Multistep Photoluminescence Decay Reveals Dissociation of Geminate Charge Pairs in Organolead Trihalide Perovskites

Charge carrier dynamics in organolead iodide perovskites is analyzed by employing time‐resolved photoluminescence spectroscopy with several ps time resolution. The measurements performed by varying photoexcitation intensity over five orders of magnitude enable separation of photoluminescence components related to geminate and nongeminate charge carrier recombination and to address the dynamics of an isolated geminate electron–hole pair. Geminate recombination dominates at low excitation fluence and determines the initial photoluminescence decay. This decay component is remarkably independent of the material structure and experimental conditions. It is demonstrated that dependences of the geminate and nongeminate radiative recombination components on excitation intensity, repetition rate, and temperature, are hardly compatible with carrier trapping and exciton dissociation models. On the basis of semiclassical and quantum mechanical numerical calculation results, it is argued that the fast photoluminescence decay originates from gradual spatial separation of photogenerated weakly bound geminate charge pairs.     

Brazilin-Toluidine Blue O and Hematoxylin-Darrow Red Methods for Brain and Spinal Cord

Tissue fixed in 10% formalin, formalin-95% ethanol 1:s CaCO₂ or phosphate buffer neutralized formalin, or methanol-chloroform 2:1, was dehydrated and embedded in paraffin or double-embedded by infiltration in 1% celloidin followed by a chloroform-paraffin sequence. Sections were attached to slides with either albumen or gelatine adhesive and processed throughout at room temperature of 24-26 C. For either method, mordanting 30-60 min in 1% iron alum was followed by a 10 min wash in 4 changes of distilled water. For brazilin-toluidne blue O, myelin was stained for 20-60 min, depending upon section thickness, in a self-differentiating solution consisting of: 0.15% Li₂CO₃ 75 ml; 6% brazilin in 95% ethanol, 25 ml; and NaIO₃ 75 mg. After a thorough washing, Nissl material was stained for 3-8 min in a solution consisting of: 0.1 M acetic acid, 90 ml; 0.1 M sodium acetate, 10 ml; and 1% toluidine blue 0, 2.5 ml. For hematoxylin-Darrow red, myelin was stained for 2-6 hr in a self-differentiating solution consisting of: 0.15% Li₂,CO₃ 95 ml; 10% hematoxylin in 95% ethanol, 5 ml; and NaIO₃ 25 mg. After a thorough washing, Nissl material was stained for 20 min or less in a solution consisting of: 0.1 M acetic acid, 90 ml; 0.1 M sodium acetate, 10 ml; Darrow red, 25 mg. This mixture was first boiled, cooled to room temperature and filtered. In both methods, washing, dehydration, clearing, and mounting completed the process. In the brazilin-toluidine blue technic, myelin sheaths were stained reddish purple; neuronal nuclei light blue with dark granules of chromatin; nucleoli dark blue; and cytoplasm blue with dark blue Nissl granules. In the hematoxylin-Darrow red procedure, myelin sheaths were blue-black; nuclei light red with dark granules of chromatin; nucleoli almost black; and cytoplasm red with bright red Nissl granules.     

Use of Gallocyanin as a Myelin Stain for Brain and Spinal Cord

Tissue fixed in 10% formalin, formol saline, CaCO₃ or phosphate buffer neutralized formalin, Baker's formol calcium, Cajal's formol ammonium bromide, formalin-95% ethanol 1:9, formalin-methanol 1:9, Lillie's methanol-chloroform or Salthouse's formol cetyltrimethylammonium bromide was dehydrated and embedded in paraffin. Sections were attached to slides with either albumen or gelatine adhesive and processed throughout at room temperature of 22-25 C. Mordanting 30-60 min in 1% iron alum was followed by a 10 min wash in 4 changes of distilled water. Myelin was stained in a gallocyanin self-differentiating solution for 1-2.5 hr; thick sections requiring the longer time. The staining solution (pH approximately 7.4) consisted of Na₂CO₃, 90 mg; distilled water, 100 ml; gallocyanin, 250 mg; and ethanol, 5 ml. The ethanol was added to this mixture last, and after the other ingredients had been boiled and then cooled to room temperature. After a staining and thorough washing, Nissl granules were stained for 5-10 min in a solution consisting of: 0.1 M acetic acid, 60 ml; 0.1 M sodium acetate, 40 ml; methyl green, 500 mg. Washing, dehydration, clearing and mounting completed the process. Myelin sheaths were stained dark violet; neuronal nuclei, light green with dark granules of chromatin; nucleoli of motor cells and erythrocytes, dark violet; cytoplasm, green with dark green Nissl granules. The simple and reliable method can be adapted easily for use with automatic tissue processors.     

Supravital Staining and Fixation of Brain and Spinal Cord by Intravascular Perfusion

Forty single and 13 combinations of dyes were tested for concomitant supravital staining and fixation of brain and spinal cord of rats, cats and squirrel monkeys by intravascular perfusion in 3 steps: (1) 60 or 80 ml of physiological saline containing 40 mg/100 ml of NaNO₂ as a vasodilator; (2) 250 or 550 ml of stain-fixative solution consisting of either: A—2 parts of dye solution in a concentration from 0.001% to 0.05% dissolved in saline containing 40 mg/100 ml of NaNO₂ and 1 part undiluted formalin; or B—2 parts of dye solution in a concentration from 0.001% to 0.05% dissolved in distilled water acidified with 1.5 ml of glacial acetic acid per 100 ml of water, and 1 part undiluted formalin; and (3) 100 or 150 ml of 6% dextrose in distilled water. Complete staining and fixation was accomplished in 53 min for rats and 41 min for cats and monkeys. Brains and spinal cord were frozen sectioned, and the cut surfaces of the frozen tissue were photographed similar to the procedure described by Gasteiger et al