Painless, rapid, controlled, minimally invasive molecular transport across human skin for drug delivery and analyte acquisition is of widespread interest. Creation of microconduits through the stratum corneum and epidermis is achieved by stochastic scissioning events localized to typically 250 μm diameter areas of human skin in vivo.
Microscissioning is achieved by a limited flux of accelerated gas: 25 μm inert particles passing through the aperture in a mask held against the stratum corneum. The particles scize (cut) tissue, which is removed by the gas flow with the sensation of a gentle stream of air against the skin. The resulting microconduit is fully open and may be between 50 and 200 μm deep.
In vivo adult human tests show that microconduits reduce the electrical impedance between two ECG electrodes from approximately 4,000 Ω to 500 Ω. Drug delivery has been demonstrated in vivo by applying lidocaine to a microconduit from a cotton swab. Sharp point probing demonstrated full anaesthesia around the site within three minutes. Topical application without the microconduit required approximately 1.5 hours. Approximately 180 μm deep microconduits in vivo yielded blood sample volumes of several μl, with a faint pricking sensation as blood enters tissue. Blood glucose measurements were taken with two commercial monitoring systems. Microconduits are invisible to the unaided eye, developing a slight erythematous macule that disappears over days.
Microscissioned microconduits may provide a minimally invasive basis for delivery of any size molecule, and for extraction of interstitial fluid and blood samples. Such microconduits reduce through-skin electrical impedance, have controllable diameter and depth, are fully open and, after healing, no foreign bodies were visible using through-skin confocal microscopy. In subjects to date, microscissioning is painless and rapid.
Convenient, cost effective medical technology is needed to provide better care at lower cost. Minimally invasive technologies that meet present and future medical needs are extremely desirable. There is, for example, a recognized need for improved diabetes treatment [1,2]. With this in mind, minimally invasive transdermal drug delivery and analyte sampling are of long-standing interest.
Molecular transport through the skin is fundamentally limited by the skin's barrier function [3,4]. This has motivated the investigation of active molecular and ionic transport through relatively unperturbed skin by diffusion  and electrical current (iontophoresis) [6-8]. Other approaches alter the barrier function by using high voltage pulses (electroporation) , stress waves , or by interventions creating relatively large openings or defects in the stratum corneum. The latter include cavitation by ultrasound [11,12], laser drilled openings  and chemically-enhanced electroporation . Microneedles and other sharp devices have also been proposed [15,16]. Of the many techniques investigated, only the hypodermic needle has met the major needs. However, needle introduction is often painful.
An alternative means of avoiding these problems is to create one or more small holes (microconduits) through the stratum corneum and underlying tissues (Figures 1 and 2). Techniques using a combination of momentum transfer and scizing are well known in cosmetic dermatology. The relatively hard, roughened stratum corneum and epidermis resulting from aging processes can be removed by moderate velocity, sharp particles impinging obliquely against the skin surface. The hypodermic needle cuts the tissue and holds it open. Upon needle removal, the tissues essentially close the opening. In contrast, microscission can rapidly and painlessly produce small, open microconduits by means of a gas-entrained stream of inert, sharp particles on a defined skin area (Figure 3). We report here on the use of scission through a mask to painlessly produce microconduits in the skin as well as proof-of-concept drug introduction into and analyte extraction from the human body.
Here we describe the exploratory use of sharp particles, combined with masking techniques, to define small areas of the skin to be scized. Preliminary experiments were performed using an unmodified Airbrasive Model K, Series II (S.S. White Mfg. Co, Trenton, NJ, USA). Microscopic comparison of various particulates led to the selection of Aluminum Oxide Al-602 (Atlantic Equipment Engineers, Bergenfield, NJ, USA). These fell in the range of 10 μm to 70 μm, with a high percentage of irregular, sharp particles (Figure 4). Parameters such as particle size, shape, velocity, flux, carrier gas pressure and nozzle-mask spacing were varied to investigate their effects on the removal rate of the stratum corneum and underlying epidermis and dermis.
Figure 4. Al2O3 scizing particulate (marked width upper center = 35 μm).
A 75 μm thick Teflon mask with one or four holes with a specified diameter and center-to-center distance was used to constrain the area of the skin exposed to the abrasive particles. The mask was mounted on a holder with provision to position the gas nozzle directly above the mask (Figure 5, left and right). The mask with a single 200 μm diameter opening, a 450 μm diameter nozzle and a nozzle to mask spacing of 1,500 μm was used. The particles in a nitrogen stream under a pressure of 552 kPa was directed toward a site on the inner left wrist, 10 cm back from the center of the palm (Figure 6) of an adult subject. The proof-of-concept results presented in this paper are based on experiments on the research team's principal investigators. The protocol was approved by the Committee on the Use of Humans as Experimental Subjects at MIT. If the mask was held tightly against the skin, the stratum corneum, epidermis and dermis were removed to the capillary level in 20 seconds (Table 1). Blood was clearly visible in the 200 μm diameter microconduit, suggesting a depth of 100–150 μm. This result led to parameter optimization in five areas.
