal vehicle control (DMSO, 0.001%) in ferrets (N = 4). Results indicated that NPD was sensitive to inhibition; as the primary measure of CFTR activity, Δchloride-free forskolin, was significantly diminished (Fig 3A and 3B). All ferrets recovered following acute administration of GlyH101 and were adequately tolerant of repeat analyses.
A: Representative NPD tracing in ferrets one hour after acute intranasal administration with either vehicle (DMSO 0.001% in saline) or CFTR-specific inhibitor GlyH101 (10μM). B: Summary of CFTR-dependent PD differences in vehicle and GlyH101-treated ferrets. N = 4, * P<0.05.
Lower airway potential difference (LAPD) measurements in ferrets
PD measurements across the epithelial membrane in the lower airway provide a measure of the ion transport of the lung, and are potentially useful to evaluate inhaled interventions. Therefore, we developed a protocol to assess LAPD in ferrets, as this measure may be more informative than NPD for testing of therapies delivered specifically to the lungs [25, 26]. The representative ferret LAPD tracing (Fig 4A) and summary data (Fig 4B) demonstrate expected changes in PD upon sequential perfusion of test solutions. Average LAPD Δchloride-free froskolin was -11.0 ± 4.6 mV, and other PD measures (Fig 4C, Table 4) were also consistent with NPD, reflective of the similarities between the two outcome measures.
A. Representative LAPD tracing in a sedated intubated ferret indicating PD changes following perfusion with Ringer’s solution, amiloride (100 μM), chloride-free, chloride-free + forskolin (20 μM), and CFTR-specific inhibitor GlyH101 (10 μM); N = 5. B: Summary tracing of PD changes in ferrets following infusion of the 5 sequential reagents, N = 5. C: Change in LAPD measurements from 5 (male and female) adult, wild type ferrets.
ALI cultures of ferret airway epithelial cells provide a comparable in vitro model system to ex vivo tracheal tissue for electrophysiologic studies
Asymmetric distribution of proteins on polarized epithelium renders the apical properties of these cells distinctly different from their basolateral properties. Primary human airway epithelial cells grown on semi-permeable filters at ALI have been used extensively as a physiologically relevant in vitro model system [27]. To extend the advantages of ALI cultures to the ferret model, we isolated tracheobronchial epithelia from ferret trachea and investigated their eletrophysiological responses. We estimate over 1 x 108 cells are available from a single ferret trachea prep, based on an area of 39 cm2 for a ferret trachea of 15 cm length & cell density comparable to that observed in ALI cultures. On histology, ALI cultures of ferret bronchial epithelial cells resembled primary human airway epithelial cells (Fig 5A). We tested CFTR activation with low chloride forskolin (10 μM), in the presence of amiloride (100 μM) to block ENaC channels, followed by CFTR inhibition with GlyH101 (20 μM). As shown in representative Isc tracing, increased anion transport occurred with addition of forskolin, which was immediately followed by CFTR inhibition with GlyH101, indicating CFTR specificity (Fig 5B). Summary data (Fig 5C) shows a mean Δforskolin Isc of 4.9 (± 1.6) μA/cm2 and a mean ΔGlyH101 Isc of -5.0 (± 2.6) μA/cm2.
A: Representative hematoxylin and eosin stained image of a well-differentiated ferret bronchial epithelial cells grown at air-liquid interface. B: Representative Isc tracings of primary ferret bronchial epithelial cells sequentially exposed to forskolin (10 μM), followed by GlyH101 (20 μM) in the setting of amiloride (100 μM) and a chloride secretory gradient. C: Summary data of Isc measurements from different ALI cultures indicating stimulated Isc following acute addition of forskolin or GlyH101. N = 4/condition. D: Representative Isc tracing of an ex vivo ferret trachea sequentially exposed to Ringer’s, chloride-free, forskolin (20 μM), followed by GlyH101 (20 μM) in the setting of amiloride (100 μM). E: Summary data of Isc measurements from different trachea showing stimulated Isc following acute addition of amiloride, forskolin, or GlyH101. N = 7/condition.
To evaluate the findings in comparison to native tissue, we tested whether the same response was also observed in excised ferret airway explants. As seen in ferret ALI monolayers, ferret tracheal Isc tracings showed acute CFTR activation with both low chloride and forskolin as well as significant inhibition with GlyH101 (Fig 5D); summary dot showed stimulus with forskolin produced a mean ΔIsc of 240.4(± 34.6 μA/cm2 and GlyH101 induced a mean reduction of -391.4 ± 69.46 μA/cm2 (Fig 5E). Overall, these data demonstrate that ferret ALI cultures successfully recapitulate characteristics and functions comparable to in vivo and ex vivo systems.
Discussion
Here we demonstrate multiple methods for conducting electrophysiologic studies of the airway epithelium of ferrets, a species of increasing importance in airway biology research. First, we establish a method for measuring nasal transepithelial PD—including the within-subject repeatability of the measurements—enabling estimation of ENaC, CFTR, and alternative chloride channel activity. A particular strength of the technique established here is that the methods are almost identical to those performed in humans, and include the advantages of a non-perfusion catheter, allowing for suitable translation [19, 28]. Sample size estimates suggest that a reasonable number of animals are required to detect meaningful changes in CFTR-dependent PD with an intervention or treatment, allowing for appropriately powered studies. Using these principles, we validate this concept showing blockade of CFTR activity upon nasal instillation of the CFTR inhibitor GlyH101. Overall findings suggest that it will be feasible to test for an electrophysiological effect in ferrets in vivo, such as the noxious effects of inhalational exposures, or the pharmacological benefit manifest by novel small molecules that activate ion channels [15]. They also render it possible to screen molecular reagents (e.g antibodies) and pharmacologic entities for their use in in-vivo studies with ferrets.
In a related effort, we also extend transepithelial PD measurements to the lower airway of ferrets, and demonstrate feasibility of the technique in sedated ferrets. Just as our laboratory and others have measured PD in the lungs of patients with CF or COPD [24, 25], we used a similar method to measure ferret LAPD. Although blinded placement of the catheter was required, the long trachea of ferrets provide reasonable assurance of position by measurement of the catheter, where we found consistent values between animals. As expected and observed in humans, the amiloride- and forskolin-sensitive PD in the lung was slightly lower than in the nose, probably reflective of channel density [29]. LAPD measurements may be particularly useful for agents that are administered directly to the lungs, where the nose may not serve as an appropriate proxy. For example, the effect of viral infections, intra-tracheally delivered gene therapy vectors, or inhalational molecules that target the lower airways for delivery all may be better served by evaluation of LAPD, as compared to NPD [25, 26]. Parallel efforts analyzing the electrophysiology of ferret tracheal explants confirmed PD findings, and provide a means to substantiate in vivo effects using PD with more definitive Isc results.
To enable in vitro analysis of electrophysiological mechanisms that cannot be replicated in-vivo, or is more efficient to test ex vivo, we report a method to grow differentiated ferret airway epithelia at ALI, and then measure ion transport activity using modified Ussing chambers. Evaluation of primary bronchial epithelial cells in parallel to tissue samples and in vivo studies has proven a powerful means to establish novel mechanisms and in vivo relevance in CF pigs [16–18], and the methods shown here should be suitable for similar studies of this sort. While a variety of techniques can be used to encourage terminal differentiation of airway epithelial cells in a manner that allows the measurement of vectoral ion transport [30, 31], we focused these initial studies using culture methods frequently reported in the literature for humans and other species [32]; further refinements unique to ferrets may be beneficial to explore in the future. This may be particularly important for evaluating differences in ENaC expression (e.g. alpha, beta, gamma, delta channel subunits) or function, which can vary by species with respect to altered CFTR function [33]. Whether differences in ATP12A expression and function, which has been shown to be crucial for airway acidification in humans and pigs but absent in mice, is another relevant question [17].
Establishing techniques for the study of ferrets may be particularly beneficial for aspects of airway disease that are not represented in mice. For example, even for a monogenetic disease such as CF, mouse models developed by knocking out the causative gene CFTR across a variety of genetic backgrounds failed to recapitulate spontaneous lung disease [34]. Similarly, mouse models of COPD, including those generated by exposing to cigarette smoke and/or exogenous protease administration or introducing genetic deficiencies in anti-proteases, develop emphysematous small airway enlargement, but exhibit minimal alterations in the other pathologic features, especially in conducting airways [35]. Additionally, this study along with previous studies of ion transport in ferrets will help develop more suitable avenues to investigate to specific pathological processes which are more demonstrable in the ferret model of airway disease [36, 37]. Many of the airway disorders have the potential to benefit from a high-order mammal which more faithfully recapitulates human disease, and may be impacted by changes in ion transport. Our hope is that establishing the assays presented here will help enable research of this sort, advancing our understanding of these common and important conditions.
Supporting information
S1 Fig. CT scan of a ferret head.
Sagittal reconstructed CT scan image of a ferret head showing the location for the placement of the nasal cannula for measuring nasal potential difference in ferrets.
https://doi.org/10.1371/journal.pone.0186984.s001
(TIFF)
S1 Table. Solutions for potential difference measurements.
Solutions used in the measurement of potential difference listed in the sequential order in which they are perfused.
https://doi.org/10.1371/journal.pone.0186984.s002
(DOCX)
Acknowledgments
The authors appreciate the assistance of Ms. Denise Stanford for preparing a saggital CT image of a ferret. Editorial assistance was also provided by Dr. Emily Falk Libby.
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