Figure 5. Mask holder and nozzle fixture: Left: Mask/nozzle holder and wrist fixture; Right: Close up of 4-hole mask and nozzles.
Figure 6. Microscissioning arrangement: Forearm with attaching strap, mask holder, nozzle, electrical connections to holder and ECG electrode.
Table 1. Microconduit depth and electrical resistance versus scission time.
1. Scizing depends on an optimum incoming particle flux, related to the mask opening diameter. Lower and higher fluxes reduce scizing rates. Excess particles per unit time tend to clog the mask opening and cause particle trapping between the mask and stratum corneum. At this limit, excess particles impede the entry and exit of particles, slowing the scizing process. The particle generator has a pressurized particle reservoir, the bottom of which is separated from the carrier gas path by a thin aperture plate with holes in it. This system is vibrated by an electrical solenoid with motion amplitude control to provide controlled delivery of microparticles into the gas stream. This arrangement was modified by replacing the eight, 500 μm diameter holes with a single 325 μm diameter opening, giving a particle flux that produced a peak scission rate near the maximum shake amplitude.
2. High gas pressure deflected the stratum corneum away from the mask, causing particle trapping and poor microconduit definition due to loss of particulate collimation. Experiments on test polyethylene substrates that are 'soft' and on human skin in vivo showed the scission rate to be the same at 103 to 172 kPa as at 552 kPa.
3. The particle flux was initially observed to vary significantly due to the reservoir shake solenoid, synchronized with valving in the gas stream creating large pressure pulses. This variability was greatly decreased by removing all gas flow controls and externally actuating the reservoir vibration solenoid. A voltmeter was installed in the shake solenoid to permit accurate shake amplitude repeatability. After the gas pressure is turned on and flow established for ten seconds, the shake solenoid is energized. This sequence is reversed to turn the system off. A full cycle particle flux variation of 4% is achieved, with the flux during scission constant to within 2%.
4. Carbide nozzles (S.S. White Mfg. Co, Trenton, NJ, USA) with aperture diameters of either 275 μm or 450 μm were used. Smaller diameters clogged, and larger diameters produced excessively large flux diameters at the mask surface for the single or four hole masks used throughout. A nozzle to mask spacing of 750–850 μm produces a 3,800 μm diameter flux cone. This exposes the surface of the stratum corneum to approximately 350–500 particles per second through each 150 μm diameter hole in the one or four opening masks at a shake voltage of 74 V and nitrogen gas pressure of 138 kPa. These parameters give a scizing rate of approximately 10–15 μm per second on the stratum corneum of adult subjects who participated in the in vivo trials. The mask holder with the four nozzle array below it is shown (Figure 5, left). The mask is cut to extend beyond the circular ring that presses it against the stratum corneum. The square hole that rigidly fixes the nozzle location in three axes is above it. The rectangular arm extending left acts as a bridge over which a strap around the wrist pulls the holder against the wrist. At the left end is a square, electrically insulating plate that acts as a stabilizing fulcrum. The four-hole mask (Figure 5, right) is seen from the stratum corneum side, backed by a thin metal plate with a hole having a 100 μm ridge around its edge that presses the mask against the stratum corneum. Three nozzles are just visible through the mask.
5. Polyimide film – a hard, electrically insulating, high temperature polymer – was used for scission rate testing and as a mask material. It exhibited the same resistance to mask thinning by impinging particles as teflon, which scize less rapidly than glass or stainless steel. Polyimide can be shaped readily by laser ablation, drilling, chemical or plasma etching, lending itself to low cost, mass produced single-use masks. Polyimide mask life time is 60–90 seconds, equivalent to opening five to eight microconduits 150 μm deep, providing ample margin for a single scizing operation. Beyond this life time, the masking holes in polyimide increase in size by extended abrasion.
Results and discussion
Scized microconduits in vivo
Attempts to do in vitro testing were abandoned when properties of human cadaver skin were found to be quite different from in vivo skin. There was considerable sample-to-sample variability in the stratum corneum thickness and the skin impedance in human cadaver skin prior to microscissioning. The variability may have been caused by the preservation techniques, length of time between death and skin harvest and the site of skin on the body. Superficial mechanical state of the skin varied from tough to near-disintegration among samples. As the wide range of possible applications became apparent, a decision was made to demonstrate proofs-of-concept only. Reliable demonstration of drug delivery (lidocaine), analyte sampling (blood glucose) and even electrical impedance measurement were not possible with in vitro testing.
All in vivo results are from experiments done on two adult subjects. We sterilized the aluminum oxide particulate and masks by heating to 200°C for one hour. Nozzles, hoses and the particle reservoir were rinsed in methanol. Sterile gloves were worn and the target areas swabbed with ethanol. Sterile saline solution was used for electrical tests with syringes and needles for handling saline being rinsed with methanol, and nitrogen dried prior to use.
The depth of scized microconduits can be determined approximately by measuring the electrical impedance between an ECG electrode on the subject's unperturbed skin and the mask holding fixture (Figure 6). A SR715 LCR meter (Stanford Research, Sunnyvale, CA, USA) operating at 1 V and 1 kHz was used. The metal mask holder was electrically connected to the microconduit by normal saline placed in the ring to which the mask was bonded. Since the mask was held tight against the skin, the saline did not leak between the mask and skin, thus providing electrical continuity with the microconduit. Typical microconduits generated with a four nozzle, four hole mask are shown (Figure 7, left and right). The data (Table 1) are averages of approximately 100 experiments on two subjects. Microconduit depths were measured using the Vivascope 1000 (Lucid, Rochester, NY, USA), an in vivo near-infrared reflectance-mode confocal microscope, with an illumination wavelength of 830 nm, 30 mW power and a 30 ×, 0.9 N.A. water immersion objective providing a viewing depth of 200 μm. The instrument captures images with a spatial resolution of 0.5 to 1.0 μm in the lateral dimension and 3 to 5 μm in the axial dimension. Further details of this system have been reported recently . Standard particle generator parameters were used, that is, N2 under 138 kPa pressure, reservoir drive of 80 V, 450 μm nozzle diameter.
Figure 7. In vivo microconduits: Four 150 μm microconduits on 450 μm centers with abrasive particles present in the microconduits (left) and with particles removed from the microconduits (right).
Microconduit profiles are revealed by infrared confocal microscopy (Figure 8). Microconduits made with a four hole mask and a scission time of 20 seconds are shown on the left. The white lines are an electron microscope grid placed on the skin to provide high contrast for focusing. The 160 μm diameter openings are nearly uniform, with the upper right one corresponding to the upper left image in the confocal views. The confocal images at nine depths clearly illustrate that the microconduit is fully open throughout its depth of approximately 165 μm (lower right image). At its bottom, the diameter is approximately 65 μm.
Figure 8. Depth profile of a microconduit: Top: Confocal skin surface view of four 160 μm diameter microconduit openings in vivo in human stratum corneum. Bottom: Cross-section of lower right microconduit (blue arrow) with increasing depth obtained by in vivo confocal microscopy.
Usually there are no residual Al2O3 microparticles, which are easy to see as bright 30 micrometer particles at full depth. In some cases, up to about ten microparticles were observed. However, a deionized water rinse from a hypodermic needle at low pressure is effective in removing particles. In cases where particles were seen and left, they were not visible in the confocal microscope at the site after full healing. This suggests they were moved out by the healing process, but has not been confirmed by other methods.
Transdermal electrical impedance reduction
Removal of the high electrical resistance stratum corneum takes place during the initial few seconds of scizing a microconduit. If stopped, then scizing is a fast, simple, totally sensation-free method for reducing the electrical impedance through the skin. At 1 kHz and 1V, the impedance between two electrocardiogram electrodes (Type 510–005, Lynn Medical, MI, USA) is approximately 4 kΩ. Placing two of the same type of electrocardiogram electrodes over two 200 μm diameter shallow microconduits reduces the impedance to 500 Ω, measured under the same conditions. This implies that the 1 kHz impedance associated with a single microconduit is only 250 Ω, and, therefore, four microconduits can provide a local skin resistance of the order of 100 Ω each.
Assessment of microconduit efficacy for delivering a drug into the dermis and epidermis was carried out using the topical anaesthetic, lidocaine. The presence of lidocaine was evaluated by using non-scarring pulses from a 585 nm pulsed-dye laser, employed as a pain inducer . Also, the 'pin stick' on skin around the microconduit tests for sensation was used to map lateral anesthesized distance from the microconduit. Masks with four 160 μm diameter holes on 450 μm centers were used. Testing was done on the inner, left wrist, approximately 10 cm away from the palm center.
The first test determined lidocaine uptake and level of anesthesia. After scission for 7 seconds, a subject reported a barely perceptible 'pricking' sensation. The microconduits had an impedance of 23 kΩ, implying a depth of 140 μm. A slight discharge of clear fluid was evident. Both the microconduit and control sites were exposed to a 50% lidocaine solution (5 gm lidocaine hydrochloride in 5 ml normal saline) in saturated filter paper pads with Finn chambers taped over each. In prior studies, we used 40% and 50% lidocaine solution and found that the subjective degree of anesthesia was easily quantifiable by the subjects enrolled in those studies, so we selected 50% lidocaine concentration for this proof-of-concept demonstration . These two sites were exposed to a lidocaine 'soak' for 5 minutes. A third 'normal' control site, receiving no lidocaine exposure, was marked and tested. These sites were separated by 5–6 cm. Sensation testing was done with a Coherent Palomar (Burlington, MA, USA) Light Sheer Laser emitting a 30 ms, 35 mJ pulse. The sites were lazed randomly three to five times each, with and without power on, while the subject's arm was extended and the subject looked away. The subject verbally reported sensation effects. The testing was carried out 15, 30 and 75 minutes after lidocaine exposure (Tables 2 and 3). The sensation data strongly suggest that the area around microconduits was anesthetized.
Table 2. Efficacy of lidocaine delivery to tissues through four microconduits.
Table 3. Efficacy of lidocaine delivery to tissues through one microconduit.
A number of additional tests were done using the 'pin stick' test for sensation, to determine the minimum time for full anaesthetic effect. Most testing was done on one subject, with verification tests done on two other subjects. These tests were done on a single 160 μm diameter microconduit, 100–150 μm deep on the left inner wrist. Using 50% lidocaine saturated cotton pads as the anesthetic source, anesthesia of a control area without a microconduit required 60–90 minutes. Anesthesia became discernable (sensation diminishes perceptibly) after 1 minute. Maximum anesthetic effect and anesthetized radius occurred between 2.5 and 3.5 minutes. The anesthetized radius was 1,800–2,200 μm. When the lidocaine was applied to the microconduit under a pressure of 30 inches of water, the full anesthetic effect occurred in 1.5–2 minutes and the anesthetized radius increased to 2,800–3,000 μm.
The onset of anesthesia takes longer in microconduits deep enough to yield blood than in shallower, non-blood producing microconduits. Possibly the blood outflow impedes inflow of the externally-applied lidocaine to the sub-stratum corneum tissues, or the clotting blood partially obstructs the microconduit.
Analyte extraction and analysis
Experiments involving creation of deep microconduits provided blood samples for glucose testing and assessment of the sensation (pain) level involved. Testing was carried out with a FastTake glucose monitor (Lifescan, Milpitas, CA, USA). The instrument's disposable test strips required a minimum blood volume of 1.5 μl.
These experiments involved one subject using a subjective pain sensation scale of one to ten ('none' to 'sharp'). The test site was always on the side of the left hand fourth finger or the left hand middle finger between the finger end and outer joint. The standard mask-nozzle-generator conditions were used. Opening a microconduit to the blood capillary level consistently took 14–18 seconds. Within 3–6 seconds after removing the scizing device, 1–3 μl of blood formed in a drop (Figure 9, left and right). The FastTake test strip end was held against the drop and a sample was drawn into the sensing chamber by capillary action. Results are summarized (Table 4) comparing accessing blood with the Penlet II Automatic Blood Sampler (a lancet system supplied with the FastTake instrument) and through microconduits made by scizing. The tests were done two days apart, with the two lancet tests first, followed by the scizing tests. Time for the lancet test is zero due to its rapid plunge in/withdraw action. Times for scizing were intentionally varied slightly to test sensation and blood flow effects. The glucose readings were all in a 'normal' range. These experiments show that scized microconduits may provide painless acquisition of samples for established blood glucose tests.
The formation of microconduits in vivo through human stratum corneum, epidermis and dermis, has been demonstrated painlessly and with little or no detectable sensation. These 100–250 μm diameter, 200 μm deep openings are made repeatedly, quickly and painlessly through sharp, inert particles microscissioning the tissues. Accurate control of particle size, flux, carrier gas pressure, area exposed to particles, and time of exposure is essential. Microconduit diameter and depth can be controlled; no foreign bodies were discernable after healing. In vivo through-skin drug delivery, analyte access and significantly reduced electrocardiogram electrical impedance have been demonstrated.
List of abbreviations
N.A., numerical aperture.
JCW, RRA and TOH developed the basic concept. TOH designed and built several experimental microscissioning apparatuses, and carried out the experiments with assistance from TRG, SG and JCW and guidance from RRA. TRG carried out the microscopy and analyzed the images. SG designed and conducted the sensation experiments. TOH, JCW and TRG prepared the manuscript. All authors read and approved the final manuscript.
The authors are grateful to Rieko Tachihara and Milind Rajadhyaksha of the M.G.H Wellman Laboratory of Photomedicine, Department of Dermatology for their assistance and cooperation with in vivo testing, useful discussions and assistance in using the Lucid Vivascope 1000. We thank James Howard of MIT Lincoln Laboratory for the many experiments he performed in perfecting the scission process. This research was supported by grants from Massachusetts Institute of Technology Lincoln Laboratory, and NIH, with additional support from Massachusetts General Hospital and CIMIT.
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